Next Article in Journal
BECLIN1: Protein Structure, Function and Regulation
Next Article in Special Issue
The Impact of Glucose-Lowering Drugs on Sarcopenia in Type 2 Diabetes: Current Evidence and Underlying Mechanisms
Previous Article in Journal
Dynamic Evaluation of Circulating miRNA Profile in EGFR-Mutated NSCLC Patients Treated with EGFR-TKIs
Previous Article in Special Issue
Muscle Homeostasis and Regeneration: From Molecular Mechanisms to Therapeutic Opportunities
 
 
Search for Articles:
Title / Keyword
Author / Affiliation / Email
Journal
Article Type
 
 
Advanced Search
 
Section
Special Issue
Volume
Issue
Number
Page
 
Journals
Cells
Volume 10
Issue 6
10.3390/cells10061521
cells-logo
Submit to this Journal Review for this Journal Propose a Special Issue
► Article Menu

Article Menu

share Share announcement Help format_quote Cite question_answer Discuss in SciProfiles thumb_up
...
Endorse textsms
...
Comment
first_page
settings
Order Article Reprints
Font Type:
Arial Georgia Verdana
Font Size:
Aa Aa Aa
Line Spacing:
Column Width:
Background:
Review

Ion Channel Gene Mutations Causing Skeletal Muscle Disorders: Pathomechanisms and Opportunities for Therapy

by
Lorenzo Maggi
1,*,
Silvia Bonanno
1,
Concetta Altamura
2 and
Jean-François Desaphy
2
1
Neuroimmunology and Neuromuscular Disorders Unit, Fondazione IRCCS Istituto Neurologico Carlo Besta, 20133 Milan, Italy
2
Department of Biomedical Sciences and Human Oncology, School of Medicine, University of Bari Aldo Moro, 70124 Bari, Italy
*
Author to whom correspondence should be addressed.
Cells 2021, 10(6), 1521; https://doi.org/10.3390/cells10061521
Submission received: 4 May 2021 / Revised: 3 June 2021 / Accepted: 10 June 2021 / Published: 16 June 2021
(This article belongs to the Special Issue Muscle Homeostasis and Regeneration: From Molecular Mechanisms to Therapeutic Opportunities)
Browse Figures
Versions Notes

Abstract

:
Skeletal muscle ion channelopathies (SMICs) are a large heterogeneous group of rare genetic disorders caused by mutations in genes encoding ion channel subunits in the skeletal muscle mainly characterized by myotonia or periodic paralysis, potentially resulting in long-term disabilities. However, with the development of new molecular technologies, new genes and new phenotypes, including progressive myopathies, have been recently discovered, markedly increasing the complexity in the field. In this regard, new advances in SMICs show a less conventional role of ion channels in muscle cell division, proliferation, differentiation, and survival. Hence, SMICs represent an expanding and exciting field. Here, we review current knowledge of SMICs, with a description of their clinical phenotypes, cellular and molecular pathomechanisms, and available treatments.

1. Introduction

Primary ion channelopathies are rare diseases caused by mutations in genes encoding ion channel subunits. The first ion channelopathy was identified in hyperkalemic periodic paralysis (hyperPP), a genetic disease affecting exclusively skeletal muscles and caused by mutations in the SCN4A gene encoding the alpha subunit of voltage-gated sodium channel Nav1.4, which expression is limited to the skeletal muscle fiberfibers [1]. The discovery of CFTR gene mutations linked to cystic fibrosis was contemporaneous, but the chloride channel activity of the CFTR protein was not known yet. Thus, skeletal muscle ion channelopathies (SMICs) have been a paradigm for the discovery of ion channelopathies affecting all organs. Considering the importance of ion channels in modulating membrane electrical activity, the diseases related to ion channel mutations were characterized by disturbance of muscle fiber excitability, such as the non-dystrophic myotonias (NDM) presenting with muscle stiffness (myotonia) due to membrane over-excitability and the periodic paralysis (PP) showing episodes of paralysis due to sarcolemma inexcitability.
Yet, with the development of more advanced technologies, including next-generation and whole-exome sequencing, it appears more and more evident that ion channel mutations may cause further muscle phenotypes, including progressive myopathies, altering muscle structure, thereby highlighting a significant role of ion channels in muscle cell division, proliferation, differentiation, and survival.
Hence, SMICs represent a large heterogeneous group of rare genetic disorders resulting in long-term disabilities with a relevant burden to the patients, families and National Health Care Services. SMICs usually present in childhood, but late-onset cases have been reported. SMICs diagnosis requires a high clinical suspicion, being mainly based on the detailed clinical history and neurological examination, followed by molecular confirmation.
Here, we review current knowledge of SMICs, with a description of clinical phenotype, cellular and molecular pathomechanisms, and available therapies. We also included the description of two neuronal ion channelopathies (TRPV4 and KCNA1 genes), which may have pronounced effects on skeletal muscles. Ion channel gene mutations and related clinical muscular phenotypes are summarized in Table 1.

2. Skeletal Muscle Sodium Channelopathies

Voltage-gated sodium channels are responsible for the upstroke of action potentials and modulate firing frequency in excitable cells. From the first week of life, the main sodium channel expressed in skeletal muscles is Nav1.4, which alpha-subunit is encoded by SCN4A. The spectrum of SCN4A-related myopathy spans from the complete loss of the channel (null mutations) to a gain of function (missense mutations) through various degrees of altered function, resulting in highly heterogeneous clinical presentation, mainly characterized by myotonia or PP, which represents a continuum in the clinical spectrum (Figure 1). In particular, the most frequent phenotype is paramyotonia congenita (PMC), followed by sodium channel myotonia (SCM), while PP is less frequent [2,3,4].

2.1. Hyperkalemic Periodic Paralysis, Paramyotonia Congenita, and Sodium Channel Myotonia

The SCN4A mutations were first identified in patients suffering from the autosomal dominant hyperPP [1,5,6]. HyperPP is characterized by episodes of flaccid paralysis, leading to muscle weakness, generally associated with ictal hyperkalemia (>4.5 mEq/L). The paralytic attack can last for up to 2 h. Loading of K+ can provoke or worsen an attack; other triggers include rest after exercise, fasting, and cold exposure. Emotional stress and pregnancy can increase the likelihood of attacks. The first attack is generally experienced during the first decade of life. Permanent weakness may progressively take place after the fourth decade. Myotonia is experienced by many hyperPP patients [4,7].
PMC is allelic to hyperPP, being caused by autosomal dominant SCN4A missense mutations [8]. PMC is mainly characterized by paradoxical myotonia that typically worsens with exercise and shows no warm-up phenomenon, which is usually detected in myotonia congenita (MC). In addition, episodes of flaccid paralysis can represent a relevant feature in patients with PMC [4,9]. Triggers of myotonia are similar to those reported in hyperPP. Thus, PMC and hyperPP are considered as a continuum manifesting as pure PMC, pure hyperPP, or intermediary PMC plus hyperPP. Other SCN4A mutations are responsible for SCM, which can be distinguished from PMC by the lack of both paradoxical myotonia and episodes of flaccid paralysis [10]. In addition, PMC differs from SCM for earlier onset, higher cold-sensitivity, and more frequent involvement of hand and cranial muscles [4,9,11]. Symptoms in SCM are quite variable in severity and may show specific features; thus, various subgroups have been described, such as myotonia fluctuans (moderate), myotonia permanens (severe), acetazolamide-responsive myotonia, potassium-aggravated myotonia, and painful myotonia. In addition, myotonia permanens can be associated with harmful neonatal symptoms, such as severe neonatal episodic laryngospasm (SNEL) [12].
It needs to be noted that some mutations can lead to different phenotypes, even in the same kindred. Again, this argues for a continuum of these disorders and suggests the importance of disease-modifying genes. As more mutations are identified, many variable phenotypes are emerging, such as myotonia with normokalemic/hypokalemic PP, PP associated with myotonia instead of paradoxical myotonia, or the presence of myopathic traits [13,14,15,16,17,18].
Up to date, about seventy missense SCN4A mutations were found to be linked to these diseases, half of which were functionally characterized. Patch-clamp and computational experiments have clearly demonstrated that myotonia is due to a gain of function of the mutated Nav1.4 channel, mainly through the defects of inactivation and enhancement of activation [19]. Thus, the mutated channel activates more quickly or inactivates more slowly or incompletely, as compared to the wild-type channel. Recovery from inactivation can be accelerated. The voltage dependence of activation and inactivation can also be shifted toward potentials favoring channel activity [19]. These effects may be temperature-dependent, in accord with the cold sensitivity of the patients. The resulting increased influx of sodium ions rends the muscle fibers more excitable and inclined to generate high-frequency firing of action potentials that persists after the end of motoneuron stimulation. Such after-discharges cause a delay in relaxation and muscle stiffness. Spontaneous firing can also occur in the absence of a nervous stimulus, which can induce muscle spasms, fasciculation, and cramps. Continuous activity can induce muscle hypertrophy.
The voltage-gated sodium channels can enter two inactivated states: the fast one normally occurring on a millisecond time scale and the slow one occurring on a second time scale. The mutations that produce a persistent inward sodium current due to incomplete fast inactivation and impair Nav1.4 slow inactivation are more inclined to induce PP than myotonia [20,21]. In these conditions, the persistent depolarization of sarcolemma may, in turn, inactivate the wild-type sodium channels, rendering the cell inexcitable with flaccid paralysis.
Treatment of myotonia relies on the use of frequency-dependent sodium channel blockers that reduce excessive action potential firing in the overexcited muscle fibers. The cardiac antiarrhythmic, mexiletine, has been granted as an orphan drug for myotonic syndromes after the success of randomized clinical trials (RCT) and is widely recognized as the first drug of choice in myotonia [22,23]. However, up to 30% of myotonic patients have an unsatisfactory response to mexiletine because of a suboptimal response or side effects [24,25]. The antiepileptic drug lamotrigine was beneficial in an RCT, and it is now considered the second choice in several countries [26,27]. Moreover, the antiarrhythmic flecainide and propafenone were proved useful in mexiletine-refractory patients carrying specific SCN4A mutations, suggesting the possibility of defining a mutation-driven pharmacological strategy [28,29,30,31]. It is feasible to introduce the marketed sodium channel blockers for repurposing myotonia [32,33,34,35] or developing new derivatives with increased efficacy [36,37].
Intuitively, the use of sodium channel blockers would not be recommended in hyperPP because they might worsen the fiber inexcitability. Intravenous insulin/glucose or inhaled salbutamol can be used to abort a paralytic attack because they induce the hyperpolarization of muscle membrane through stimulation of Na+-K+ pump. Prophylaxis of recurrent attacks is based on the use of carbonic anhydrase inhibitors (CAI), acetazolamide (ACZ) or dichlorphenamide, and/or thiazide diuretics to maintain the low blood level of potassium. The CAI can enhance the activity of Ca2+-activated K+ (BK) channels and ClC-1 chloride channels in muscle membranes [38,39]. The benefits of dichlorphenamide in hyperPP were confirmed in an RCT [40]. Recommendations and guidelines on diagnosis and treatment of NDM and PP were previously detailed by Stunnenberg et al. and Statland et al., respectively [41,42].

2.2. Hypokalemic Periodic Paralysis Type 2

Hypokalemic PP type 2 (hypoPP2) is a distinct syndrome caused by the missense SCN4A mutations [43,44]. It is characterized by episodes of focal (limb) or more frequently generalized flaccid paralysis, with a longer duration than hyperPP, lasting more than 2 h up to days, with concomitant hypokalemia (<3.5 mEq/L), and absence of myotonia [4,7,41]. The attack triggers include carbohydrate or alcohol ingestion and rest after vigorous exercise. The disease onset is variable, occurring in between the first and third decade of life. The frequency and severity of attacks generally decrease after the third decade, but permanent weakness and progressive myopathy may develop in the proximal muscles of the lower limbs.
Ten SCN4A mutations have been linked to hypoPP2, which accounts for about 20% of all hypoPP cases. Indeed, around 60% of hypoPP cases are caused by CACNA1S mutations (hypoPP type 1, hypoPP1) [2,3]. All the hypoPP are inherited with an autosomal dominant trait. Interestingly, most SCN4A and CACNA1S hypoPP mutations share a similar molecular defect [45]. These mutations are all sited in the voltage-sensing S4 segments of the channel, neutralizing a positive charge through the substitution of an arginine residue [45]. Functional studies suggested that the mutations induce various degrees of loss of function, but it appeared that the most likely pathomechanism consists in the creation of an aberrant pore beside the normal ion conduction pathway [45]. This so-called gating pore permits small leakage of cationic currents at rest, favoring membrane depolarization in hypokalemia that, in turn, inactivates sodium channels and rends the fiber inexcitable.
Oral or intravenous potassium loading is the only way to abort a paralytic attack in hypoPP. For prophylaxis, the use of ACZ or dichlorphenamide is the preferred strategy. Their mechanism of action in hypoPP is not well defined but might involve systemic acidosis and BK channel activation. The K+-sparing diuretics, such as eplerenone or spironolactone, can be used in addition or alternative to CAI. Evidence has been provided that suggests a relationship between genotype and response to CAI, with hypoPP2 often less responsive than hypoPP1 and arginine-to-histidine mutations more responsive than other mutations, highlighting again the importance of genotyping for better addressing therapy [46].

2.3. Congenital Myasthenia and Congenital Myopathy Related to SCN4A

Very rare SCN4A mutations producing a loss of function of Nav1.4 channels have been associated with congenital disorders. They include congenital myasthenic syndrome (CMS) with brief and abrupt attacks of muscle weakness since birth, which may eventually lead to respiratory arrest; other mutations induce neonatal hypotonia and congenital myopathy; finally, some mutations may produce severe fetal hypokinesia leading to death in utero or soon after birth [47,48]. These mutations are inherited in an autosomal recessive mode. The presence of two mutations producing a partial loss of Nav1.4 function leads to congenital myasthenia. A heterozygous null mutation in the SCN4A gene is associated with neonatal hypotonia and congenital myopathy; the concomitance of two null mutations induces neonatal death [19,33]. ACZ has provided some benefits in some patients, but its mechanism of action is still unknown [49,50].

3. Calcium Channel-Related Myopathies

Calcium ions play a central role in regulating muscle function. In the short term, calcium ions released by the sarcoplasmic reticulum (SR) in response to electrical excitation of the cell membrane trigger muscle fiber contraction. In the long term, calcium ions modulate gene expression, contributing to muscle plasticity, which is the ability of muscle fibers to adapt their mass and metabolism to functional needs. Thus, calcium ion-permeable channels and associated proteins are critical for the maintenance of the contraction apparatus of muscle. Deleterious mutations in these proteins cause diseases characterized by alteration of excitability, excitation–contraction coupling, and skeletal muscle structure (Figure 2).

3.1. CACNA1S-Related Disorders

The CACNA1S gene codes for the CaV1.1 channel, the pore-forming subunit of the dihydropyridine receptor (DHPR), a voltage-gated L-type Ca2+ channel located on the T-tubule, which activates the type 1 ryanodine receptor (Ryr1) calcium channel sited in the SR, during excitation–contraction coupling.
Different phenotypes were reported in patients with mutations in CACNA1S, such as hypoPP1, congenital myopathy, and malignant hyperthermia susceptibility (MHS).

3.1.1. Hypokalemic Periodic Paralysis Type 1

The main phenotype caused by autosomal dominant mutations in CACNA1S is hypoPP1) [51]. The frequency of attacks is highly variable, from daily to once in a lifetime. The age of onset is usually earlier, and the duration of paralytic episodes longer in hypoPP1 than hypoPP2 [7]. Muscle strength is normal between attacks; however, permanent muscle weakness, regardless of the episodes of paralysis, is frequently observed in later disease stages of hypoPP1, while it is not reported in hypoPP2. In this regard, a recent paper on a large cohort of hypoPP1 patients showed that at least one-third developed permanent weakness with ageing [52].
Carbohydrate load and rest after a strenuous exercise are the most common triggers for hypoPP, although attacks may occur spontaneously. Muscle biopsy in hypoPP1 may show non-rimmed vacuoles, whereas, in hypoPP2, vacuoles occur as frequently as tubular aggregates [7]. However, hypoPP diagnosis is essentially based on medical history and then confirmed by molecular analysis. ACZ is the most common treatment choice for hypoPP, in particular for type 1 [46]. Recently, two randomized, double-blind, placebo-controlled trials showed a reduction of attack frequency with dichlorphenamide [40].
Missense mutations causing hypoPP affect highly conserved arginine residues of the S4 voltage-sensing domains of the CaV1.1, resulting in aberrant gating pore currents leading to paradoxical depolarization of the membrane in low potassium conditions and inexcitability [45,53,54].
Two mutations, p.R528H and p.R1239H, occur in nearly 80% of patients with hypoPP1 in England and The Netherlands [2,3].

3.1.2. Calcium Channel-Related Congenital Myopathy

Autosomal dominant or recessive mutations in CACNA1S have been detected through exome sequencing in seven families manifesting a congenital myopathy [55]. Patients presented with antenatal/congenital or early-onset generalized, predominantly axial muscle weakness. Ophthalmoplegia was detected in about one-third of the patients. Notably, one patient also developed PP. Histological analysis showed features resembling core and centronuclear myopathies. Taken together, all these features were suggestive of congenital myopathies. Notably, congenital myopathies were mostly considered as disorders of excitation–contraction coupling and impaired calcium handling [56]. There is no genotype–phenotype correlation in those patients with CaV1.1 mutation-induced congenital myopathy. Both dominant and recessive mutations caused a decrease in DHPR function in skeletal muscle, with a decrease in protein level and a relevant impairment of Ca2+ release induced by the sarcolemma depolarization in cultured myotubes. A further case of congenital myopathy with ophthalmoplegia has been reported by Hunter and collaborators [57]; two additional severe cases with fetal akinesia leading to premature termination of pregnancy at 26 weeks of gestation or death after 10 days of were reported by Ravenscroft and collaborators [58]. Three Turkish siblings carrying homozygous CACNA1S mutation presented a congenital myopathy with additional features, including cognitive delay, pes equinovarus deformity, and neurogenic changes at muscle biopsy [59].

3.2. STAC3-Related Disorder

EC coupling in skeletal muscles operates through the triad junctions, where the voltage sensor CaV1.1, through its β1a subunit, physically interacts with the Ryr1 calcium release channel. Recently, the STAC3 (SH3 and cysteine-rich domain 3) protein consisting of three scaffold proteins was found to be another key component of the skeletal muscle EC coupling [60]. STAC3 is specifically expressed in skeletal muscles, where it binds to Cav1.1 in the triads, and its inactivation generates skeletal muscle paralysis within the framework of conserved muscle differentiation and NMJ formation, indicating that the mechanism is altered downstream muscle excitation [61,62]. Recently, a homozygous missense mutation, p.W284S of human Stac3 (c.1046G>C), was identified in a cohort of five families (5 individuals affected and 13 unaffected) presenting a rare autosomal recessive congenital myopathy [62]. The disease was initially described in 21 Lumbee Native Americans, thus called “NAM,” Native American Myopathy, also known as Bailey-Bloch congenital myopathy (MYPBB) [63,64,65]. The symptoms of NAM usually occur at birth or in the first years of life with facial involvement (ptosis, downturned corners of the mouth, cleft palate), bone and joint deformities (arthrogryposis, scoliosis, and short stature), MHS, congenital weakness, and delayed motor milestones. Premature death occurs by the age of 18 in 6%–30% of the cases [62,66]. Recently, the homozygous p.W284S mutation was found in 2 siblings from Qatar, and the compound heterozygous for the p.W284S and a 4-bp deletion was described in other two siblings from Puerto Rico [67], all of the patients exhibiting the NAM phenotype. In addition, 18 patients of African, Middle Eastern, and South American ancestry presenting symptoms ranging from severe prenatal/neonatal onset to slowly progressive congenital myopathy (6 months–22 years old) were found homozygous or compound heterozygous for the p.W84S mutation. Thus, the p.W284S mutation is not restricted to the Native American population [68]. The first NAM-affected patient of Turkish origin carries two heterozygous variants (c.862A>T; p.K288* and c.432+4A>T), close to but not into the p.W284S region of the STAC3 gene [69]. The STAC3 SH3-1 domain is highly conserved throughout species and is the site of all the NAM causative Stac3 variants to date [66,70]. This domain interacts with the II-III loop Cav1.1 and is crucial for EC coupling. Several in vitro and in vivo studies demonstrated that Stac3 operates as a chaperone for CaV1.1 and modulates the L-type calcium currents [60]. Lastly, it has been speculated that Stac3 directly binds to Ryr1, which possibly constitutes the long-sought physical link between CaV1.1 and Ryr1 [71]. Yet, further evidence is needed to demonstrate the existence of this binding site and its therapeutic implications in CaV1.1/ Ryr1/STAC3 channelopathies.

3.3. STIM1 and ORAI1-Related Disorders

Store-operated Ca2+ entry (SOCE) is the process by which calcium depletion in the endoplasmic or sarcoplasmic reticulum stimulates extracellular Ca2+ influx through the plasma membrane [72]. This calcium current is mediated by the calcium release-activated calcium modulator 1 (ORAI1) and the stromal interaction molecule type 1 (STIM1), which constitute the Ca2+ release-activated Ca2+ (CRAC) channels [73,74]. ORAI1 is a four alpha-helical transmembrane protein forming the pore unit in the sarcolemma; its activation is mediated by the direct interaction with STIM1, a single-span transmembrane protein situated on the SR membrane where it senses Ca2+ depletion [75,76]. Regulation and function of the CRAC channel have been largely investigated, highlighting their relevance in fundamental cellular processes such as gene transcription, cellular metabolism, vesicle trafficking, muscle contraction, and myoblasts development [77,78,79]. Due to their crucial role in calcium signaling, mutations in STIM1 and ORAI1 are associated with abnormal SOCE and multi-systemic clinical phenotypes, ranging from immune system dysregulation to hematological defects and, notably, different forms of muscle involvement depending on the loss- or gain-of-function mutations of the genes.
Loss-of-function mutations in ORAI1 and STIM1 result in suppressed protein expression, thus abolishing SOCE. They are very rare, all inherited in an autosomal recessive manner, and constitute the “CRAC channelopathies” that present with a homogeneous syndromic phenotype characterized by neonatal immunodeficiency with recurrent severe infections due to defective lymphocyte activation, ectodermal dysplasia (altered tooth enamel, anhidrosis), autoimmune neutropenia and thrombocytopenia, encephalopathy and seizures, along with congenital non-progressive muscular hypotonia. The myopathy in patients with ORAI 1 and STIM 1 loss-of-function mutations is characterized by delayed motor milestones, proximal lower limb weakness, nasal speech, generalized hypotonia with atrophy of type 2 fibers, and reduced fatigue resistance [74]. Missense mutations in ORAI1 impair but not abolish ORAI1 protein expression [80,81]; however, they cause a severe clinical CRAC channelopathy spectrum. In contrast, missense mutations in the C-terminus of STIM1, which may allow a minimal residual SOCE, present with a later onset and a milder phenotype [82,83].
Contrarily to loss-of-function mutations, different gain-of-function (GoF) mutations in ORAI1 and STIM1 result in the activation and increased SOCE. They are inherited in an autosomal dominant manner, constituting rare clinical phenotypes with a wide disease spectrum. The complex Stormorken syndrome (STRMK) is characterized by bleeding diathesis, thrombocytopenia, congenital miosis, ichthyosis, asplenia, tubular aggregate myopathy (TAM), small stature with syndromic facial features, and cognitive impairment [84,85]. However, GoF mutation in ORAI1 and STIM1 might also result in the York platelet syndrome [86], showing thrombocytopenia, bleeding diathesis, and muscle weakness until isolated TAM [87]. TAM is a progressive muscle disorder characterized by subsarcolemmal basophilic inclusions, stained red on modified Gomori trichrome, positive to NADH and negative for SDH reactions [88]. It remains unclear how tubular aggregates (TA) form, but it has been suggested that constitutive Ca2+ loading may result in misfolding and aggregation of SR proteins [89], especially in type II atrophic fibers [90]. Tubular aggregates are not specific for TAM, as they may also appear in congenital myasthenic syndrome caused by DPAGT1 and GFPT1 mutations [91,92], in hypoPP [93]. STIM1 is the major gene responsible for TAM (TAM type 1). STIM1-EF hands at the N-terminus coordinate Ca2+-binding and maintain STIM1 in an inactive conformation. At least eight mutations in the EF hands have been reported in the His109 and Phe108 residues, a potential TAM mutation hotspot [94,95,96,97]. TAM phenotype is clinical heterogeneous ranging from slowly progressive proximal muscle weakness predominantly affecting the lower limbs, with adult onset (>35 year), to myalgia only. Serum creatine kinase is usually elevated, and patients may develop eye movement disabilities and joint contractures during disease progression [74,94,98]. Notably, the same STIM1 mutations can also be responsible both for the STRMK [89,90,99] and the York syndrome [86], emphasizing how all these conditions represent a continuum. Slowly progressive TAM with elevated creatine phosphokinase (CPK) levels might be related even to GoF mutations in ORAI1 (TAM type 2) transmembrane domains, which are sometimes accompanied by miosis constituting an STRMK-like syndrome [89,100,101,102].
A few CRAC channel modulators are currently in a clinical trial, mainly for psoriasis treatment [103]; the continuous advancement in the comprehension of the STIM1–ORAI1 interaction and molecular regulation is expected to underscore new potential therapeutic targets to modulate SOCE and restore aberrant Ca2+ homeostasis.

3.4. RYR1-Related Disorders

The RYR1 gene is located on chromosome 19q13.1 and encodes RyR1, the principal sarcoplasmic reticulum calcium release channel playing a fundamental role in the EC coupling process [104].
RYR1-related myopathies represent the most common form of congenital myopathy [105]. Phenotypes associated with Ryr1 gene mutations include a wide range of diseases with some overlaps, hence representing a continuum in the clinical spectrum [106,107,108,109,110,111,112]. Hence, a relevant issue in Ryr1 gene analysis is the definition of pathogenicity of novel variants, in particular considering the great clinical variability associated with RYR1 mutations. In this regard, the correlation of genetic findings together with clinical, histological, and muscle imaging data may be helpful. All these diseases show impaired intracellular calcium homeostasis through different pathomechanisms, such as leaky Ryr1 channels, reduced Ryr1 expression, impaired Ryr1 interdomain interactions, increased sensitivity to modulators/activators, or impaired excitation–contraction coupling [113]. The impaired calcium homeostasis may cause secondary cellular dysfunction with increased oxidative stress, abnormal post-translational modifications, mitochondrial dysfunction, and altered protein–protein and protein–ligand interactions [113].

3.4.1. RYR1-Related Congenital Myopathies

Autosomal dominant mutations in RYR1 have been associated with the core myopathies (CM), the most frequent congenital myopathy subtype. Most of the mutations are missense, with a few small deletions and duplications [114,115,116,117,118,119,120]. Core myopathies include central core disease (CCD) and multiminicore myopathy, characterized by the presentation of cores and minicores, respectively, in the muscle fibers and defined as distinct areas of myofibrillar disruption lacking mitochondria. Patients with dominant core myopathy typically present at birth or first years of life with muscle hypotonia, proximal weakness, mild cranial involvement, and orthopedic complications, as contractures, congenital hip dislocation and scoliosis [121,122].
More recently, recessive mutations in RYR1 have been described in patients with CCD or centronuclear myopathy, another congenital myopathy subtype [106,121,123,124].
Mutations in RYR1 were associated with the specific subtypes of congenital myopathy, such as congenital fiber-type disproportion and rod-core myopathy [123,125]. The frequency of recessive mutations was similar to that of dominant ones [106]. Dominant mutations are usually associated with milder phenotypes, whereas patients with recessive inheritance show earlier onset, more pronounced weakness and motor function disabilities. Bulbar and extraocular muscle involvement was almost exclusively reported in the recessive cases [106].
Although there are three hotspot regions (N-terminal residues 1–614, central residues 2163–2458, and C-terminal pore/transmembrane residues 4136–4973), autosomal dominant RYR1 mutations in CCD and MHS may cover the entire gene [106,117,126]. In recessive RYR1-related myopathies, mutations are widespread across the entire RYR1 gene, usually identified as a combination of a null mutation and a missense mutation or two missense mutations, with the variable clinical severity [106,123,127,128].
Recently, an additional congenital myopathy phenotype has been described, which is characterized by irregular areas of myofibrillar disorganization with a reddish-purple granular material deposition with uneven oxidative stain and devoid of ATPase activity; this novel histological entity has been named dusty core myopathy (DCM) and is clinically indistinguishable from the aforementioned recessive core myopathy cases [111]. The authors of [111] suggested that DCM represents the most common CM associated with recessive RYR1 mutations.
Fetal akinesia syndrome represents the most severe phenotype associated with RYR1 mutations; it has been reported in patients carrying autosomal dominant or recessive RYR1 mutations and with histological diagnosis of CCD [129].

3.4.2. Malignant Hyperthermia Susceptibility

MHS is characterized by muscle hypermetabolism that is triggered by anesthetic agents, particularly volatile gases (e.g., sevoflurane, desflurane) and depolarizing muscle relaxants (succinylcholine), which cause muscle rigidity and hyperthermia [130]. The incidence of MHS is estimated to be as high as one in 2000 Western Europeans, one event in every 50,000 anesthesia uses in adults, and one event in every 10,000 anesthesia uses in children. MHS represents a medical emergency and is lethal in about 70% of cases if not treated in time with supportive care measures and dantrolene, which antagonizes the excessive intracellular release of calcium by the Ryr1. Autosomal dominant mutations in RYR1 represent by far the most frequent cause of MHS, followed by mutations in CACNA1S, accounting for about one-fourth of cases [131]; in addition, a few cases have been reported in association with mutations in the STAC3 gene [132].
The in vitro contracture test on muscle biopsy tissue is the definitive diagnostic test for MHS. It cannot be routinely performed because it requires specific skills and is not possible in an emergency. In addition, false-positive diagnoses have been reported, and an underlying myopathy may produce a positive contraction test [133]. Genetic testing is also challenging, as about half of the MHS patients have no detected mutations in RYR1, CACN1AS, or STAC3.
The King Denborough syndrome, which is characterized by MHS combined with a dysmorphic syndrome, was found to be associated with RYR1 mutations [134].

3.4.3. Exertional Rhabdomyolysis

Recently, mutations in RYR1 were found in one-third of unexplained rhabdomyolysis and/or exertional myalgia [107]. Patients usually presented between 3 and 45 years of age with rhabdomyolysis and/or exertional myalgia (n = 12), whereas isolated exertional myalgia was much less frequent. The most frequent triggers for rhabdomyolysis were exercise and heat [107]. Muscle strength was normal, and muscle biopsies revealed non-specific changes in most of the cases. RYR1 mutations/variants detected in these cases have been previously reported in MHS or were localized to known MHS mutational hotspots, although only one out of the 24 reported patients had the MHS history [107].

3.4.4. Other Ryr1-Related Phenotypes

Predominant axial myopathy had been reported in 12 RYR1-mutated patients, presenting between the third and eighth decade of life and suggesting RYR1 as a possible cause of idiopathic camptocormia or bent spine syndrome [108,135]. Serum creatine kinase levels were normal or moderately elevated, and muscle imaging revealed the involvement of the lower paravertebral muscles and the posterior thigh. Muscle biopsy findings were described as discrete, with cores rarely reported. As for exertional rhabdomyolysis, RYR1 sequencing revealed heterozygous missense variants previously associated with MHS trait or localizing to known MHS mutational hotspots.
Dominant or recessive RYR1 mutations have been detected in four patients with late-onset atypical PP, both with and without congenital myopathy [112,136]. Myalgia and cramps were prominent features in all the patients. In this regard, the direct interaction between the Cav1.1 channel and Ryr1 in the context of the excitation–contraction coupling makes the overlapping phenotypes when one of them is mutated, manifested by episodes of paralysis or congenital myopathy. Of note, marked impairment of the normal Cav1.1– Ryr1 interaction was observed in RYR1-related PP and recessive type myopathies [110,136].

3.5. RYR3-Related Myopathy with Nemaline Bodies

The RyR3 isoform expression and its active role in mammalian muscle contractility after post-natal age are unclear [137,138]. To date, there is only one report describing the mutation in the RyR3 gene in a 22-year-old woman affected by nemaline myopathy (NEM3) [139]. The patient showed dysmorphic facial features (high-arched palate, facial weakness, and micrognathia), proximal weakness of lower limbs starting at the age of five, and normal CPK but the myopathic pattern in electromyography. Skeletal muscle biopsy revealed predominant atrophic type 1 fibers, increased internal nuclei, and abundant nemaline bodies. She presented compound heterozygous missense mutations in RYR3, which are classified as variants of uncertain significance, as the role of RyR3 in muscle pathology is yet to be clarified [139].

3.6. TRPV4 Channel Related Myopathies

Among the transient receptor potential (TRP) cation channels, the vanilloid subtype TRPV4 is one of the most abundantly expressed in skeletal muscle [140]. In mouse muscles, it was found in a fraction of muscle fibers located at the sarcolemma and myonuclei. The TRPV4 protein is ubiquitously expressed and forms calcium-permeable channels opened by cell swelling, mechanical stimuli, and a variety of endogenous lipids. Physiologically, it may contribute to mechanosensitive ion channels, and its activation may attenuate fatigue by allowing Ca2+ influx [141,142]. Mutations in TRPV4 can induce a number of peripheral neuropathies with implications for skeletal muscles, such as hereditary motor and sensory neuropathy type 2C mainly presenting in the pediatric age (HMSN2C), scapuloperoneal spinal muscular atrophy (SPSMA), and congenital distal SMA [143,144,145,146]. The genotype-phenotype relationship appears quite complicated. First, a number of asymptomatic carriers have been observed in several affected kindred, suggesting a reduced penetrance of some mutations. Second, TRPV4 mutations can also cause skeletal dysplasias [147,148]. Surprisingly, a mutation previously found in a patient affected by autosomal dominant brachyolmia was detected in a patient suffering from HMSN2 [146,147]. Thus, it is now widely acknowledged that TRPV4 channelopathies can present with great phenotypic variability and overlapping features [149,150,151,152,153,154]. Interestingly, many of the mutations reported so far affect highly-conserved arginine residues located in the N-terminal ankyrin repeat domain (ARD), which is involved in oligomerization, intracellular trafficking, and interaction with other proteins [146,155]. Mutations located in other parts of the protein have been reported. The TRPV4 mutations linked to skeletal dysplasia were shown to cause a gain of function of the channel [147,148]. Regarding neuropathy-causing mutations, various molecular defects have been proposed, including the gain of function, loss of function, and formation of intracellular aggregates with reduced plasma membrane expression. Very recently, in vivo experiments in Drosophila and primary mouse neurons showed that the expression of a TRPV4 mutant causes neuronal dysfunction and axonal degeneration [156]. These effects were due to increased intracellular Ca2+ concentration, activation of a Ca2+/calmodulin-dependent protein kinase II, and impairment of axonal mitochondrial transport. Importantly, these effects were inhibited by TRPV4 blockers, which may suggest a promising therapeutic strategy. Noteworthy, little is known about the contribution of skeletal muscle TRPV4 channels to the diseases.
Besides peripheral neuropathies, a very recent study elegantly showed that skeletal muscle TRPV4 channels are involved in mechanically induced myotonia because the latter is inhibited by TRPV4 inhibitors or missing in muscles of TRPV4−/− mice [157]. The authors proposed that mechanical stimulation of muscle fibers induces the opening of TRPV4 channels, leading to sarcolemma depolarization that is normally dampened by ClC-1 chloride currents. In myotonic muscles, the defective ClC-1 chloride channel cannot counteract the TRPV4-induced depolarization that, in turn, triggers hyperexcitability [157].
All these studies suggest that TRPV4 blockers may provide promising therapies. Such drugs are currently in development and have proven to be safe and well-tolerated in humans [158].

3.7. Congenital Amyotrophy Related to CACNA1H (T-Type Channel)

Very recently, a female baby presenting with severe amyotrophy at birth was reported [159]. Whole exome sequencing revealed the presence of two compound heterozygous mutations in the CACNA1H gene, which encodes a T-type voltage-gated calcium channel (Cav3.2). This channel is expressed in central and peripheral nervous systems, including motor neurons, neuroendocrine glands, smooth muscles, heart and kidney. Mutations in this gene have been clearly linked to primary hyperaldosteronism, while polymorphisms may increase susceptibility to childhood absence epilepsy and idiopathic generalized epilepsy. In these diseases, the pathomechanism is likely explained by a gain of function in the Cav3.2 channel. Conversely, functional study of mutations causing congenital amyotrophy suggested a loss of function. Since the channel may be involved in myoblast differentiation and fusion during embryogenesis, it is possible that loss of function impaired normal muscle development.

4. Potassium Channel-Related Myopathies

Potassium channels constitute the larger and most variegated family of ion channels, being involved in most cell functions. Thus, mutations in K channel genes have been linked to many diseases affecting many organs and, in some cases, to multisystem diseases (Figure 3).

4.1. Andersen–Tawil Syndrome

Andersen–Tawil syndrome (ATS) is a very rare autosomal dominant disorder (prevalence of 1 per 1,000,000) characterized by a triad of PP, cardiac arrhythmias, and typical facial and skeletal malformations [160,161]. Cardiac arrhythmias include ventricular arrhythmia, prolonged QT interval at the ECG, and prominent U waves. Malformations include ocular hypertelorism, low-set ears, small mandible, scoliosis, fifth digit clinodactyly, syndactyly, short stature, and a broad forehead [162]. However, a great variety of symptoms has been reported, making the diagnosis quite challenging. In addition, only one symptom of the triad may be present; hence, ATS should always be considered in patients presenting with only PP [163]. ATS usually presents within the first two decades of life. Regarding skeletal muscle, episodic weakness occurs with normo-, hyper-, or hypokalemia. Permanent muscle weakness was reported in a few cases [164,165,166,167]. Myokymia has been observed in one patient [168]. ATS is a potentially fatal disorder due to the occurrence of ventricular arrhythmia, and early diagnosis is required for proper management [41].
Mutations in KCNJ2 encoding the inward-rectifying potassium channel Kir2.1 are responsible for about 60% of ATS cases (ATS type 1, also referred to as LQT7). This channel is expressed in skeletal muscle, heart, and bones, where it plays a role in stabilizing the resting membrane potential and contributes to cardiac action potential repolarizing phase. The ATS mutations induce a loss of function of Kir2.1 channels and consequent reduction of IK1 current in cardiomyocytes [169]. Many mutations are located in the binding site for phosphatidylinositol-4,5-biphosphate (PIP2), which is a known activator of Kir2.1 channels. Accordingly, several ATS mutations were shown to reduce PIP2 sensitivity [170,171,172,173]. However, other ATS mutations are distributed throughout the entire Kir2.1 protein, suggesting additional mechanisms. Indeed, some mutations were shown to impair intracellular trafficking [171,174]. Most of the ATS mutations exert a dominant negative effect on the wild-type channel subunit [169]. In addition, a mutation was shown to produce haploinsufficiency due to impaired synthesis or increased degradation [175].
Thus, the impairment of Kir2.1 channels logically accounts for the skeletal muscle and heart symptoms. In bones, experiments suggested that Kir2.1 is critical for osteoblastogenesis and bone morphogenetic protein signaling [176,177,178]. However, there is no clear correlation between the molecular defect and phenotypic variability, suggesting that other genes may influence the disease. One possible explanation resides in the capacity of Kir channels to form heteromultimeric channels [179,180]. Thus, the expression of the symptoms might depend on the expression balance between the various Kir subunits with respect to Kir2.1. Another possibility might be the occurrence of polymorphisms in other ion channel genes, including KCNQ1, KCNH2 and SCN5A, which may influence the cardiac phenotype [181,182].
Noteworthy, gain-of-function mutations in KCNJ2 have been linked to short QT syndrome [183,184].
Mutations of the KCNJ5-encoding Kir3.4 channel are found in about 15% of ATS cases (ATS type 2; LQT13) [162]. As for KCNJ2, KCNJ5 mutations may have incomplete penetrance, and the expression of symptoms is variable [168,185,186]. This channel is responsible for the IK(ACh) current in cardiomyocytes. A KCNJ5 mutation was shown to reduce IK(ACH) currents and to exert dominant negative effects on wild-type Kir3.4 and wild-type Kir2.1 channels [185,186].
The treatment of ATS may be challenging because of the need to address two distinct phenotypes—periodic paralysis and cardiac arrhythmias [161]. There is a risk that drugs beneficial to one organ may negatively affect the other. For cardiac arrhythmias, treatment includes the use of β-blockers such as propranolol. There are anecdotic observations of the positive effects of calcium or sodium channel blockers. In patients not responding to pharmacological treatment, the use of a pacemaker or an implantable defibrillator may be required. For PP, the treatment usually follows the guidelines for hypoPP or hyperPP, including the inhibitors of carbonic anhydrases such as ACZ and dichlorphenamide to reduce the frequency of attacks. However, muscle weakness exacerbation with ACZ has been reported in an ATS individual [187]. In the case of hypokalemic attacks, potassium supplementation may abort a paralytic attack while simultaneously shortening the QT interval. Potassium-sparing diuretics, such as spironolactone or triamterene, may be used in association with CAI or alone. In case of hyperkalemic attacks, the use of potassium-wasting diuretics, such as hydrochlorothiazide, should be considered very carefully due to the risk of a cardiac adverse effect of drug-induced hypokalemia.

4.2. Hypokalemic Periodic Paralysis

The KCNE3 gene encodes MirP2, an auxiliary subunit of K channels. The missense p.R83H mutation in KCNE3 was found in two pedigrees affected by periodic paralysis [188]. The same mutation was found in one of 14 patients affected by thyrotoxic periodic paralysis (TPP) [189]. However, the direct link between p.R83H and periodic paralysis was challenged by genetic studies performed on larger groups, showing a frequency similar in controls and patients as well as lacking segregation of the mutation with PP [190,191,192,193]. Thus, more studies are needed to verify whether KCN3E mutations cause hypoPP, constitute susceptibility polymorphisms, or are simply not related to hypoPP. Intriguingly, we found a reduced KCNE3 mRNA level in muscle biopsies of two patients affected by recessive myotonia congenita (Becker’s disease), but an increase in one patient with dominant myotonia congenita (Thomsen’s disease), compared to control individuals [194,195].

4.3. Thyrotoxic Periodic Paralysis

TPP linked to hyperthyroidism is the most common cause of hypokalemic flaccid muscle weakness in adult Asian and Hispanic males [196]. Of note, TPP is often indistinguishable from hypoPP; thus, an assessment of thyroid function should be always performed in patients with hypoPP. Besides, sporadic periodic paralysis (SPP) is characterized by normal thyroid function and lack of CACNA1S, SCN4A, or KCNJ2 mutation. Nevertheless, TTP and SPP are closely related since they appear to share a number of susceptibility genes [197,198,199,200]. Mutations in the KCNJ18 gene have been reported in a few cases with TPP [201,202,203,204]. The KCNJ18 gene encodes the skeletal muscle inward-rectifier K channel Kir2.6, the expression of which is enhanced by thyroid hormone (T3) through a promoter response element. Several KCNJ18 variants were shown to reduce Kir2.6 currents by affecting single-channel conductance, open probability, or cell surface expression. Some of these effects were T3-dependent, including altered modulation by PIP2 and PKC, which are activated during thyrotoxicosis. In addition, some Kir2.6 mutants exert a dominant negative effect not only on wild-type Kir2.6 but also on Kir2.1 channels, where the mutation is responsible for ATS1 [202]. It was proposed that wild-type Kir2.6 channels are activated by T3 in healthy muscle to maintain the resting membrane potential, thereby balancing the T3-induced weakness. Consequently, the loss-of-function mutations in KCNJ18 may increase the susceptibility of muscle to thyrotoxicosis-induced weakness. Interestingly, other susceptibility genes were identified in both TTP and SPP on chromosome 17q close to the KCNJ2 gene, suggesting a possible influence on Kir2.1 channel expression [197,205,206,207]. In addition, a variant of the ABCC8 gene encoding SUR1, the sulfonylurea receptor type 1 associated with ATP-sensitive inward-rectifier K channels (KATP), was proposed as another susceptibility gene for TPP [208]. Thus, it appears that the pathomechanism of TPP and SPP may be similar to that found in ATS. Nonetheless, many questions are still open, and more studies are needed to confirm the genotype–phenotype relationship [204,209,210].

4.4. Intellectual Disability Myopathy Syndrome

Recently, a new disease named intellectual disability myopathy syndrome (IDMS) was described in two pedigrees from Norway [211]. The disease is multisystemic, inducing intellectual disability, partial hearing loss, developmental delay, anxiety, sleep disorder, hyperreflexia, cerebral MRI anomalies, skeletal dysmorphism, cardiac systolic dysfunction, and myopathy. The muscle symptoms include generalized hypotonia in childhood and weakness and fatigability in adults. A muscle biopsy performed in one patient showed variations in fiber diameter and the presence of mitochondria aggregates. A splice-site mutation was identified in the ABCC9 gene that codes for SUR2, the sulfonylurea receptor type 2. From genetic databases, it appeared that, in the heterozygous state, the variant frequency was higher in the Finnish population compared to other Europeans and was absent outside Europe. All the patients were homozygous for the variant, in accord with the recessive inheritance. The SUR2 variant induced a complete loss of functional KATP channels in cells co-expressing Kir6.2. In agreement with the inheritance trait, the mutant does not exert any dominant negative effect on WT SUR2. In mice, the insertion of a premature stop codon in ABCC9, which induced a loss of function of SUR2, jeopardized the physical performance due to increased fatigability in patients. Differences in muscle symptoms associated with SUR1 (TPP) and SUR2 variants are quite surprising since both subunits bind to Kir6.2 to form KATP channels. However, the relative abundance of SUR1 and SUR2 is probably muscle-type-specific, as shown in mice [212], and their contribution to mitochondrial KATP channels is not established yet [213]. Another important difference between ATS and IDMS regards the inheritance mode of SUR1 and SUR2 mutations. Thus, as for most of the muscle ion channelopathies, recessive mutations are more threatening than dominant ones.

4.5. Episodic Ataxia/Myokymia

The episodic ataxias are a heterogeneous group of autosomal dominant diseases characterized by recurring attacks of cerebellar ataxia. Episodic ataxia type 1 (EA1) is caused by mutations in the KCNA1 gene encoding the voltage-dependent potassium Kv1.1 channel [214,215]. EA1 shows a broad phenotypic spectrum, including cerebellar ataxia, muscle spasticity, dyskinesia, seizures, epileptic encephalopathy, hyperthermia, and hypomagnesemia [216,217]. Muscle symptoms include constant myokymia and acute episodes of uncontrolled muscle contractions of the face and limbs, stiffness, cramps, and weakness, as well as malignant hyperthermia susceptibility in one kindred. In a few patients, muscle symptoms are largely preponderant. Functional studies of KCNA1 mutations in heterologous systems of expression indicate a loss of function of the Kv1.1 channel through altered gating, expression, or modulation. Studies of a knock-in mouse EA1 model provided mechanistic insights for the disease [218]. Loss of function in Kv1.1 increases the excitability of basket cells to release GABA that, in turn, inhibits Purkinje cells in the cerebellum, thereby inducing ataxia [218,219]. Mutations linked to ataxia are spanned over the entire protein. However, the loss of function of juxtaparanodal Kv1.1 channels increases the motor nerve excitability, which promotes myokymia [220]. Interestingly, mutations causing preeminent muscle symptoms with little or no ataxia are clustered in the transmembrane S2 and S3 helices and the S2–S3 intracellular linker [195,221,222,223]. Since KV1.1 channels are expressed in many central neurons, loss-of-function mutations may induce excessive brain excitability leading to epilepsy. Mutations affecting the channel pore region appear especially inclined to induce seizures. Those mutations in the conserved Pro-Val-Pro motif in the sixth transmembrane segment are linked to epileptic encephalopathy, i.e., recurrent seizures and intellectual disability [224,225]. The selective deletion of KCNA1 in neurons causes epilepsy, premature death, and cardiorespiratory dysregulation in mice [226]. The variability of symptoms associated with KCNA1 mutations suggests that mutations may manifest their effects in a cell type-dependent manner. Such effects might depend on the specific biophysical defect or on specific interactions with other proteins, such as other Kv subunits. In addition, environmental factors and gene modifiers may account for the different symptoms observed in patients carrying the same mutation [195,217]. Such a great variability in symptoms makes KCNA1-related diseases difficult to diagnose. For instance, next-generation sequencing recently revealed an already known KCNA1 mutation (p.N255D) in a patient diagnosed with myotonia, presenting with hand and facial stiffness without ataxia [227].
Pharmacological therapy of KCNA1-related diseases is symptomatic only [216,228,229]. The carbonic anhydrase inhibitor ACZ provided some relief in a number of patients. However, limiting side effects can develop in the long term (kidney stones, excessive sweating, paresthesia, muscle stiffness and fatigability, gastrointestinal disorders, concentration and memory difficulties). In addition, non-responders have been frequently observed. The mechanism of action of ACZ in EA1 and other ion channelopathies is still unclear. Whether Kv1.1 channels are sensitive to the change in pH value is unknown. Antiepileptic drugs, including sodium channel blockers (carbamazepine, oxcarbazepine, lamotrigine, phenytoin, valproic acid), phenobarbital, benzodiazepine (clonazepam, clozapam), vigabatrin, and gabapentin, have been used with some benefit to relieve ataxia and seizures. In some patients, these drugs may be ineffective or may worsen symptoms. However, there is no drug-class effect, as a patient refractory to one or more antiepileptic drugs may have benefited from another. No information is available regarding the effects of these drugs on wild-type or mutated Kv1.1 channels. In addition, information is lacking regarding the effects of treatment on muscle symptoms.

5. Chloride Channel-Related Muscle Disorders

The chloride channel family includes a variety of proteins involved in many different cellular functions, which include maintenance of ion homeostasis, trans-epithelial fluid transport, modulation of intracellular compartment pH value, cell volume regulation, and the regulation of cell excitability [230]. In skeletal muscle fibers, the high level of sarcolemma chloride conductance (gCl) is crucial for the stabilization of the resting membrane potential and the repolarization of action potentials [231].
The gCl in skeletal muscle is mediated by the voltage-gated ClC-1 chloride channels. It was the first mammalian voltage-gated chloride-channel identified belonging to the family of CLC proteins [232].
With a mass of ~120 kDa, ClC-1 is the largest protein of this family, composed of two identical subunits, each forming a gated pore. Each subunit consists of 18 α-helices, 17 of which are embedded in the plasma membrane, and 2 tandem cystathionine-β-synthase (CBS) domains located in the intracellular C-terminal region [233,234].
Loss-of-function mutations in the CLCN1 gene abolish or reduce ClC-1 plasma membrane currents, leading to myotonia congenita (MC), the most frequent hereditary skeletal muscle channelopathy in humans [2,235,236]. MC can be inherited either as an autosomal dominant (Thomsen’s disease) or an autosomal recessive (Becker’s disease) trait; Becker’s disease is associated with a more severe phenotype. MC patients present with muscle stiffness and delayed muscle relaxation after a voluntary movement, a clinical sign called myotonia. Myotonia in MC is worse at rest and instead improves with exercise, the so-called warm-up phenomenon [42]. Other symptoms include muscle hypertrophy, more frequent in Becker’s disease and conferring a “hercules” habitus to the patient, and cold sensitivity of myotonia, although less frequent than in patients carrying SCN4A mutations. Myotonia in MC is more frequently observed in the limbs, while cranial myotonia is much more suggestive of SCM or PMC [4,11,237]. Painful myotonia is more frequent in SCM than in MC [11,237]. Furthermore, patients with Becker’s disease may experience transient weakness at the onset of voluntary contraction that may rarely lead to falls [238].
More than 250 CLCN1 mutations have been found to be associated with MC. They scattered over the entire sequence of the channel protein, but a few regions with high-frequency mutations have been described in exons 4, 5, and 8 [2,239,240,241]. With the exception of a few nonsense mutations leading to truncated ClC-1 proteins, all dominant mutations are missense mutations. Recessive mutations include deletions, insertions, splice-site, missense, or nonsense errors. In addition, a combination of whole exon deletions or duplications and point mutations in CLCN1 accounted for 6% of patients with MC [242].
In vitro functional studies of ClC-1 mutations have clarified the molecular mechanisms by which the dominant and recessive mutations alter ion channel function and expression (Figure 4). In Thomsen’s disease, the mutant subunit is expected to exert a dominant-negative effect on the associated wild-type (WT) subunit in the dimeric channel [243]. Thus, in the heterozygous carrier, the gCl is reduced by more than 50%, leading to overexcitability. This is the case of the p.T335N mutation, identified for the first time in an Italian family. This mutation induced a reduction of chloride current and exerted a dominant negative effect on the WT subunit, consistent with mild Thomsen’s phenotype [244]. In contrast, ClC-1 mutated subunits associated with recessive myotonia do not exert a significant dominant-negative effect on the associated subunit. In the heterozygous carrier, WT subunits sustain at least 50% of the gCl, and muscle function is preserved. In the compound heterozygous carrier, all the subunits are mutated, and the gCl is reduced 50% more, leading to myotonia [243].
The majority of MC mutations are predicted to reduce chloride currents by impaired ClC-1 proteostasis (impaired synthesis, defective cell trafficking, increased degradation) or by impairing ClC-1 function through various gating defects. The latter one includes a positive shift of the voltage-dependent activation of fast and slow channel gating, reduction of single-channel conductance, altered ion selectivity, or an inverted voltage dependence (hyperpolarization-activated) [241,244,245,246,247,248,249]. A number of ClC-1 mutations found in myotonic patients show no evidence of any functional defect when studied in heterologous expression systems. Notable examples include several missense mutations, such as p.T82A, p.F167L, p.R453W, p.L628P, and p.L861P [28,194,246,247]. This suggests that the defect of these variants may arise only in the skeletal muscle cells due to altered interactions with muscle proteins.
Currently, MC patients receive symptomatic treatment, which aims at dampening skeletal muscle hyperexcitability through inhibition of voltage-gated sodium channels. Thus, mexiletine was employed as the first-line therapy in MC, similarly to sodium channel myotonia and paramyotonia congenita [22]. Very recently, persistent sodium currents have been proposed to be involved in the mechanism underlying the transient weakness in recessive MC [250]. This may explain why mexiletine is greatly efficient against this debilitating symptom [238]. Similar to PMC and SCM, lamotrigine can be considered as a second choice in MC [26,27].
Besides sodium channel blockers, ACZ was reported to be efficient in small cohorts of MC patients [251,252] and could be considered a second choice. The mechanism of ACZ is not well defined, but it might stimulate the ClC-1 channel activity through intracellular acidification [39,253]. However, there is no known direct activator of ClC-1 available. The classification of ClC-1 mutations according to their functional defect would be fundamental to help the discovery of new drugs that target mutant channels’ defects with the hope of ensuring a personalized treatment for MC patients. This includes the drug able to correct mutant channel gating (gating-modifiers) or to improve the expression of traffic-defective mutants (pharmacological chaperones) [231].

6. Nicotinic Receptor-Channels

Nicotinic acetylcholine receptor (AChR) is localized on the crests of the folded postsynaptic muscle membrane. The binding of acetylcholine with its receptor opens the central ion channel pore of the AChR, resulting in depolarization of the muscle membrane. The AChR is a pentamer comprising four different subunits (α, β, δ, ε in a ratio of 2:1:1:1), with each subunit encoded by a separate gene and forming a transmembrane ligand-gated ion channel. Congenital myasthenic syndrome (CMS) is a rare genetic disorder due to mutations in genes encoding proteins involved in the neuromuscular junction (NMJ) structure and function, causing skeletal muscle weakness and fatigability [254]. CMS may be classified based on the localization in the NMJ or the function of the mutated protein, with AChR defects accounting for around half of the CMS cases [255]. CMS related to AChR defects includes AChR deficiency and, much less frequently, AChR kinetic defects, which can be classified into slow and fast-channel syndromes. All the AChR subunits may be involved in CMS, especially the epsilon subunit gene (CHRNE) is mutated in about 20%–50% of the cases [255,256,257]. CMS related to AChR defects are recessively inherited, except for slow-channel syndrome (SCS), which is an autosomal dominant disease [254].
The clinical presentation of CMS due to AChR defects is highly variable, ranging from mild symptoms to severe manifestations, sometimes with life-threatening respiratory episodes, especially in the first decade of life. These CMS subtypes usually present at birth or in infancy, often with hypotonia in association with ocular, facial, bulbar or respiratory symptoms and followed by delayed motor milestones. Alternatively, they may present later with walking difficulty and frequent falls. Prenatal onset with arthrogryposis multiplex congenital (AMC) and fetal akinesia (FA) was originally reported on patients mutated in CHRNG, coding for the gamma subunit of the fetal form of AChR [258]. No myasthenic symptoms were observed at birth or later because the adult AChR was normally expressed. AMC and FA have been reported in association with mutations in other CMS genes, including CHRNA1 and CHRND, characterized by CMS symptoms and absence of adult AChR in the disease animal model [259,260]. CMS is usually characterized by static or slowly progressive course over the years, although acute exacerbations may be triggered by infectious episodes, surgery, or stress, sometimes leading to acute respiratory failure, in particular in the first years of life [254]. The central nervous system and heart are not involved. The CMS diagnosis is based on clinical and electromyography findings, followed by the identification of the molecular defect, which may be guided by specific clinical, neurophysiological or histological clues [254].
Only symptomatic pharmacological therapies are available for CMS treatment. Of note, drugs with positive effects on specific forms of CMS may worsen another one, as pyridostigmine in SCS. Hence, genetic diagnosis is highly recommended to optimize pharmacologic treatment. Drugs useful to treat CMS due to AChR defects are mainly cholinergic agonists (PYR and 3,4 DAP). Adrenergic agonists (salbutamol/albuterol and ephedrine) may be used in patients not responsive to cholinergic agonists. Fluoxetine and quinidine are long-lived open-channel blockers of the AChR ion channel, and they are currently used only in SCS [254]. Salbutamol may be used even in SCS [261].

7. Concluding Remarks

The SMICs represent an expanding field; in this regard, new genes and new phenotypes have been recently discovered after the introduction of next-generation sequencing [227,262,263,264,265]. Clinical variability warrants better comprehension of genotype–phenotype correlations and of other mechanisms influencing clinical expression [266]. For instance, the coexistence of mutations in two different genes and non-genetic factors (epigenetic, environmental, and hormonal) may help the understanding of the clinical variability [24,267,268,269].
Up to date, most treatments are only symptomatic. However, knowledge of the pathomechanisms and detailed phenotyping may offer the possibility to develop more targeted therapies with increased efficacy and safety. Early molecular diagnosis is critical because the choice of therapeutic option may help save lives or slow down the disease progression. Ion channels are expressed on the membrane and may be easily druggable with small molecular weight molecules or monoclonal antibodies. Small compounds able to correct the specific defect induced by mutations are warranted, as it occurred for the pharmacological treatment of CFTR mutations in cystic fibrosis [270]. To this purpose, an interdisciplinary approach including both clinical, molecular, neurophysiological and pharmacological data is the only promising strategy to find efficient new treatments for SMICs.

Author Contributions

Conceptualization L.M. and J.-F.D.; manuscript draft preparation S.B. and C.A.; revision and editing L.M. and J.-F.D. All authors have read and agreed to the published version of the manuscript.

Funding

J.-F.D. is supported by Association Française contre les Myopathies (grant #16123) and Bari University (grant #2017–2018).

Institutional Review Board Statement

Not applicable.

Informed Consent Statement

Not applicable.

Data Availability Statement

Not applicable.

Acknowledgments

Lorenzo Maggi is a member of the ERN Muscle Working group.

Conflicts of Interest

The authors report no disclosure relevant to the manuscript.

References

  1. Fontaine, B.; Khurana, T.S.; Hoffman, E.P.; Bruns, G.A.; Haines, J.L.; Trofatter, J.A.; Hanson, M.P.; Rich, J.; McFarlane, H.; Yasek, D.M. Hyperkalemic periodic paralysis and the adult muscle sodium channel alpha-subunit gene. Science 1990, 250, 1000–1002. [Google Scholar] [CrossRef] [PubMed]
  2. Horga, A.; Rayan, D.L.; Matthews, E.; Sud, R.; Fialho, D.; Durran, S.C.; Burge, J.A.; Portaro, S.; Davis, M.B.; Haworth, A.; et al. Prevalence study of genetically defined skeletal muscle channelopathies in England. Neurology 2013, 80, 1472–1475. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  3. Stunnenberg, B.C.; Raaphorst, J.; Deenen, J.C.; Links, T.P.; Wilde, A.A.; Verbove, D.J.; Kamsteeg, E.J.; van den Wijngaard, A.; Faber, C.G.; van der Wilt, G.J.; et al. Prevalence and mutation spectrum of skeletal muscle channelopathies in the Netherlands. Neuromuscul. Disord. 2018, 28, 402–407. [Google Scholar] [CrossRef] [PubMed]
  4. Maggi, L.; Brugnoni, R.; Canioni, E.; Tonin, P.; Saletti, V.; Patrizia, S.; Cotti Piccinelli, S.; Colleoni, L.; Ferrigno, P.; Antonella, P.; et al. Clinical and Molecular Spectrum of Myotonia and Periodic Paralyses Associated With Mutations in SCN4A in a Large Cohort of Italian Patients. Front. Neurol. 2020, 11, 646. [Google Scholar] [CrossRef] [PubMed]
  5. Ptáček, L.J.; George, A.L., Jr.; Griggs, R.C.; Tawil, R.; Kallen, R.G.; Barchi, R.L.; Robertson, M.; Leppert, M.F. Identification of a mutation in the gene causing hyperkalemic periodic paralysis. Cell 1991, 67, 1021–1027. [Google Scholar] [CrossRef]
  6. Rojas, C.V.; Wang, J.Z.; Schwartz, L.S.; Hoffman, E.P.; Powell, B.R.; Brown, R.H., Jr. A Met-to-Val mutation in the skeletal muscle Nav channel alpha-subunit in hyperkalaemic periodic paralysis. Nature 1991, 354, 387–389. [Google Scholar] [CrossRef] [PubMed]
  7. Miller, T.M.; Da Silva, M.D.; Miller, H.A.; Kwiecinski, H.; Mendell, J.R.; Tawil, R.; McManis, P.; Griggs, R.C.; Angelini, C.; Servidei, S.; et al. Correlating phenotype and genotype in the periodic paralyses. Neurology 2004, 63, 1647–1655. [Google Scholar] [CrossRef] [PubMed]
  8. Ptáček, L.J.; George, A.L., Jr.; Barchi, R.L.; Griggs, R.C.; Riggs, J.E.; Robertson, M.; Leppert, M.F. Mutations in an S4 segment of the adult skeletal muscle sodium channel cause paramyotonia congenita. Neuron 1992, 8, 891–897. [Google Scholar] [CrossRef]
  9. Matthews, E.; Fialho, D.; Tan, S.V.; Venance, S.L.; Cannon, S.C.; Sternberg, D.; Fontaine, B.; Amato, A.A.; Barohn, R.J.; Griggs, R.C.; et al. The non-dystrophic myotonias: Molecular pathogenesis, diagnosis and treatment. Brain 2010, 133, 9–22. [Google Scholar] [CrossRef]
  10. Lerche, H.; Heine, R.; Pika, U.; George Jr, A.L.; Mitrovic, N.; Browatzki, M.; Weiss, T.; Rivet-Bastide, M.; Franke, C.; Lomonaco, M. Human sodium channel myotonia: Slowed channel inactivation due to substitutions for a glycine within the III-IV linker. J. Physiol. 1993, 470, 13–22. [Google Scholar] [CrossRef] [PubMed]
  11. Trip, J.; Drost, G.; Ginjaar, H.B.; Nieman, F.H.; van der Kooi, A.J.; de Visser, M.; van Engelen, B.G.; Faber, C.G. Redefining the clinical phenotypes of non-dystrophic myotonic syndromes. J. Neurol. Neurosurg. Psychiatry 2009, 80, 647–652. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  12. Cea, G.; Andreu, D.; Fletcher, E.; Ramdas, S.; Sud, R.; Hanna, M.G.; Matthews, E. Sodium channel myotonia may be associated with high-risk brief resolved unexplained events. Wellcome Open Res. 2020, 5, 57. [Google Scholar] [CrossRef] [PubMed]
  13. Fusco, C.; Frattini, D.; Salerno, G.G.; Canali, E.; Bernasconi, P.; Maggi, L. New phenotype and neonatal onset of sodium channel myotonia in a child with a novel mutation of SCN4A gene. Brain Dev. 2015, 37, 891–893. [Google Scholar] [CrossRef] [PubMed]
  14. Bednarz, M.; Stunnenberg, B.C.; Kusters, B.; Kamsteeg, E.J.; Saris, C.G.; Groome, J.; Winston, V.; Meola, G.; Jurkat-Rott, K.; Voermans, N.C. A novel Ile1455Thr variant in the skeletal muscle sodium channel alpha-subunit in a patient with a severe adult-onset proximal myopathy with electrical myotonia and a patient with mild paramyotonia phenotype. Neuromuscul. Disord. 2017, 27, 175–182. [Google Scholar] [CrossRef]
  15. Luo, S.; Castañeda, M.S.; Matthews, E.; Sud, R.; Hanna, M.G.; Sun, J.; Song, J.; Lu, J.; Qiao, K.; Zhao, C.; et al. Hypokalaemic periodic paralysis and myotonia in a patient with homozygous mutation p.R1451L in Nav1.4. Sci. Rep. 2018, 8, 9714. [Google Scholar] [CrossRef] [PubMed]
  16. Elia, N.; Nault, T.; McMillan, H.J.; Graham, G.E.; Huang, L.; Cannon, S.C. Myotonic myopathy with secondary joint and skeletal anomalies from the c.2386C>G, p.L769V mutation in SCN4A. Front. Neurol. 2020, 11, 77. [Google Scholar] [CrossRef] [PubMed]
  17. Poulin, H.; Gosselin-Badaroudine, P.; Vicart, S.; Habbout, K.; Sternberg, D.; Giuliano, S.; Fontaine, B.; Bendahhou, S.; Nicole, S.; Chahine, M. Substitutions of the S4DIV R2 residue (R1451) in NaV1.4 lead to complex forms of paramyotonia congenita and periodic paralyses. Sci. Rep. 2018, 8, 2041. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  18. Taminato, T.; Mori-Yoshimura, M.; Miki, J.; Sasaki, R.; Sato, N.; Oya, Y.; Nishino, I.; Takahashi, Y. Paramyotonia Congenita with Persistent Distal and Facial Muscle Weakness: A Case Report with Literature Review. J. Neuromuscul. Dis. 2020, 7, 193–201. [Google Scholar] [CrossRef]
  19. Cannon, S.C. Sodium channelopathies of skeletal muscle. Handb. Exp. Pharmacol. 2018, 246, 309–330. [Google Scholar]
  20. Cannon, S.C.; Brown, R.H., Jr.; Corey, D.P. Theoretical reconstruction of myotonia and paralysis caused by incomplete inactivation of sodium channels. Biophys. J. 1993, 65, 270–288. [Google Scholar] [CrossRef] [Green Version]
  21. Hayward, L.J.; Sandoval, G.M.; Cannon, S.C. Defective slow inactivation of sodium channels contributes to familial periodic paralysis. Neurology 1999, 52, 1447–1453. [Google Scholar] [CrossRef] [PubMed]
  22. Statland, J.M.; Bundy, B.N.; Wang, Y.; Rayan, D.R.; Trivedi, J.R.; Sansone, V.A.; Salajegheh, M.K.; Venance, S.L.; Ciafaloni, E.; Matthews, E.; et al. Mexiletine for symptoms and signs of myotonia in nondystrophic myotonia: A randomized controlled trial. JAMA 2012, 308, 1357–1365. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  23. Stunnenberg, B.C.; Raaphorst, J.; Groenewoud, H.M.; Statland, J.M.; Griggs, R.C.; Woertman, W.; Stegeman, D.F.; Timmermans, J.; Trivedi, J.; Matthews, E.; et al. Effect of mexiletine on muscle stiffness in patients with nondystrophic myotonia evaluated using aggregated N-of-1 trials. JAMA 2018, 320, 2344–2353. [Google Scholar] [CrossRef] [PubMed]
  24. Suetterlin, K.J.; Bugiardini, E.; Kaski, J.P.; Morrow, J.M.; Matthews, E.; Hanna, M.G.; Fialho, D. Long-term safety and efficacy of mexiletine for patients with skeletal muscle channelopathies. JAMA Neurol. 2015, 72, 1531–1533. [Google Scholar] [CrossRef] [Green Version]
  25. Modoni, A.; D’Amico, A.; Primiano, G.; Capozzoli, F.; Desaphy, J.-F.; Lo Monaco, M. Long-term safety and usefulness of mexiletine in a large cohort of patients affected by non-dystrophic myotonias. Front. Neurol. 2020, 11, 300. [Google Scholar] [CrossRef] [PubMed]
  26. Andersen, G.; Hedermann, G.; Witting, N.; Duno, M.; Andersen, H.; Vissing, J. The antimyotonic effect of lamotrigine in non-dystrophic myotonias: A double-blind randomized study. Brain 2017, 140, 2295–2305. [Google Scholar] [CrossRef] [PubMed]
  27. Vereb, N.; Montagnese, F.; Gläser, D.; Schoser, B. Non-dystrophic myotonias: Clinical and mutation spectrum of 70 German patients. J. Neurol. 2021, 268, 1708–1720. [Google Scholar] [CrossRef]
  28. Desaphy, J.F.; Modoni, A.; Lomonaco, M.; Camerino, D.C. Dramatic improvement of myotonia permanens with flecainide: A two-case report of a possible bench-to-bedside pharmacogenetics strategy. Eur. J. Clin. Pharmacol. 2013, 69, 1037–1039. [Google Scholar] [CrossRef] [Green Version]
  29. Desaphy, J.F.; Carbonara, R.; D’Amico, A.; Modoni, A.; Roussel, J.; Imbrici, P.; Pagliarani, S.; Lucchiari, S.; Lo Monaco, M.; Conte Camerino, D. Translational approach to address therapy in myotonia permanens due to a new SCN4A mutation. Neurology 2016, 86, 2100–2108. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  30. Farinato, A.; Altamura, C.; Imbrici, P.; Maggi, L.; Bernasconi, P.; Mantegazza, R.; Pasquali, L.; Siciliano, G.; Monaco, M.L.; Vial, C.; et al. Pharmacogenetics of myotonic hNav1.4 sodium channel variants situated near the fast inactivation gate. Pharmacol. Res. 2019, 141, 224–235. [Google Scholar] [CrossRef] [PubMed]
  31. Desaphy, J.F.; Altamura, C.; Vicart, S.; Fontaine, B. Targeted Therapies for Skeletal Muscle Ion Channelopathies: Systematic Review and Steps Towards Precision Medicine. J. Neuromuscul. Dis. 2021, 8, 357–381. [Google Scholar] [CrossRef]
  32. Desaphy, J.F.; Carbonara, R.; Costanza, T.; Conte Camerino, D. Preclinical evaluation of marketed sodium channel blockers in a rat model of myotonia discloses promising antimyotonic drugs. Exp. Neurol. 2014, 255, 96–102. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  33. Desaphy, J.F.; Farinato, A.; Altamura, C.; De Bellis, M.; Imbrici, P.; Tarantino, N.; Caccia, C.; Melloni, E.; Padoani, G.; Vailati, S.; et al. Safinamide’s potential in treating nondystrophic myotonias: Inhibition of skeletal muscle voltage-gated sodium channels and skeletal muscle hyperexcitability in vitro and in vivo. Exp. Neurol. 2020, 328, 113287. [Google Scholar] [CrossRef] [PubMed]
  34. Novak, K.R.; Norman, J.; Mitchell, J.R.; Pinter, M.J.; Rich, M.M. Sodium channel slow inactivation as a therapeutic target for myotonia congenita. Ann. Neurol. 2015, 77, 320–332. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  35. Skov, M.; de Paoli, F.V.; Nielsen, O.B.; Pedersen, T.H. The anti-convulsants lacosamide, lamotrigine, and rufinamide reduce myotonia in isolated human and rat skeletal muscle. Muscle Nerve 2017, 56, 136–142. [Google Scholar] [CrossRef] [PubMed]
  36. De Bellis, M.; Carbonara, R.; Roussel, J.; Farinato, A.; Massari, A.; Pierno, S.; Muraglia, M.; Corbo, F.; Franchini, C.; Carratù, M.R.; et al. Increased sodium channel use-dependent inhibition by a new potent analogue of tocainide greatly enhances in vivo antimyotonic activity. Neuropharmacology 2017, 113, 206–216. [Google Scholar] [CrossRef] [Green Version]
  37. De Bellis, M.; De Luca, A.; Desaphy, J.F.; Carbonara, R.; Heiny, J.A.; Kennedy, A.; Carocci, A.; Cavalluzzi, M.M.; Lentini, G.; Franchini, C.; et al. Combined modifications of mexiletine pharmacophores for new lead blockers of Na(v)1.4 channels. Biophys. J. 2013, 104, 344–354. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  38. Tricarico, D.; Mele, A.; Conte Camerino, D. Carbonic anhydrase inhibitors ameliorate the symptoms of hypokalaemic periodic paralysis in rats by opening the muscular Ca2+- activated-K+channels. Neuromuscul. Disord. 2006, 16, 39–45. [Google Scholar] [CrossRef]
  39. Altamura, C.; Fonzino, A.; Tarantino, N.; Conte, E.; Liantonio, A.; Imbrici, P.; Carratù, M.R.; Pierno, S.; Desaphy, J.F. Increased sarcolemma chloride conductance as one of the mechanisms of action of carbonic anhydrase inhibitors in muscle excitability disorders. Exp. Neurol. 2021, 342, 113758. [Google Scholar] [CrossRef]
  40. Sansone, V.A.; Burge, J.; McDermott, M.P.; Smith, P.C.; Herr, B.; Tawil, R.; Pandya, S.; Kissel, J.; Ciafaloni, E.; Shieh, P.; et al. Randomized, placebo-controlled trials of dichlorphenamide in periodic paralysis. Neurology 2016, 86, 1408–1416. [Google Scholar] [CrossRef] [Green Version]
  41. Statland, J.M.; Fontaine, B.; Hanna, M.G.; Johnson, N.E.; Kissel, J.T.; Sansone, V.A.; Shieh, P.B.; Tawil, R.N.; Trivedi, J.; Cannon, S.C.; et al. Review of the Diagnosis and Treatment of Periodic Paralysis. Muscle Nerve 2018, 57, 522–530. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  42. Stunnenberg, B.C.; LoRusso, S.; Arnold, W.D.; Barohn, R.J.; Cannon, S.C.; Fontaine, B.; Griggs, R.C.; Hanna, M.G.; Matthews, E.; Meola, G.; et al. Guidelines on clinical presentation and management of nondystrophic myotonias. Muscle Nerve 2020, 62, 430–444. [Google Scholar] [CrossRef]
  43. Bulman, D.E.; Scoggan, K.A.; van Oene, M.D.; Nicolle, M.W.; Hahn, A.F.; Tollar, L.L.; Ebers, G.C. A novel sodium channel mutation in a family with hypokalemic periodic paralysis. Neurology 1999, 53, 1932–1936. [Google Scholar] [CrossRef]
  44. Jurkat-Rott, K.; Mitrovic, N.; Hang, C.; Kouzmenkine, A.; Iaizzo, P.; Herzog, J.; Lerche, H.; Nicole, S.; Vale-Santos, J.; Chauveau, D.; et al. Voltage-sensor sodium channel mutations cause hypokalemic periodic paralysis type 2 by enhanced inactivation and reduced current. Proc. Natl. Acad. Sci. USA 2000, 97, 9549–9554. [Google Scholar] [CrossRef] [Green Version]
  45. Matthews, E.; Labrum, R.; Sweeney, M.G.; Sud, R.; Haworth, A.; Chinnery, P.F.; Meola, G.; Schorge, S.; Kullmann, D.M.; Davis, M.B.; et al. Voltage sensor charge loss accounts for most cases of hypokalemic periodic paralysis. Neurology 2009, 72, 1544–1547. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  46. Matthews, E.; Portaro, S.; Ke, Q.; Sud, R.; Haworth, A.; Davis, M.B.; Griggs, R.C.; Hanna, M.G. ACZ efficacy in hypokalemic periodic paralysis and the predictive role of genotype. Neurology 2011, 77, 1960–1964. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  47. Tsujino, A.; Maertens, C.; Ohno, K.; Shen, X.M.; Fukuda, T.; Harper, C.M.; Cannon, S.C.; Engel, A.G. Myasthenic syndrome caused by mutation of the SCN4A sodium channel. Proc. Natl. Acad. Sci. USA 2003, 100, 7377–7382. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  48. Zaharieva, I.T.; Thor, M.G.; Oates, E.C.; Van Karnebeek, C.; Hendson, G.; Blom, E.; Witting, N.; Rasmussen, M.; Gabbett, M.T.; Ravenscroft, G.; et al. Loss-of-function mutations in SCN4A cause severe foetal hypokinesia or classical congenital myopathy. Brain 2016, 139, 674–691. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  49. Thompson, R.; Bonne, G.; Missier, P.; Lochmüller, H. Targeted therapies for congenital myasthenic syndromes: Systematic review and steps towards a treatabolome. Emerg. Top. Life Sci. 2019, 3, 19–37. [Google Scholar] [PubMed]
  50. Matthews, E.; Hartley, L.; Sud, R.; Hanna, M.G.; Muntoni, F.; Munot, P. Acetazolamide can improve symptoms and signs in ion channel-related congenital myopathy. J. Neurol. Neurosurg. Psychiatry 2019, 90, 243–245. [Google Scholar] [CrossRef] [PubMed]
  51. Ptáček, L.J.; Tawil, R.; Griggs, R.C.; Engel, A.G.; Layzer, R.B.; Kwieciński, H.; McManis, P.G.; Santiago, L.; Moore, M.; Fouad, G.; et al. Dihydropyridine receptor mutations cause hypokalemic periodic paralysis. Cell 1994, 77, 863–868. [Google Scholar] [CrossRef]
  52. Holm-Yildiz, S.; Witting, N.; Dahlqvist, J.; de Stricker Borch, J.; Solheim, T.; Fornander, F.; Eisum, A.S.; Duno, M.; Soerensen, T.; Vissing, J. Permanent muscle weakness in hypokalemic periodic paralysis. Neurology 2020, 95, e342–e352. [Google Scholar] [CrossRef] [PubMed]
  53. Fan, C.; Lehmann-Horn, F.; Weber, M.A.; Bednarz, M.; Groome, J.R.; Jonsson, M.K. Transient compartment-like syndrome and normokalaemic periodic paralysis due to a Ca(v)1.1 mutation. Brain 2013, 136, 3775–3786. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  54. Wu, F.; Mi, W.; Hernández-Ochoa, E.O.; Burns, D.K.; Fu, Y.; Gray, H.F.; Struyk, A.F.; Schneider, M.F.; Cannon, S.C. A calcium channel mutant mouse model of hypokalemic periodic paralysis. J. Clin. Investig. 2012, 122, 4580–4591. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  55. Schartner, V.; Romero, N.B.; Donkervoort, S.; Treves, S.; Munot, P.; Pierson, T.M.; Dabaj, I.; Malfatti, E.; Zaharieva, I.T.; Zorzato, F.; et al. Dihydropyridine receptor (DHPR, CACNA1S) congenital myopathy. Acta Neuropathol. 2017, 133, 517–533. [Google Scholar] [CrossRef] [PubMed]
  56. Jungbluth, H.; Treves, S.; Zorzato, F.; Sarkozy, A.; Ochala, J.; Sewry, C.; Phadke, R.; Gautel, M.; Muntoni, F. Congenital myopathies: Disorders of excitation-contraction coupling and muscle contraction. Nat. Rev. Neurol. 2018, 14, 151–167. [Google Scholar] [CrossRef] [PubMed]
  57. Hunter, J.M.; Ahearn, M.E.; Balak, C.D.; Liang, W.S.; Kurdoglu, A.; Corneveaux, J.J.; Russell, M.; Huentelman, M.J.; Craig, D.W.; Carpten, J.; et al. Novel pathogenic variants and genes for myopathies identified by whole exome sequencing. Mol. Genet. Genomic Med. 2015, 3, 283–301. [Google Scholar] [CrossRef]
  58. Ravenscroft, G.; Clayton, J.S.; Faiz, F.; Sivadorai, P.; Milnes, D.; Cincotta, R.; Moon, P.; Kamien, B.; Edwards, M.; Delatycki, M.; et al. Neurogenetic fetal akinesia and arthrogryposis: Genetics, expanding genotype-phenotypes and functional genomics. J. Med. Genet. 2020. [Google Scholar] [CrossRef]
  59. Yiş, U.; Hiz, S.; Güneş, S.; Diniz, G.; Baydan, F.; Töpf, A.; Sonmezler, E.; Lochmüller, H.; Horvath, R.; Oktay, Y. Dihydropyridine Receptor Congenital Myopathy In A Consangineous Turkish Family. J. Neuromuscul. Dis. 2019, 6, 377–384. [Google Scholar] [CrossRef]
  60. Flucher, B.E.; Campiglio, M. STAC proteins: The missing link in skeletal muscle EC coupling and new regulators of calcium channel function. Biochim. Biophys. Acta Mol. Cell. Res. 2019, 1866, 1101–1110. [Google Scholar] [CrossRef]
  61. Nelson, B.R.; Wu, F.; Liu, Y.; Anderson, D.M.; McAnally, J.; Lin, W.; Cannon, S.C.; Bassel-Duby, R.; Olson, E.N. Skeletal muscle-specific T-tubule protein STAC3 mediates voltage-induced Ca2+ release and contractility. Proc. Natl. Acad. Sci. USA 2013, 110, 11881–11886. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  62. Horstick, E.J.; Linsley, J.W.; Dowling, J.J.; Hauser, M.A.; McDonald, K.K.; Ashley-Koch, A.; Saint-Amant, L.; Satish, A.; Cui, W.W.; Zhou, W.; et al. Stac3 is a component of the excitation-contraction coupling machinery and mutated in Native American myopathy. Nat. Commun. 2013, 4, 1952. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  63. Bailey, A.G.; Bloch, E.C. Malignant hyperthermia in a three-month-old American Indian infant. Anesth. Analg. 1987, 66, 1043–1045. [Google Scholar] [CrossRef] [PubMed]
  64. Stewart, C.R.; Kahler, S.G.; Gilchrist, J.M. Congenital myopathy with cleft palate and increased susceptibility to malignant hyperthermia: King syndrome? Pediatr. Neurol. 1988, 4, 371–374. [Google Scholar] [CrossRef]
  65. Stamm, D.S.; Aylsworth, A.S.; Stajich, J.M.; Kahler, S.G.; Thorne, L.B.; Speer, M.C.; Powell, C.M. Native American myopathy: Congenital myopathy with cleft palate, skeletal anomalies, and susceptibility to malignant hyperthermia. Am. J. Med. Genet. A 2008, 146, 1832–1841. [Google Scholar] [CrossRef] [PubMed]
  66. Flucher, B.E. Skeletal muscle Cav1.1 channelopathies. Pflug. Arch. 2020, 472, 739–754. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  67. Telegrafi, A.; Webb, B.D.; Robbins, S.M.; Speck-Martins, C.E.; FitzPatrick, D.; Fleming, L.; Redett, R.; Dufke, A.; Houge, G.; van Harssel, J.J.; et al. Identification of STAC3 variants in non-Native American families with overlapping features of Carey-Fineman-Ziter syndrome and Moebius syndrome. Am. J. Med. Genet. A 2017, 173, 2763–2771. [Google Scholar] [CrossRef]
  68. Zaharieva, I.T.; Sarkozy, A.; Munot, P.; Manzur, A.; O’Grady, G.; Rendu, J.; Malfatti, E.; Amthor, H.; Servais, L.; Urtizberea, J.A.; et al. STAC3 variants cause a congenital myopathy with distinctive dysmorphic features and malignant hyperthermia susceptibility. Hum. Mutat. 2018, 39, 1980–1994. [Google Scholar] [CrossRef] [Green Version]
  69. Grzybowski, M.; Schänzer, A.; Pepler, A.; Heller, C.; Neubauer, B.A.; Hahn, A. Novel STAC3 Mutations in the First Non-Amerindian Patient with Native American Myopathy. Neuropediatrics 2017, 48, 451–455. [Google Scholar]
  70. Wong King Yuen, S.M.; Campiglio, M.; Tung, C.C.; Flucher, B.E.; Van Petegem, F. Structural insights into binding of STAC proteins to voltage-gated calcium channels. Proc. Natl. Acad. Sci. USA 2017, 114, E9520–E9528. [Google Scholar] [CrossRef] [Green Version]
  71. Campiglio, M.; Kaplan, M.M.; Flucher, B.E. STAC3 incorporation into skeletal muscle triads occurs independent of the dihydropyridine receptor. J. Cell. Physiol. 2018, 233, 9045–9051. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  72. Hoth, M.; Penner, R. Depletion of intracellular calcium stores activates a calcium current in mast cells. Nature 1992, 355, 353–356. [Google Scholar] [CrossRef] [PubMed]
  73. Prakriya, M. The molecular physiology of CRAC channels. Immunol. Rev. 2009, 231, 88–98. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  74. Lacruz, R.S.; Feske, S. Diseases caused by mutations in ORAI1 and STIM1. Ann. N. Y. Acad. Sci. 2015, 1356, 45–79. [Google Scholar] [CrossRef] [Green Version]
  75. Roos, J.; DiGregorio, P.J.; Yeromin, A.V.; Ohlsen, K.; Lioudyno, M.; Zhang, S.; Safrina, O.; Kozak, J.A.; Wagner, S.L.; Cahalan, M.D.; et al. STIM1, an essential and conserved component of store-operated Ca2+ channel function. J. Cell. Biol. 2005, 169, 435–445. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  76. Vig, M.; Peinelt, C.; Beck, A.; Koomoa, D.L.; Rabah, D.; Koblan-Huberson, M.; Kraft, S.; Turner, H.; Fleig, A.; Penner, R.; et al. CRACM1 is a plasma membrane protein essential for store-operated Ca2+ entry. Science 2006, 312, 1220–1223. [Google Scholar] [CrossRef] [Green Version]
  77. González-Sánchez, P.; Del Arco, A.; Esteban, J.A.; Satrústegui, J. Store-Operated Calcium Entry Is Required for mGluR-Dependent Long Term Depression in Cortical Neurons. Front. Cell. Neurosci. 2017, 11, 363. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  78. Lunz, V.; Romanin, C.; Frischauf, I. STIM1 activation of Orai1. Cell Calcium 2019, 77, 29–38. [Google Scholar] [CrossRef]
  79. Conte, E.; Pannunzio, A.; Imbrici, P.; Camerino, G.M.; Maggi, L.; Mora, M.; Gibertini, S.; Cappellari, O.; De Luca, A.; Coluccia, M.; et al. Gain-of-Function STIM1 L96V Mutation Causes Myogenesis Alteration in Muscle Cells From a Patient Affected by Tubular Aggregate Myopathy. Front. Cell. Dev. Biol. 2021, 9, 635063. [Google Scholar] [CrossRef] [PubMed]
  80. Feske, S.; Gwack, Y.; Prakriya, M.; Srikanth, S.; Puppel, S.H.; Tanasa, B.; Hogan, P.G.; Lewis, R.S.; Daly, M.; Rao, A. A mutation in Orai1 causes immune deficiency by abrogating CRAC channel function. Nature 2006, 441, 179–185. [Google Scholar] [CrossRef]
  81. Hou, X.; Pedi, L.; Diver, M.M.; Long, S.B. Crystal structure of the calcium release-activated calcium channel Orai. Science 2012, 338, 1308–1313. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  82. Wang, X.; Wang, Y.; Zhou, Y.; Hendron, E.; Mancarella, S.; Andrake, M.D.; Rothberg, B.S.; Soboloff, J.; Gill, D.L. Distinct Orai-coupling domains in STIM1 and STIM2 define the Orai-activating site. Nat. Commun. 2014, 5, 3183. [Google Scholar] [CrossRef] [PubMed]
  83. Schaballie, H.; Rodriguez, R.; Martin, E.; Moens, L.; Frans, G.; Lenoir, C.; Dutré, J.; Canioni, D.; Bossuyt, X.; Fischer, A.; et al. A novel hypomorphic mutation in STIM1 results in a late-onset immunodeficiency. J. Allergy Clin. Immunol. 2015, 136, 816–819. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  84. Stormorken, H.; Sjaastad, O.; Langslet, A.; Sulg, I.; Egge, K.; Diderichsen, J. A new syndrome: Thrombocytopathia, muscle fatigue, asplenia, miosis, migraine, dyslexia and ichthyosis. Clin. Genet. 1985, 28, 67–74. [Google Scholar] [CrossRef] [PubMed]
  85. Mizobuchi, M.; Tanaka, C.; Sako, K.; Murakami, N.; Nihira, A.; Abe, T.; Tateno, Y.; Takahashi, T.; Nonaka, I. Muscle involvement of Stormorken’s syndrome. Rinsho Shinkeigaku 2000, 40, 915–920. [Google Scholar] [PubMed]
  86. Markello, T.; Chen, D.; Kwan, J.Y.; Horkayne-Szakaly, I.; Morrison, A.; Simakova, O.; Maric, I.; Lozier, J.; Cullinane, A.R.; Kilo, T.; et al. York platelet syndrome is a CRAC channelopathy due to gain-of-function mutations in STIM1. Mol. Genet. Metab. 2015, 114, 474–482. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  87. Cameron, C.H.S.; Allen, I.V.; Patterson, V.; Avaria, M.A. Dominantly inherited tubular aggregate myopathy. J. Pathol. 1992, 168, 397–403. [Google Scholar] [CrossRef] [PubMed]
  88. Engel, W.K. Mitochondrial Aggregates In Muscle Disease. J. Histochem. Cytochem. 1964, 12, 46–48. [Google Scholar] [CrossRef] [Green Version]
  89. Nesin, V.; Wiley, G.; Kousi, M.; Ong, E.C.; Lehmann, T.; Nicholl, D.J.; Suri, M.; Shahrizaila, N.; Katsanis, N.; Gaffney, P.M.; et al. Activating mutations in STIM1 and ORAI1 cause overlapping syndromes of tubular myopathy and congenital miosis. Proc. Nat. Acad. Sci. USA 2014, 111, 4197–4202. [Google Scholar] [CrossRef] [Green Version]
  90. Morin, G.; Bruechle, N.O.; Singh, A.R.; Knopp, C.; Jedraszak, G.; Elbracht, M.; Brémond-Gignac, D.; Hartmann, K.; Sevestre, H.; Deutz, P.; et al. Gain-of-function mutation in STIM1 (P.R304W) is associated with Stormorken syndrome. Hum. Mutat. 2014, 35, 1221–1232. [Google Scholar] [CrossRef]
  91. Guergueltcheva, V.; Müller, J.S.; Dusl, M.; Senderek, J.; Oldfors, A.; Lindbergh, C.; Maxwell, S.; Colomer, J.; Mallebrera, C.J.; Nascimento, A.; et al. Congenital myasthenic syndrome with tubular aggregates caused by GFPT1 mutations. J. Neurol. 2012, 259, 838–850. [Google Scholar] [CrossRef]
  92. Belaya, K.; Finlayson, S.; Slater, C.R.; Cossins, J.; Liu, W.W.; Maxwell, S.; McGowan, S.J.; Maslau, S.; Twigg, S.R.; Walls, T.J.; et al. Mutations in DPAGT1 cause a limb-girdle congenital myasthenic syndrome with tubular aggregates. Am. J. Hum. Genet. 2012, 91, 193–201. [Google Scholar] [CrossRef] [Green Version]
  93. Sternberg, D.; Maisonobe, T.; Jurkat-Rott, K.; Nicole, S.; Launay, E.; Chauveau, D.; Tabti, N.; Lehmann-Horn, F.; Hainque, B.; Fontaine, B. Hypokalaemic periodic paralysis type 2 caused by mutations at codon 672 in the muscle sodium channel gene SCN4A. Brain 2001, 124, 1091–1099. [Google Scholar] [CrossRef] [Green Version]
  94. Böhm, J.; Chevessier, F.; De Paula, A.M.; Koch, C.; Attarian, S.; Feger, C.; Hantaï, D.; Laforêt, P.; Ghorab, K.; Vallat, J.M.; et al. Constitutive activation of the calcium sensor STIM1 causes tubular-aggregate myopathy. Am. J. Hum. Genet. 2013, 92, 271–278. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  95. Böhm, J.; Chevessier, F.; Koch, C.; Peche, G.A.; Mora, M.; Morandi, L.; Pasanisi, B.; Moroni, I.; Tasca, G.; Fattori, F.; et al. Clinical, histological and genetic characterisation of patients with tubular aggregate myopathy caused by mutations in STIM1. J. Med. Genet. 2014, 51, 824–833. [Google Scholar] [CrossRef] [PubMed]
  96. Hedberg, C.; Niceta, M.; Fattori, F.; Lindvall, B.; Ciolfi, A.; D’Amico, A.; Tasca, G.; Petrini, S.; Tulinius, M.; Tartaglia, M.; et al. Childhood onset tubular aggregate myopathy associated with de novo STIM1 mutations. J. Neurol. 2014, 261, 870–876. [Google Scholar] [CrossRef] [PubMed]
  97. Claeys, T.; Goosens, V.; Racé, V.; Theys, T.; Thal, D.R.; Depuydt, C.E.; Claeys, K.G. Clinical and muscle MRI features in a family with tubular aggregate myopathy and novel STIM1 mutation. Neuromuscul. Disord. 2020, 30, 709–718. [Google Scholar] [CrossRef] [PubMed]
  98. Silva-Rojas, R.; Laporte, J.; Böhm, J. STIM1/ORAI1 Loss-of-Function and Gain-of-Function Mutations Inversely Impact on SOCE and Calcium Homeostasis and Cause Multi-Systemic Mirror Diseases. Front. Physiol. 2020, 11, 604941. [Google Scholar] [CrossRef] [PubMed]
  99. Misceo, D.; Holmgren, A.; Louch, W.E.; Holme, P.A.; Mizobuchi, M.; Morales, R.J.; De Paula, A.M.; Stray-Pedersen, A.; Lyle, R.; Dalhus, B.; et al. A dominant STIM1 mutation causes Stormorken syndrome. Hum. Mutat. 2014, 35, 556–564. [Google Scholar] [CrossRef]
  100. Endo, Y.; Noguchi, S.; Hara, Y.; Hayashi, Y.K.; Motomura, K.; Miyatake, S.; Murakami, N.; Tanaka, S.; Yamashita, S.; Kizu, R.; et al. Dominant mutations in ORAI1 cause tubular aggregate myopathy with hypocalcemia via constitutive activation of store-operated Ca(2)(+) channels. Hum. Mol. Genet. 2015, 24, 637–648. [Google Scholar] [CrossRef] [Green Version]
  101. Böhm, J.; Bulla, M.; Urquhart, J.E.; Malfatti, E.; Williams, S.G.; O’Sullivan, J.; Szlauer, A.; Koch, C.; Baranello, G.; Mora, M.; et al. ORAI1 Mutations with Distinct Channel Gating Defects in Tubular Aggregate Myopathy. Hum. Mutat. 2017, 38, 426–438. [Google Scholar] [CrossRef] [Green Version]
  102. Garibaldi, M.; Fattori, F.; Riva, B.; Labasse, C.; Brochier, G.; Ottaviani, P.; Sacconi, S.; Vizzaccaro, E.; Laschena, F.; Romero, N.B.; et al. A novel gain-of-function mutation in ORAI1 causes late-onset tubular aggregate myopathy and congenital miosis. Clin. Genet. 2017, 91, 780–786. [Google Scholar] [CrossRef] [PubMed]
  103. Stauderman, K.A. CRAC channels as targets for drug discovery and development. Cell. Calcium. 2018, 74, 147–159. [Google Scholar] [CrossRef]
  104. Phillips, M.S.; Fujii, J.; Khanna, V.K.; DeLeon, S.; Yokobata, K.; de Jong, P.J.; MacLennan, D.H. The structural organization of the human skeletal muscle ryanodine receptor (RYR1) gene. Genomics 1996, 34, 24–41. [Google Scholar] [CrossRef] [PubMed]
  105. Dowling, J.J.D.; Gonorazky, H.; Cohn, R.D.; Campbell, C. Treating pediatric neuromuscular disorders: The future is now. Am. J. Med. Genet. A 2018, 176, 804–841. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  106. Klein, A.; Lillis, S.; Munteanu, I.; Scoto, M.; Zhou, H.; Quinlivan, R.; Straub, V.; Manzur, A.Y.; Roper, H.; Jeannet, P.Y.; et al. Clinical and genetic findings in a large cohort of patients with ryanodine receptor 1 gene-associated myopathies. Hum. Mutat. 2012, 33, 981–988. [Google Scholar] [CrossRef] [PubMed]
  107. Dlamini, N.; Voermans, N.C.; Lillis, S.; Stewart, K.; Kamsteeg, E.J.; Drost, G.; Quinlivan, R.; Snoeck, M.; Norwood, F.; Radunovic, A.; et al. Mutations in RYR1 are a common cause of exertional myalgia and rhabdomyolysis. Neuromuscul. Disord. 2013, 23, 540–548. [Google Scholar] [CrossRef]
  108. Løseth, S.; Voermans, N.C.; Torbergsen, T.; Lillis, S.; Jonsrud, C.; Lindal, S.; Kamsteeg, E.J.; Lammens, M.; Broman, M.; Dekomien, G.; et al. A novel late-onset axial myopathy associated with mutations in the skeletal muscle ryanodine receptor (RYR1) gene. J. Neurol. 2013, 260, 1504–1510. [Google Scholar] [CrossRef] [PubMed]
  109. Zou, Y.; Liang, Y.; Gong, H.; Zhou, N.; Ma, H.; Guan, A.; Sun, A.; Wang, P.; Niu, Y.; Jiang, H.; et al. Ryanodine receptor type 2 is required for the development of pressure overload-induced cardiac hypertrophy. Hypertension 2011, 58, 1099–1110. [Google Scholar] [CrossRef] [Green Version]
  110. Zhou, H.; Rokach, O.; Feng, L.; Munteanu, I.; Mamchaoui, K.; Wilmshurst, J.M.; Sewry, C.; Manzur, A.Y.; Pillay, K.; Mouly, V.; et al. RyR1 deficiency in congenital myopathies disrupts excitation-contraction coupling. Hum. Mutat. 2013, 34, 986–996. [Google Scholar] [CrossRef] [Green Version]
  111. Garibaldi, M.; Rendu, J.; Brocard, J.; Lacene, E.; Fauré, J.; Brochier, G.; Beuvin, M.; Labasse, C.; Madelaine, A.; Malfatti, E.; et al. Dusty core disease (DuCD): Expanding morphological spectrum of RYR1 recessive myopathies. Acta Neuropathol. Commun. 2019, 7, 3. [Google Scholar] [CrossRef] [PubMed]
  112. Matthews, E.; Neuwirth, C.; Jaffer, F.; Scalco, R.S.; Fialho, D.; Parton, M.; Rayan, D.R.; Suetterlin, K.; Sud, R.; Spiegel, R.; et al. Atypical periodic paralysis and myalgia: A novel RYR1 phenotype. Neurology 2018, 90, e412–e418. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  113. Lawal, T.A.; Todd, J.J.; Witherspoon, J.W.; Bönnemann, C.G.; Dowling, J.J.; Hamilton, S.L.; Meilleur, K.G.; Dirksen, R.T. Ryanodine receptor 1-related disorders: An historical perspective and proposal for a unified nomenclature. Skelet. Muscle 2020, 10, 32. [Google Scholar] [CrossRef] [PubMed]
  114. Davis, M.R.; Haan, E.; Jungbluth, H.; Sewry, C.; North, K.; Muntoni, F.; Kuntzer, T.; Lamont, P.; Bankier, A.; Tomlinson, P.; et al. Principal mutation hotspot for central core disease and related myopathies in the C-terminal transmembrane region of the RYR1 gene. Neuromuscul. Disord. 2003, 13, 151–157. [Google Scholar] [CrossRef]
  115. Levano, S.; Vukcevic, M.; Singer, M.; Matter, A.; Treves, S.; Urwyler, A.; Girard, T. Increasing the number of diagnostic mutations in malignant hyperthermia. Hum. Mutat. 2009, 30, 590–598. [Google Scholar] [CrossRef] [PubMed]
  116. Robinson, R.; Carpenter, D.; Shaw, M.A.; Halsall, J.; Hopkins, P. Mutations in RYR1 in malignant hyperthermia and central core disease. Hum. Mutat. 2006, 27, 977–989. [Google Scholar] [CrossRef] [PubMed]
  117. Wu, S.; Ibarra, M.C.; Malicdan, M.C.; Murayama, K.; Ichihara, Y.; Kikuchi, H.; Nonaka, I.; Noguchi, S.; Hayashi, Y.K.; Nishino, I. Central core disease is due to RYR1 mutations in more than 90% of patients. Brain 2006, 129, 1470–1480. [Google Scholar] [CrossRef] [Green Version]
  118. Zhou, H.; Jungbluth, H.; Sewry, C.A.; Feng, L.; Bertini, E.; Bushby, K.; Straub, V.; Roper, H.; Rose, M.R.; Brockington, M.; et al. Molecular mechanisms and phenotypic variation in RYR1-related congenital myopathies. Brain 2007, 130, 2024–2036. [Google Scholar] [CrossRef] [Green Version]
  119. Maggi, L.; Scoto, M.; Cirak, S.; Robb, S.A.; Klein, A.; Lillis, S.; Cullup, T.; Feng, L.; Manzur, A.Y.; Sewry, C.A.; et al. Congenital myopathies—clinical features and frequency of individual subtypes diagnosed over a 5-year period in the United Kingdom. Neuromuscul. Disord. 2013, 23, 195–205. [Google Scholar] [CrossRef]
  120. Colombo, I.; Scoto, M.; Manzur, A.Y.; Robb, S.A.; Maggi, L.; Gowda, V.; Cullup, T.; Yau, M.; Phadke, R.; Sewry, C.; et al. Congenital myopathies: Natural history of a large pediatric cohort. Neurology 2015, 84, 28–35. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  121. Jungbluth, H. Central core disease. Orphanet J. Rare Dis. 2007, 2, 25. [Google Scholar] [CrossRef] [Green Version]
  122. Jungbluth, H. Multi-minicore disease. Orphanet J. Rare Dis. 2007, 2, 31. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  123. Clarke, N.F.; Waddell, L.B.; Cooper, S.T.; Perry, M.; Smith, R.L.; Kornberg, A.J.; Muntoni, F.; Lillis, S.; Straub, V.; Bushby, K.; et al. Recessive mutations in RYR1 are a common cause of congenital fibre type disproportion. Hum. Mutat. 2010, 31, e1544–e1550. [Google Scholar] [CrossRef] [PubMed]
  124. Monnier, N.; Marty, I.; Faure, J.; Castiglioni, C.; Desnuelle, C.; Sacconi, S.; Estournet, B.; Ferreiro, A.; Romero, N.; Laquerriere, A.; et al. Null mutations causing depletion of the type 1 ryanodine receptor (RYR1) are commonly associated with recessive structural congenital myopathies with cores. Hum. Mutat. 2008, 29, 670–678. [Google Scholar] [CrossRef]
  125. Monnier, N.; Romero, N.B.; Lerale, J.; Nivoche, Y.; Qi, D.; MacLennan, D.H.; Fardeau, M.; Lunardi, J. An autosomal dominant congenital myopathy with cores and rods is associated with a neomutation in the RYR1 gene encoding the skeletal muscle ryanodine receptor. Hum. Mol. Genet. 2000, 9, 2599–2608. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  126. Jungbluth, H.; Dowling, J.J.; Ferreiro, A.; Muntoni, F. 182nd ENMC International Workshop: RYR1-related myopathies, 15-17th April 2011, Naarden, The Netherlands. Neuromuscul. Disord. 2012, 22, 453–462. [Google Scholar] [CrossRef]
  127. Wilmshurst, J.M.; Lillis, S.; Zhou, H.; Pillay, K.; Henderson, H.; Kress, W.; Müller, C.R.; Ndondo, A.; Cloke, V.; Cullup, T.; et al. RYR1 mutations are a common cause of congenital myopathies with central nuclei. Ann. Neurol. 2010, 68, 717–726. [Google Scholar] [CrossRef] [Green Version]
  128. Ferreiro, A.; Monnier, N.; Romero, N.B.; Leroy, J.P.; Bönnemann, C.; Haenggeli, C.A.; Straub, V.; Voss, W.D.; Nivoche, Y.; Jungbluth, H.; et al. A recessive form of central core disease, transiently presenting as multi-minicore disease, is associated with a homozygous mutation in the ryanodine receptor type 1 gene. Ann. Neurol. 2002, 51, 750–759. [Google Scholar] [CrossRef] [PubMed]
  129. Romero, N.B.; Monnier, N.; Viollet, L.; Cortey, A.; Chevallay, M.; Leroy, J.P.; Lunardi, J.; Fardeau, M. Dominant and recessive central core disease associated with RYR1 mutations and fetal akinesia. Brain 2003, 126, 2341–2349. [Google Scholar] [CrossRef] [PubMed]
  130. De Wel, B.; Claeys, K.G. Malignant hyperthermia: Still an issue for neuromuscular diseases? Curr. Opin. Neurol. 2018, 31, 628–634. [Google Scholar] [CrossRef] [PubMed]
  131. Carpenter, D.; Robinson, R.L.; Quinnell, R.J.; Ringrose, C.; Hogg, M.; Casson, F.; Booms, P.; Iles, D.E.; Halsall, P.J.; Steele, D.S.; et al. Genetic variation in RYR1 and malignant hyperthermia phenotypes. Br. J. Anaesth. 2009, 103, 538–548. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  132. Rosenberg, H.; Pollock, N.; Schiemann, A.; Bulger, T.; Stowell, K. Malignant hyperthermia: A review. Orphanet J. Rare Dis. 2015, 10, 93. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  133. Lehmann-Horn, F.; Iaizzo, P.A. Are myotonias and periodic paralyses associated with susceptibility to malignant hyper—thermia? Br. J. Anaesth. 1990, 65, 692–697. [Google Scholar] [CrossRef]
  134. Dowling, J.J.; Lillis, S.; Amburgey, K.; Zhou, H.; Al-Sarraj, S.; Buk, S.J.; Wraige, E.; Chow, G.; Abbs, S.; Leber, S.; et al. King-Denborough syndrome with and without mutations in the skeletal muscle ryanodine receptor (RYR1) gene. Neuromuscul. Disord. 2011, 21, 420–427. [Google Scholar] [CrossRef] [PubMed]
  135. Jungbluth, H.; Lillis, S.; Zhou, H.; Abbs, S.; Sewry, C.; Swash, M.; Muntoni, F. Late-onset axial myopathy with cores due to a novel heterozygous dominant mutation in the skeletal muscle ryanodine receptor (RYR1) gene. Neuromuscul. Disord. 2009, 19, 344–347. [Google Scholar] [CrossRef] [PubMed]
  136. Zhou, H.; Lillis, S.; Loy, R.E.; Ghassemi, F.; Rose, M.R.; Norwood, F.; Mills, K.; Al-Sarraj, S.; Lane, R.J.; Feng, L.; et al. Multi-minicore disease and atypical periodic paralysis associated with novel mutations in the skeletal muscle ryanodine receptor (RYR1) gene. Neuromuscul. Disord. 2010, 20, 166–173. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  137. Bertocchini, F.; Ovitt, C.E.; Conti, A.; Barone, V.; Schöler, H.R.; Bottinelli, R.; Reggiani, C.; Sorrentino, V. Requirement for the ryanodine receptor type 3 for efficient contraction in neonatal skeletal muscles. EMBO J. 1997, 16, 6956–6963. [Google Scholar] [CrossRef]
  138. Perez, C.F.; López, J.R.; Allen, P.D. Expression levels of RyR1 and RyR3 control resting free Ca2+ in skeletal muscle. Am. J. Physiol. Cell. Physiol. 2005, 88, C640–C649. [Google Scholar] [CrossRef] [PubMed]
  139. Nilipour, Y.; Nafissi, S.; Tjust, A.E.; Ravenscroft, G.; Hossein Nejad Nedai, H.; Taylor, R.L.; Varasteh, V.; Pedrosa Domellöf, F.; Zangi, M.; Tonekaboni, S.H.; et al. Ryanodine receptor type 3 (RYR3) as a novel gene associated with a myopathy with nemaline bodies. Eur. J. Neurol. 2018, 25, 841–847. [Google Scholar] [CrossRef]
  140. Krüger, J.; Kunert-Keil, C.; Bisping, F.; Brinkmeier, H. Transient receptor potential cation channels in normal and dystrophic mdx muscle. Neuromuscul. Disord. 2008, 18, 501–513. [Google Scholar] [CrossRef] [PubMed]
  141. Ho, T.C.; Horn, N.A.; Huynh, T.; Kelava, L.; Lansman, J.B. Evidence TRPV4 contributes to mechanosensitive ion channels in mouse skeletal muscle fibers. Channels 2012, 6, 246–254. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  142. Pritschow, B.W.; Lange, T.; Kasch, J.; Kunert-Keil, C.; Liedtke, W.; Brinkmeier, H. Functional TRPV4 channels are expressed in mouse skeletal muscle and can modulate resting Ca2+ influx and muscle fatigue. Pflug. Arch. 2011, 46, 115–122. [Google Scholar] [CrossRef] [PubMed]
  143. Auer-Grumbach, M.; Olschewski, A.; Papić, L.; Kremer, H.; McEntagart, M.E.; Uhrig, S.; Fischer, C.; Fröhlich, E.; Bálint, Z.; Tang, B.; et al. Alterations in the ankyrin domain of TRPV4 cause congenital distal SMA, scapuloperoneal SMA and HMSN2C. Nat. Genet. 2010, 42, 160–164. [Google Scholar] [CrossRef] [PubMed]
  144. Deng, H.X.; Klein, C.J.; Yan, J.; Shi, Y.; Wu, Y.; Fecto, F.; Yau, H.J.; Yang, Y.; Zhai, H.; Siddique, N.; et al. Scapuloperoneal spinal muscular atrophy and CMT2C are allelic disorders caused by alterations in TRPV4. Nat. Genet. 2010, 42, 165–169. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  145. Landouré, G.; Zdebik, A.A.; Martinez, T.L.; Burnett, B.G.; Stanescu, H.C.; Inada, H.; Shi, Y.; Taye, A.A.; Kong, L.; Munns, C.H.; et al. Mutations in TRPV4 cause Charcot-Marie-Tooth disease type 2C. Nat. Genet. 2010, 42, 170–174. [Google Scholar] [CrossRef] [PubMed]
  146. Zimoń, M.; Baets, J.; Auer-Grumbach, M.; Berciano, J.; Garcia, A.; Lopez-Laso, E.; Merlini, L.; Hilton-Jones, D.; McEntagart, M.; Crosby, A.H.; et al. Dominant mutations in the cation channel gene transient receptor potential vanilloid 4 cause an unusual spectrum of neuropathies. Brain 2010, 133, 1798–1809. [Google Scholar] [CrossRef] [Green Version]
  147. Rock, M.J.; Prenen, J.; Funari, V.A.; Funari, T.L.; Merriman, B.; Nelson, S.F.; Lachman, R.S.; Wilcox, W.R.; Reyno, S.; Quadrelli, R.; et al. Gain-of-function mutations in TRPV4 cause autosomal dominant brachyolmia. Nat. Genet. 2008, 40, 999–1003. [Google Scholar] [CrossRef] [Green Version]
  148. Krakow, D.; Vriens, J.; Camacho, N.; Luong, P.; Deixler, H.; Funari, T.L.; Bacino, C.A.; Irons, M.B.; Holm, I.A.; Sadler, L.; et al. Mutations in the gene encoding the calcium-permeable ion channel TRPV4 produce spondylometaphyseal dysplasia, Kozlowski type and metatropic dysplasia. Am. J. Hum. Genet. 2009, 84, 307–315. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  149. Cho, T.J.; Matsumoto, K.; Fano, V.; Dai, J.; Kim, O.H.; Chae, J.H.; Yoo, W.J.; Tanaka, Y.; Matsui, Y.; Takigami, I.; et al. TRPV4-pathy manifesting both skeletal dysplasia and peripheral neuropathy: A report of three patients. Am. J. Med. Genet. A 2012, 158A, 795–802. [Google Scholar] [CrossRef] [PubMed]
  150. Echaniz-Laguna, A.; Dubourg, O.; Carlier, P.; Carlier, R.Y.; Sabouraud, P.; Péréon, Y.; Chapon, F.; Thauvin-Robinet, C.; Laforêt, P.; Eymard, B.; et al. Phenotypic spectrum and incidence of TRPV4 mutations in patients with inherited axonal neuropathy. Neurology 2014, 82, 1919–1926. [Google Scholar] [CrossRef]
  151. Oonk, A.M.; Ekker, M.S.; Huygen, P.L.; Kunst, H.P.; Kremer, H.; Schelhaas, J.J.; Pennings, R.J. Intrafamilial variable hearing loss in TRPV4 induced spinal muscular atrophy. Ann. Otol. Rhinol. Laryngol. 2014, 123, 859–865. [Google Scholar] [CrossRef] [PubMed]
  152. Evangelista, T.; Bansagi, B.; Pyle, A.; Griffin, H.; Douroudis, K.; Polvikoski, T.; Antoniadi, T.; Bushby, K.; Straub, V.; Chinnery, P.F.; et al. Phenotypic variability of TRPV4 related neuropathies. Neuromuscul. Disord. 2015, 25, 516–521. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  153. Koutsis, G.; Lynch, D.; Manole, A.; Karadima, G.; Reilly, M.M.; Houlden, H.; Panas, M. Charcot-Marie-Tooth disease type 2C and scapuloperoneal muscular atrophy overlap syndrome in a patient with the R232C TRPV4 mutation. J. Neurol. 2015, 262, 1972–1975. [Google Scholar] [CrossRef] [PubMed]
  154. Ürel-Demir, G.; Şimşek-Kiper, P.Ö.; Öncel, İ.; Utine, G.E.; Haliloğlu, G.; Boduroğlu, K. Natural history of TRPV4-Related disorders: From skeletal dysplasia to neuromuscular phenotype. Eur. J. Paediatr. Neurol. 2021, 32, 46–55. [Google Scholar] [CrossRef] [PubMed]
  155. Sullivan, J.M.; Zimanyi, C.M.; Aisenberg, W.; Bears, B.; Chen, D.H.; Day, J.W.; Bird, T.D.; Siskind, C.E.; Gaudet, R.; Sumner, C.J. Novel mutations highlight the key role of the ankyrin repeat domain in TRPV4-mediated neuropathy. Neurol. Genet. 2015, 1, e29. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  156. Woolums, B.M.; McCray, B.A.; Sung, H.; Tabuchi, M.; Sullivan, J.M.; Ruppell, K.T.; Yang, Y.; Mamah, C.; Aisenberg, W.H.; Saavedra-Rivera, P.C.; et al. TRPV4 disrupts mitochondrial transport and causes axonal degeneration via a CaMKII-dependent elevation of intracellular Ca2+. Nat. Commun. 2020, 11, 2679. [Google Scholar] [CrossRef] [PubMed]
  157. Dupont, C.; Novak, K.; Denman, K.; Myers, J.H.; Sullivan, J.M.; Walker, P.V., 2nd. TRPV4 Antagonism Prevents Mechanically Induced Myotonia. Ann. Neurol. 2020, 88, 297–308. [Google Scholar] [CrossRef] [PubMed]
  158. Goyal, N.; Skrdla, P.; Schroyer, R.; Kumar, S.; Fernando, D.; Oughton, A.; Norton, N.; Sprecher, D.L.; Cheriyan, J. Clinical Pharmacokinetics, Safety, and Tolerability of a Novel, First-in-Class TRPV4 Ion Channel Inhibitor, GSK2798745, in Healthy and Heart Failure Subjects. Am. J. Cardiovasc. Drugs 2019, 19, 335–342. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  159. Carter, M.T.; McMillan, H.J.; Tomin, A.; Weiss, N. Compound heterozygous CACNA1H mutations associated with severe congenital amyotrophy. Channels 2019, 13, 153–161. [Google Scholar] [CrossRef] [Green Version]
  160. Tawil, R.; Ptacek, L.J.; Pavlakis, S.G.; DeVivo, D.C.; Penn, A.S.; Ozdemir, C.; Griggs, R.C. Andersen’s syndrome: Potassium-sensitive periodic paralysis, ventricular ectopy, and dysmorphic features. Ann. Neurol. 1994, 35, 326–330. [Google Scholar] [CrossRef]
  161. Sansone, V.; Tawil, R. Management and treatment of Andersen-Tawil syndrome (ATS). Neurotherapeutics 2007, 4, 233–237. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  162. Pérez-Riera, A.R.; Barbosa-Barros, R.; Samesina, N.; Pastore, C.A.; Scanavacca, M.; Daminello-Raimundo, R.; de Abreu, L.C.; Nikus, K.; Brugada, P. Andersen-Tawil Syndrome: A Comprehensive Review. Cardiol. Rev. 2021, 29, 165–177. [Google Scholar] [CrossRef] [PubMed]
  163. Nguyen, H.L.; Pieper, G.H.; Wilders, R. Andersen-Tawil syndrome: Clinical and molecular aspects. Int. J. Cardiol. 2013, 170, 1–16. [Google Scholar] [CrossRef] [PubMed]
  164. Child, N.D.; Cleland, J.C.; Roxburgh, R. Andersen-Tawil syndrome presenting as a fixed myopathy. Muscle Nerve 2013, 48, 623. [Google Scholar] [CrossRef] [PubMed]
  165. Lefter, S.; Hardiman, O.; Costigan, D.; Lynch, B.; McConville, J.; Hand, C.K.; Ryan, A.M. Andersen-Tawil syndrome with early fixed myopathy. J. Clin. Neuromuscul. Dis. 2014, 16, 79–82. [Google Scholar] [CrossRef] [PubMed]
  166. Oz Tuncer, G.; Teber, S.; Kutluk, M.G.; Albayrak, P.; Deda, G. Andersen-Tawil Syndrome with Early Onset Myopathy: 2 Cases. J. Neuromuscul. Dis. 2017, 4, 93–95. [Google Scholar] [CrossRef] [PubMed]
  167. Wu, L.; Fang, Y.; Zhang, B.R. Andersen-Tawil syndrome associated with myopathy. World J. Emerg. Med. 2020, 11, 267–269. [Google Scholar] [CrossRef] [PubMed]
  168. Hiraide, T.; Fukumura, S.; Yamamoto, A.; Nakashima, M.; Saitsu, H. Familial periodic paralysis associated with a rare KCNJ5 variant that supposed to have incomplete penetrance. Brain. Dev. 2021, 43, 470–474. [Google Scholar] [CrossRef] [PubMed]
  169. Plaster, N.M.; Tawil, R.; Tristani-Firouzi, M.; Canún, S.; Bendahhou, S.; Tsunoda, A.; Donaldson, M.R.; Iannaccone, S.T.; Brunt, E.; Barohn, R.; et al. Mutations in Kir2.1 cause the developmental and episodic electrical phenotypes of Andersen’s syndrome. Cell 2001, 105, 511–519. [Google Scholar] [CrossRef] [Green Version]
  170. Lopes, C.M.; Zhang, H.; Rohacs, T.; Jin, T.; Yang, J.; Logothetis, D.E. Alterations in conserved Kir channel-PIP2 interactions underlie channelopathies. Neuron 2002, 34, 933–944. [Google Scholar] [CrossRef] [Green Version]
  171. Ballester, L.Y.; Benson, D.W.; Wong, B.; Law, I.H.; Mathews, K.D.; Vanoye, C.G.; George, A.L., Jr. Trafficking-competent and trafficking-defective KCNJ2 mutations in Andersen syndrome. Hum. Mutat. 2006, 27, 388. [Google Scholar] [CrossRef] [PubMed]
  172. Ma, D.; Tang, X.D.; Rogers, T.B.; Welling, P.A. An andersen-Tawil syndrome mutation in Kir2.1 (V302M) alters the G-loop cytoplasmic K+ conduction pathway. J. Biol. Chem. 2007, 282, 5781–5789. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  173. Handklo-Jamal, R.; Meisel, E.; Yakubovich, D.; Vysochek, L.; Beinart, R.; Glikson, M.; McMullen, J.R.; Dascal, N.; Nof, E.; Oz, S. Andersen-Tawil Syndrome Is Associated With Impaired PIP2 Regulation of the Potassium Channel Kir2.1. Front. Pharmacol. 2020, 11, 672. [Google Scholar] [CrossRef]
  174. Bendahhou, S.; Donaldson, M.R.; Plaster, N.M.; Tristani-Firouzi, M.; Fu, Y.H.; Ptácek, L.J. Defective potassium channel Kir2.1 trafficking underlies Andersen-Tawil syndrome. J. Biol. Chem. 2003, 278, 51779–51785. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  175. Bendahhou, S.; Fournier, E.; Sternberg, D.; Bassez, G.; Furby, A.; Sereni, C.; Donaldson, M.R.; Larroque, M.M.; Fontaine, B.; Barhanin, J. In vivo and in vitro functional characterization of Andersen’s syndrome mutations. J. Physiol. 2005, 565, 731–741. [Google Scholar] [CrossRef]
  176. Sacco, S.; Giuliano, S.; Sacconi, S.; Desnuelle, C.; Barhanin, J.; Amri, E.Z.; Bendahhou, S. The inward rectifier potassium channel Kir2.1 is required for osteoblastogenesis. Hum. Mol. Genet. 2015, 24, 471–479. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  177. Belus, M.T.; Rogers, M.A.; Elzubeir, A.; Josey, M.; Rose, S.; Andreeva, V.; Yelick, P.C.; Bates, E.A. Kir2.1 is important for efficient BMP signaling in mammalian face development. Dev. Biol. 2018, 444, S297–S307. [Google Scholar] [CrossRef] [PubMed]
  178. Pini, J.; Giuliano, S.; Matonti, J.; Gannoun, L.; Simkin, D.; Rouleau, M.; Bendahhou, S. Osteogenic and Chondrogenic Master Genes Expression Is Dependent on the Kir2.1 Potassium Channel Through the Bone Morphogenetic Protein Pathway. J. Bone Miner. Res. 2018, 33, 1826–1841. [Google Scholar] [CrossRef]
  179. Preisig-Müller, R.; Schlichthörl, G.; Goerge, T.; Heinen, S.; Brüggemann, A.; Rajan, S.; Derst, C.; Veh, R.W.; Daut, J. Heteromerization of Kir2.x potassium channels contributes to the phenotype of Andersen’s syndrome. Proc. Natl. Acad. Sci. USA 2002, 99, 7774–7779. [Google Scholar] [CrossRef] [Green Version]
  180. Decher, N.; Renigunta, V.; Zuzarte, M.; Soom, M.; Heinemann, S.H.; Timothy, K.W.; Keating, M.T.; Daut, J.; Sanguinetti, M.C.; Splawski, I. Impaired interaction between the slide helix and the C-terminus of Kir2.1: A novel mechanism of Andersen syndrome. Cardiovasc. Res. 2007, 75, 748–757. [Google Scholar] [CrossRef]
  181. Jagodzińska, M.; Szperl, M.; Ponińska, J.; Kosiec, A.; Gajda, R.; Kukla, P.; Biernacka, E.K. Coexistence of Andersen-Tawil Syndrome with Polymorphisms in hERG1 Gene (K897T) and SCN5A Gene (H558R) in One Family. Ann. Noninvasive Electrocardiol. 2016, 21, 189–195. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  182. Polyak, M.E.; Shestak, A.; Podolyak, D.; Zaklyazminskaya, E. Compound heterozygous mutations in KCNJ2 and KCNH2 in a patient with severe Andersen-Tawil syndrome. BMJ Case Rep. 2020, 13, e235703. [Google Scholar] [CrossRef]
  183. Priori, S.G.; Pandit, S.V.; Rivolta, I.; Berenfeld, O.; Ronchetti, E.; Dhamoon, A.; Napolitano, C.; Anumonwo, J.; Di Barletta, M.R.; Gudapakkam, S.; et al. A novel form of short QT syndrome (SQT3) is caused by a mutation in the KCNJ2 gene. Circ. Res. 2005, 96, 800–807. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  184. Xia, M.; Jin, Q.; Bendahhou, S.; He, Y.; Larroque, M.M.; Chen, Y.; Zhou, Q.; Yang, Y.; Liu, Y.; Liu, B.; et al. A Kir2.1 gain-of-function mutation underlies familial atrial fibrillation. Biochem. Biophys. Res. Commun. 2005, 332, 1012–1019. [Google Scholar] [CrossRef] [PubMed]
  185. Yang, Y.; Yang, Y.; Liang, B.; Liu, J.; Li, J.; Grunnet, M.; Olesen, S.P.; Rasmussen, H.B.; Ellinor, P.T.; Gao, L.; et al. Identification of a Kir3.4 mutation in congenital long QT syndrome. Am. J. Hum. Genet. 2010, 86, 872–880. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  186. Kokunai, Y.; Nakata, T.; Furuta, M.; Sakata, S.; Kimura, H.; Aiba, T.; Yoshinaga, M.; Osaki, Y.; Nakamori, M.; Itoh, H.; et al. A Kir3.4 mutation causes Andersen-Tawil syndrome by an inhibitory effect on Kir2.1. Neurology 2014, 82, 1058–1064. [Google Scholar] [CrossRef] [PubMed]
  187. Nagamine, S.; Sakoda, S.; Koide, R.; Kawata, A.; Yuan, J.; Takashima, H.; Nakano, I. A case of Andersen-Tawil syndrome presenting periodic paralysis exacerbated by ACZ. J. Neurol. Sci. 2014, 347, 385–386. [Google Scholar] [CrossRef]
  188. Abott, G.W.; Butler, M.H.; Bendahhou, S.; Dalakas, M.C.; Ptacek, L.J.; Goldstein, S.A. MiRP2 forms potassium channels in skeletal muscle with Kv3.4 and is associated with periodic paralysis. Cell 2001, 104, 217–231. [Google Scholar] [CrossRef] [Green Version]
  189. Dias Da Silva, M.R.; Cerutti, J.M.; Arnaldi, L.A.; Maciel, R.M. A mutation in the KCNE3 potassium channel gene is associated with susceptibility to thyrotoxic hypokalemic periodic paralysis. J. Clin. Endocrinol. Metab. 2002, 87, 4881–4884. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  190. Sternberg, D.; Tabti, N.; Fournier, E.; Hainque, B.; Fontaine, B. Lack of association of the potassium channel-associated peptide MiRP2-R83H variant with periodic paralysis. Neurology 2003, 61, 857–859. [Google Scholar] [CrossRef]
  191. Jurkat-Rott, K.; Lehmann-Horn, F. Periodic paralysis mutation MiRP2-R83H in controls: Interpretations and general recommendation. Neurology 2004, 62, 1012–1015. [Google Scholar] [CrossRef] [PubMed]
  192. Tang, N.L.; Chow, C.C.; Ko, G.T.; Tai, M.H.; Kwok, R.; Yao, X.Q.; Cockram, C.S. No mutation in the KCNE3 potassium channel gene in Chinese thyrotoxic hypokalaemic periodic paralysis patients. Clin. Endocrinol. 2004, 61, 109–112. [Google Scholar] [CrossRef]
  193. Abbott, G.W.; Butler, M.H.; Goldstein, S.A. Phosphorylation and protonation of neighboring MiRP2 sites: Function and pathophysiology of MiRP2-Kv3.4 potassium channels in periodic paralysis. FASEB J. 2006, 20, 293–301. [Google Scholar] [CrossRef]
  194. Portaro, S.; Altamura, C.; Licata, N.; Camerino, G.M.; Imbrici, P.; Musumeci, O.; Rodolico, C.; Camerino, D.C.; Toscano, A.; Desaphy, J.F. Clinical, Molecular, and Functional Characterization of CLCN1 Mutations in Three Families with Recessive Myotonia Congenita. Neuromol. Med. 2015, 17, 285–296. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  195. Imbrici, P.; Accogli, A.; Blunck, R.; Altamura, C.; Iacomino, M.; D’adamo, M.C.; Allegri, A.; Pedemonte, M.; Brolatti, N.; Vari, S.; et al. Musculoskeletal Features without Ataxia Associated with a Novel de novo Mutation in KCNA1 Impairing the Voltage Sensitivity of Kv1.1 Channel. Biomedicines 2021, 9, 75. [Google Scholar] [CrossRef] [PubMed]
  196. Salih, M.; van Kinschot, C.M.; Peeters, R.P.; de Herder, W.W.; Duschek, E.J.; Van Der Linden, J.; van Noord, C. Thyrotoxic periodic paralysis: An unusual presentation of hyperthyroidism. Neth. J. Med. 2017, 75, 315–320. [Google Scholar]
  197. Chu, P.Y.; Cheng, C.J.; Tseng, M.H.; Yang, S.S.; Chen, H.C.; Lin, S.H. Genetic variant rs623011 (17q24.3) associates with non-familial thyrotoxic and sporadic hypokalemic paralysis. Clin. Chim. Acta 2012, 414, 105–108. [Google Scholar] [CrossRef] [PubMed]
  198. Song, I.W.; Sung, C.C.; Chen, C.H.; Cheng, C.J.; Yang, S.S.; Chou, Y.C.; Yang, J.H.; Chen, Y.T.; Wu, J.Y.; Lin, S.H. Novel susceptibility gene for nonfamilial hypokalemic periodic paralysis. Neurology 2016, 86, 1190–1198. [Google Scholar] [CrossRef]
  199. Nakaza, M.; Kitamura, Y.; Furuta, M.; Kubota, T.; Sasaki, R.; Takahashi, M.P. Analysis of the genetic background associated with sporadic periodic paralysis in Japanese patients. J. Neurol. Sci. 2020, 412, 116795. [Google Scholar] [CrossRef] [PubMed]
  200. Cannon, S.C. Further evidence for shared genetic susceptibility in both sporadic and thyrotoxic periodic paralysis. J. Neurol. Sci. 2020, 412, 116794. [Google Scholar] [CrossRef] [PubMed]
  201. Ryan, D.P.; Da Silva, M.R.; Soong, T.W.; Fontaine, B.; Donaldson, M.R.; Kung, A.W.; Jongjaroenprasert, W.; Liang, M.C.; Khoo, D.H.; Cheah, J.S.; et al. Mutations in potassium channel Kir2.6 cause susceptibility to thyrotoxic hypokalemic periodic paralysis. Cell 2010, 140, 88–98. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  202. Cheng, C.J.; Lin, S.H.; Lo, Y.F.; Yang, S.S.; Hsu, Y.J.; Cannon, S.C.; Huang, C.L. Identification and functional characterization of Kir2.6 mutations associated with non-familial hypokalemic periodic paralysis. J. Biol. Chem. 2011, 286, 27425–27435. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  203. Zheng, J.; Liang, Z.; Hou, Y.; Liu, F.; Hu, Y.; Lin, P.; Yan, C. A novel Kir2.6 mutation associated with hypokalemic periodic paralysis. Clin. Neurophysiol. 2016, 127, 2503–2508. [Google Scholar] [CrossRef] [PubMed]
  204. Paninka, R.M.; Carlos-Lima, E.; Lindsey, S.C.; Kunii, I.S.; Dias-da-Silva, M.R.; Arcisio-Miranda, M. Down-regulation of Kir2.6 channel by c-termini mutation D252N and its association with the susceptibility to Thyrotoxic Periodic Paralysis. Neuroscience 2017, 346, 197–202. [Google Scholar] [CrossRef]
  205. Cheung, C.L.; Lau, K.S.; Ho, A.Y.; Lee, K.K.; Tiu, S.C.; Lau, E.Y.; Leung, J.; Tsang, M.W.; Chan, K.W.; Yeung, C.Y.; et al. Genome-wide association study identifies a susceptibility locus for thyrotoxic periodic paralysis at 17q24.3. Nat. Genet. 2012, 44, 1026–1029. [Google Scholar] [CrossRef] [PubMed]
  206. Jongjaroenprasert, W.; Phusantisampan, T.; Mahasirimongkol, S.; Mushiroda, T.; Hirankarn, N.; Snabboon, T.; Chanprasertyotin, S.; Tantiwong, P.; Soonthornpun, S.; Rattanapichart, P.; et al. A genome-wide association study identifies novel susceptibility genetic variation for thyrotoxic hypokalemic periodic paralysis. J. Hum. Genet. 2012, 57, 301–304. [Google Scholar] [CrossRef] [Green Version]
  207. Li, X.; Yao, S.; Xiang, Y.; Zhang, X.; Wu, X.; Luo, L.; Huang, H.; Zhu, M.; Wan, H.; Hong, D. The clinical and genetic features in a cohort of mainland Chinese patients with thyrotoxic periodic paralysis. BMC Neurol. 2015, 15, 38. [Google Scholar] [CrossRef] [Green Version]
  208. Rolim, A.L.; Lindsey, S.C.; Kunii, I.S.; Crispim, F.; Moisés, R.C.; Maciel, R.M.; Dias-da-Silva, M.R. The insulin-sensitivity sulphonylurea receptor variant is associated with thyrotoxic paralysis. J. Mol. Endocrinol. 2014, 53, 295–301. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  209. Kuhn, M.; Jurkat-Rott, K.; Lehmann-Horn, F. Rare KCNJ18 variants do not explain hypokalaemic periodic paralysis in 263 unrelated patients. J. Neurol. Neurosurg. Psychiatry 2016, 87, 49–52. [Google Scholar] [PubMed] [Green Version]
  210. Paninka, R.M.; Mazzotti, D.R.; Kizys, M.M.; Vidi, A.C.; Rodrigues, H.; Silva, S.P.; Kunii, I.S.; Furuzawa, G.K.; Arcisio-Miranda, M.; Dias-da-Silva, M.R. Whole genome and exome sequencing realignment supports the assignment of KCNJ12, KCNJ17, and KCNJ18 paralogous genes in thyrotoxic periodic paralysis locus: Functional characterization of two polymorphic Kir2.6 isoforms. Mol. Genet. Genom. 2016, 291, 1535–1544. [Google Scholar] [CrossRef] [PubMed]
  211. Smeland, M.F.; McClenaghan, C.; Roessler, H.I.; Savelberg, S.; Hansen, G.Å.; Hjellnes, H.; Arntzen, K.A.; Müller, K.I.; Dybesland, A.R.; Harter, T.; et al. ABCC9-related Intellectual disability Myopathy Syndrome is a KATP channelopathy with loss-of-function mutations in ABCC9. Nat. Commun. 2019, 10, 4457. [Google Scholar] [CrossRef] [PubMed]
  212. Tricarico, D.; Mele, A.; Lundquist, A.L.; Desai, R.R.; George, A.L., Jr.; Conte Camerino, D. Hybrid assemblies of ATP-sensitive K+ channels determine their muscle-type-dependent biophysical and pharmacological properties. Proc. Natl. Acad. Sci. USA 2006, 103, 1118–1123. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  213. Flagg, T.P.; Enkvetchakul, D.; Koster, J.C.; Nichols, C.G. Muscle KATP channels: Recent insights to energy sensing and myoprotection. Physiol. Rev. 2010, 90, 799–829. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  214. Browne, D.L.; Gancher, S.T.; Nutt, J.G.; Brunt, E.R.; Smith, E.A.; Kramer, P.; Litt, M. Episodic ataxia/myokymia syndrome is associated with point mutations in the human potassium channel gene, KCNA1. Nat. Genet. 1994, 8, 136–140. [Google Scholar] [CrossRef] [PubMed]
  215. Adelman, J.P.; Bond, C.T.; Pessia, M.; Maylie, J. Episodic ataxia results from voltage-dependent potassium channels with altered functions. Neuron 1995, 15, 1449–1454. [Google Scholar] [CrossRef] [Green Version]
  216. D’Adamo, M.C.; Liantonio, A.; Rolland, J.F.; Pessia, M.; Imbrici, P. Kv1.1 Channelopathies: Pathophysiological Mechanisms and Therapeutic Approaches. Int. J. Mol. Sci. 2020, 21, 2935. [Google Scholar] [CrossRef] [PubMed]
  217. Paulhus, K.; Ammerman, L.; Glasscock, E. Clinical Spectrum of KCNA1 Mutations: New Insights into Episodic Ataxia and Epilepsy Comorbidity. Int. J. Mol. Sci. 2020, 21, 2802. [Google Scholar] [CrossRef]
  218. Herson, P.S.; Virk, M.; Rustay, N.R.; Bond, C.T.; Crabbe, J.C.; Adelman, J.P.; Maylie, J. A mouse model of episodic ataxia type-1. Nat. Neurosci. 2003, 6, 378–383. [Google Scholar] [CrossRef]
  219. Begum, R.; Bakiri, Y.; Volynski, K.E.; Kullmann, D.M. Action potential broadening in a presynaptic channelopathy. Nat. Commun. 2016, 7, 12102. [Google Scholar] [CrossRef] [Green Version]
  220. Brunetti, O.; Imbrici, P.; Botti, F.M.; Pettorossi, V.E.; D’Adamo, M.C.; Valentino, M.; Zammit, C.; Mora, M.; Gibertini, S.; Di Giovanni, G.; et al. Kv1.1 knock-in ataxic mice exhibit spontaneous myokymic activity exacerbated by fatigue, ischemia and low temperature. Neurobiol. Dis. 2012, 47, 310–321. [Google Scholar] [CrossRef] [PubMed]
  221. Eunson, L.H.; Rea, R.; Zuberi, S.M.; Youroukos, S.; Panayiotopoulos, C.P.; Liguori, R.; Avoni, P.; McWilliam, R.C.; Stephenson, J.B.; Hanna, M.G.; et al. Clinical, genetic, and expression studies of mutations in the potassium channel gene KCNA1 reveal new phenotypic variability. Ann. Neurol. 2000, 48, 647–656. [Google Scholar] [CrossRef]
  222. Kinali, M.; Jungbluth, H.; Eunson, L.H.; Sewry, C.A.; Manzur, A.Y.; Mercuri, E.; Hanna, M.G.; Muntoni, F. Expanding the phenotype of potassium channelopathy: Severe neuromyotonia and skeletal deformities without prominent Episodic Ataxia. Neuromuscul. Disord. 2004, 14, 689–693. [Google Scholar] [CrossRef] [PubMed]
  223. Chen, H.; von Hehn, C.; Kaczmarek, L.K.; Ment, L.R.; Pober, B.R.; Hisama, F.M. Functional analysis of a novel potassium channel (KCNA1) mutation in hereditary myokymia. Neurogenetics 2007, 8, 131–135. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  224. Rogers, A.; Golumbek, P.; Cellini, E.; Doccini, V.; Guerrini, R.; Wallgren-Pettersson, C.; Thuresson, A.C.; Gurnett, C.A. De novo KCNA1 variants in the PVP motif cause infantile epileptic encephalopathy and cognitive impairment similar to recurrent KCNA2 variants. Am. J. Med. Genet. A 2018, 176, 1748–1752. [Google Scholar] [CrossRef]
  225. Russo, A.; Gobbi, G.; Pini, A.; Møller, R.S.; Rubboli, G. Encephalopathy related to status epilepticus during sleep due to a de novo KCNA1 variant in the Kv-specific Pro-Val-Pro motif: Phenotypic description and remarkable electroclinical response to ACTH. Epileptic. Disord. 2020, 22, 802–806. [Google Scholar] [PubMed]
  226. Trosclair, K.; Dhaibar, H.A.; Gautier, N.M.; Mishra, V.; Glasscock, E. Neuron-specific Kv1.1 deficiency is sufficient to cause epilepsy, premature death, and cardiorespiratory dysregulation. Neurobiol. Dis. 2020, 137, 104759. [Google Scholar] [CrossRef]
  227. Brugnoni, R.; Maggi, L.; Canioni, E.; Verde, F.; Gallone, A.; Ariatti, A.; Filosto, M.; Petrelli, C.; Logullo, F.O.; Esposito, M.; et al. Next-generation sequencing application to investigate skeletal muscle channelopathies in a large cohort of Italian patients. Neuromuscul. Disord. 2021, 31, 336–347. [Google Scholar] [CrossRef] [PubMed]
  228. Graves, T.D.; Cha, Y.H.; Hahn, A.F.; Barohn, R.; Salajegheh, M.K.; Griggs, R.C.; Bundy, B.N.; Jen, J.C.; Baloh, R.W.; Hanna, M.G. Episodic ataxia type 1: Clinical characterization, quality of life and genotype-phenotype correlation. Brain 2014, 137, 1009–1018. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  229. D’Adamo, M.C.; Hasan, S.; Guglielmi, L.; Servettini, I.; Cenciarini, M.; Catacuzzeno, L.; Franciolini, F. New insights into the pathogenesis and therapeutics of episodic ataxia type 1. Front. Cell. Neurosci. 2015, 9, 317. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  230. Jentsch, T.J.; Pusch, M. CLC Chloride Channels and Transporters: Structure, Function, Physiology, and Disease. Physiol. Rev. 2018, 98, 1493–1590. [Google Scholar] [CrossRef]
  231. Altamura, C.; Desaphy, J.F.; Conte, D.; De Luca, A.; Imbrici, P. Skeletal muscle ClC-1 chloride channels in health and diseases. Pflug. Arch. 2020, 472, 961–975. [Google Scholar] [CrossRef]
  232. Steinmeyer, K.; Ortland, C.; Jentsch, T.J. Primary structure and functional expression of a developmentally regulated skeletal muscle chloride channel. Nature 1991, 354, 301–304. [Google Scholar] [CrossRef] [PubMed]
  233. Park, E.; MacKinnon, R. Structure of the CLC-1 chloride channel from Homo sapiens. eLife 2018, 7, e36629. [Google Scholar] [CrossRef] [PubMed]
  234. Wang, K.; Preisler, S.S.; Zhang, L.; Cui, Y.; Missel, J.W.; Grønberg, C.; Gotfryd, K.; Lindahl, E.; Andersson, M.; Calloe, K.; et al. Structure of the human ClC-1 chloride channel. PLoS Biol. 2019, 17, e3000218. [Google Scholar] [CrossRef] [Green Version]
  235. Koch, M.C.; Steinmeyer, K.; Lorenz, C.; Ricker, K.; Wolf, F.; Otto, M.; Zoll, B.; Lehmann-Horn, F.; Grzeschik, K.H.; Jentsch, T.J. The skeletal muscle chloride channel in dominant and recessive human myotonia. Science 1992, 257, 797–800. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  236. George, A.L., Jr.; Crackower, M.A.; Abdalla, J.A.; Hudson, A.J.; Ebers, G.C. Molecular basis of Thomsen’s disease (autosomal dominant myotonia congenita). Nat. Genet. 1993, 3, 305–310. [Google Scholar] [CrossRef]
  237. Trivedi, J.R.; Bundy, B.; Statland, J.; Salajegheh, M.; Rayan, D.R.; Venance, S.L.; Wang, Y.; Fialho, D.; Matthews, E.; Cleland, J.; et al. Non-dystrophic myotonia: Prospective study of objective and patient reported outcomes. Brain 2013, 136, 2189–2200. [Google Scholar] [CrossRef] [Green Version]
  238. Lo Monaco, M.; D’Amico, A.; Luigetti, M.; Desaphy, J.F.; Modoni, A. Effect of mexiletine on transitory depression of compound motor action potential in recessive myotonia congenita. Clin. Neurophysiol. 2015, 126, 399–403. [Google Scholar] [CrossRef]
  239. Fialho, D.; Schorge, S.; Pucovska, U.; Davies, N.P.; Labrum, R.; Haworth, A.; Stanley, E.; Sud, R.; Wakeling, W.; Davis, M.B.; et al. Chloride channel myotonia: Exon 8 hot-spot for dominant-negative interactions. Brain 2007, 130, 3265–3274. [Google Scholar] [CrossRef] [Green Version]
  240. Brugnoni, R.; Kapetis, D.; Imbrici, P.; Pessia, M.; Canioni, E.; Colleoni, L.; De Rosbo, N.K.; Morandi, L.; Cudia, P.; Gashemi, N.; et al. A large cohort of myotonia congenita probands: Novel mutations and a high-frequency mutation region in exons 4 and 5 of the CLCN1 gene. J. Hum. Genet. 2013, 58, 581–587. [Google Scholar] [CrossRef]
  241. Altamura, C.; Ivanova, E.A.; Imbrici, P.; Conte, E.; Camerino, G.M.; Dadali, E.L.; Polyakov, A.V.; Kurbatov, S.A.; Girolamo, F.; Carratù, M.R.; et al. Pathomechanisms of a CLCN1 Mutation Found in a Russian Family Suffering From Becker’s Myotonia. Front. Neurol. 2020, 11, 1019. [Google Scholar] [CrossRef]
  242. Rayan, D.R.; Haworth, A.; Sud, R.; Matthews, E.; Fialho, D.; Burge, J.; Portaro, S.; Schorge, S.; Tuin, K.; Lunt, P.; et al. A new explanation for recessive myotonia congenita: Exon deletions and duplications in CLCN1. Neurology 2012, 78, 1953–1958. [Google Scholar] [CrossRef] [Green Version]
  243. Saviane, C.; Conti, F.; Pusch, M. The muscle chloride channel ClC-1 has a double-barreled appearance that is differentially affected in dominant and recessive myotonia. J. Gen. Physiol. 1999, 113, 457–468. [Google Scholar] [CrossRef] [PubMed]
  244. Imbrici, P.; Altamura, C.; Camerino, G.M.; Mangiatordi, G.F.; Conte, E.; Maggi, L.; Brugnoni, R.; Musaraj, K.; Caloiero, R.; Alberga, D.; et al. Multidisciplinary study of a new ClC-1 mutation causing myotonia congenita: A paradigm to understand and treat ion channelopathies. FASEB J. 2016, 30, 3285–3295. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  245. Desaphy, J.F.; Gramegna, G.; Altamura, C.; Dinardo, M.M.; Imbrici, P.; George, A.L., Jr.; Modoni, A.; LoMonaco, M.; Camerino, D.C. Functional characterization of ClC-1 mutations from patients affected by recessive myotonia congenita presenting with different clinical phenotypes. Exp. Neurol. 2013, 248, 530–540. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  246. Altamura, C.; Lucchiari, S.; Sahbani, D.; Ulzi, G.; Comi, G.P.; D’Ambrosio, P.; Petillo, R.; Politano, L.; Vercelli, L.; Mongini, T.; et al. The analysis of myotonia congenita mutations discloses functional clusters of amino acids within the CBS2 domain and the C-terminal peptide of the ClC-1 channel. Hum. Mutat. 2018, 39, 1273–1283. [Google Scholar] [CrossRef] [PubMed]
  247. Imbrici, P.; Maggi, L.; Mangiatordi, G.F.; Dinardo, M.M.; Altamura, C.; Brugnoni, R.; Alberga, D.; Pinter, G.L.; Ricci, G.; Siciliano, G.; et al. ClC-1 mutations in myotonia congenita patients: Insights into molecular gating mechanisms and genotype-phenotype correlation. J. Physiol. 2015, 593, 4181–4199. [Google Scholar] [CrossRef] [Green Version]
  248. Weinberger, S.; Wojciechowski, D.; Sternberg, D.; Lehmann-Horn, F.; Jurkat-Rott, K.; Becher, T.; Begemann, B.; Fahlke, C.; Fischer, M. Disease-causing mutations C277R and C277Y modify gating of human ClC-1 chloride channels in myotonia congenita. J. Physiol. 2012, 590, 3449–3464. [Google Scholar] [CrossRef] [Green Version]
  249. Jeng, C.J.; Fu, S.J.; You, C.Y.; Peng, Y.J.; Hsiao, C.T.; Chen, T.Y.; Tang, C.Y. Defective Gating and Proteostasis of Human ClC-1 Chloride Channel: Molecular Pathophysiology of Myotonia Congenita. Front. Neurol. 2020, 11, 76. [Google Scholar] [CrossRef] [Green Version]
  250. Myers, J.H.; Denman, K.; DuPont, C.; Hawash, A.A.; Novak, K.R.; Koesters, A.; Grabner, M.; Dayal, A.; Voss, A.A.; Rich, M.M. The mechanism underlying transient weakness in myotonia congenita. eLife 2021, 10, e65691. [Google Scholar] [CrossRef]
  251. Markhorst, J.M.; Stunnenberg, B.C.; Ginjaar, I.B.; Drost, G.; Erasmus, C.E.; Sie, L.T. Clinical experience with long-term ACZ treatment in children with nondystrophic myotonias: A three-case report. Pediatr. Neurol. 2014, 51, 537–541. [Google Scholar] [CrossRef]
  252. Moreira, S.D.; Barreto, R.; Roriz, J.M. Becker myotonia-a recently identified mutation in Iberian descendants with apparent ACZ-responsive phenotype. Muscle Nerve 2015, 51, 933–934. [Google Scholar] [CrossRef] [PubMed]
  253. Eguchi, H.; Tsujino, A.; Kaibara, M.; Hayashi, H.; Shirabe, S.; Taniyama, K.; Eguchi, K. ACZ acts directly on the human skeletal muscle chloride channel. Muscle Nerve 2006, 34, 292–297. [Google Scholar] [CrossRef]
  254. Maggi, L.; Bernasconi, P.; D’Amico, A.; Brugnoni, R.; Fiorillo, C.; Garibaldi, M.; Astrea, G.; Bruno, C.; Santorelli, F.M.; Liguori, R.; et al. Italian recommendations for diagnosis and management of congenital myasthenic syndromes. Neurol. Sci. 2019, 40, 457–468. [Google Scholar] [CrossRef] [PubMed]
  255. Engel, A.G.; Shen, X.M.; Selcen, D.; Sine, S.M. Congenital myasthenic syndromes: Pathogenesis, diagnosis, and treatment. Lancet. Neurol. 2015, 14, 420–434, Erratum in: Lancet Neurol. 2015, 14, 461. [Google Scholar] [CrossRef] [Green Version]
  256. Finlayson, S.; Beeson, D.; Palace, J. Congenital myasthenic syndromes: An update. Pract. Neurol. 2013, 13, 80–91. [Google Scholar] [CrossRef]
  257. Abicht, A.; Dusl, M.; Gallenmüller, C.; Guergueltcheva, V.; Schara, U.; Della Marina, A.; Wibbeler, E.; Almaras, S.; Mihaylova, V.; von der Hagen, M.; et al. Congenital myasthenic syndromes: Achievements and limitations of phenotype-guided gene-after-gene sequencing in diagnostic practice: A study of 680 patients. Hum. Mutat. 2012, 33, 1474–1484. [Google Scholar] [CrossRef] [PubMed]
  258. Hoffmann, K.; Müller, J.S.; Stricker, S.; Megarbane, A.; Rajab, A.; Lindner, T.H.; Cohen, M.; Chouery, E.; Adaimy, L.; Ghanem, I.; et al. Escobar syndrome is a prenatal myasthenia caused by disruption of the acetylcholine receptor fetal gamma subunit. Am. J. Hum. Genet. 2006, 79, 303–312. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  259. Vogt, J.; Harrison, B.J.; Spearman, H.; Cossins, J.; Vermeer, S.; ten Cate, L.N. Mutation analysis of CHRNA1, CHRNB1, CHRND, and RAPSN genes in multiple pterygium syndrome/fetal akinesia patients. Am. J. Hum. Genet. 2008, 82, 222–227. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  260. Michalk, A.; Stricker, S.; Becker, J.; Rupps, R.; Pantzar, T.; Miertus, J.; Botta, G.; Naretto, V.G.; Janetzki, C.; Yaqoob, N.; et al. Acetylcholine receptor pathway mutations explain various fetal akinesia deformation sequence disorders. Am. J. Hum. Genet. 2008, 82, 464–476. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  261. Santovito, L.S.; Brugnoni, R.; Banfi, P.; Maggi, L. Salbutamol as effective treatment in slow-channel syndrome—first report. Neurol. Sci. 2021, 42, 1611–1612. [Google Scholar] [CrossRef]
  262. Nigro, V.; Savarese, M. Next-generation sequencing approaches for the diagnosis of skeletal muscle disorders. Curr. Opin. Neurol. 2016, 29, 621–627. [Google Scholar] [CrossRef] [PubMed]
  263. Ferradini, V.; Cassone, M.; Nuovo, S.; Bagni, I.; D’Apice, M.R.; Botta, A.; Novelli, G.; Sangiuolo, F. Targeted Next Generation Sequencing in patients with Myotonia Congenita. Clin. Chim. Acta 2017, 470, 1–7. [Google Scholar] [CrossRef] [PubMed]
  264. Vivekanandam, V.; Männikkö, R.; Matthews, E.; Hanna, M.G. Improving genetic diagnostics of skeletal muscle channelopathies. Expert. Rev. Mol. Diagn. 2020, 20, 725–736. [Google Scholar] [CrossRef] [PubMed]
  265. Yeh, H.M.; Liao, M.H.; Chu, C.L.; Lin, Y.H.; Sun, W.Z.; Lai, L.P.; Chen, P.L. Next-generation sequencing and bioinformatics to identify genetic causes of malignant hyperthermia. J. Formos. Med. Assoc. 2021, 120, 883–892. [Google Scholar] [CrossRef] [PubMed]
  266. Morales, F.; Pusch, M. An Up-to-Date Overview of the Complexity of Genotype-Phenotype Relationships in Myotonic Channelopathies. Front. Neurol. 2020, 10, 1404. [Google Scholar] [CrossRef] [PubMed]
  267. Maggi, L.; Ravaglia, S.; Farinato, A.; Brugnoni, R.; Altamura, C.; Imbrici, P.; Camerino, D.C.; Padovani, A.; Mantegazza, R.; Bernasconi, P.; et al. Coexistence of CLCN1 and SCN4A mutations in one family suffering from myotonia. Neurogenetics 2017, 18, 219–225. [Google Scholar] [CrossRef]
  268. Thor, M.G.; Vivekanandam, V.; Sampedro-Castañeda, M.; Tan, S.V.; Suetterlin, K.; Sud, R.; Durran, S.; Schorge, S.; Kullmann, D.M.; Hanna, M.G.; et al. Myotonia in a patient with a mutation in an S4 arginine residue associated with hypokalaemic periodic paralysis and a concomitant synonymous CLCN1 mutation. Sci. Rep. 2019, 9, 17560. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  269. Brenes, O.; Barbieri, R.; Vásquez, M.; Vindas-Smith, R.; Roig, J.; Romero, A.; Valle, G.D.; Bermúdez-Guzmán, L.; Bertelli, S.; Pusch, M.; et al. Functional and Structural Characterization of ClC-1 and Nav1.4 Channels Resulting from CLCN1 and SCN4A Mutations Identified Alone and Coexisting in Myotonic Patients. Cells 2021, 10, 374. [Google Scholar] [CrossRef] [PubMed]
  270. Mall, M.A.; Mayer-Hamblett, N.; Rowe, S.M. Cystic Fibrosis: Emergence of Highly Effective Targeted Therapeutics and Potential Clinical Implications. Am. J. Respir. Crit. Care Med. 2020, 201, 1193–1208. [Google Scholar] [CrossRef]
Cells 10 01521 g001 550
Figure 1. A schematic representation of skeletal muscle sodium channelopathies, reporting the mode of inheritance (AD: autosomal dominant; AR: autosomal recessive), disease name, mutation effects on sodium channel function, and main symptoms.
Figure 1. A schematic representation of skeletal muscle sodium channelopathies, reporting the mode of inheritance (AD: autosomal dominant; AR: autosomal recessive), disease name, mutation effects on sodium channel function, and main symptoms.
Cells 10 01521 g001
Cells 10 01521 g002 550
Figure 2. A schematic representation of the calcium ion-permeable channels involved in skeletal muscle myopathies. The TRPV4 channel is highly expressed even in motor neurons, and mutations cause a number of peripheral neuropathies with implications for skeletal muscles. The contribution of muscular TRPV4 channels to these diseases is unknown. The Cav3.2 channel is expressed mainly in embryonic cells, which contributes to myoblast differentiation and fusion during muscle development. (CRAC: Calcium-release activated calcium; DHPR: Dihydropyridine receptor; GoF: gain of function; HMSN2C: Hereditary motor and sensory neuropathy type 2C; HypoPP1: Hypokalemic periodic paralysis type 1; LoF: loss of function; MHS: Malignant hyperthermia susceptibility; NAM: Native American myopathy; NEM3: Nemaline myopathy type 3; SMA: Spinal muscular atrophy; SPSMA: Scapuloperoneal spinal muscular atrophy; SR: sarcoplasmic reticulum; STRMK: Stormorken syndrome; TAM: Tubular aggregate myopathy).
Figure 2. A schematic representation of the calcium ion-permeable channels involved in skeletal muscle myopathies. The TRPV4 channel is highly expressed even in motor neurons, and mutations cause a number of peripheral neuropathies with implications for skeletal muscles. The contribution of muscular TRPV4 channels to these diseases is unknown. The Cav3.2 channel is expressed mainly in embryonic cells, which contributes to myoblast differentiation and fusion during muscle development. (CRAC: Calcium-release activated calcium; DHPR: Dihydropyridine receptor; GoF: gain of function; HMSN2C: Hereditary motor and sensory neuropathy type 2C; HypoPP1: Hypokalemic periodic paralysis type 1; LoF: loss of function; MHS: Malignant hyperthermia susceptibility; NAM: Native American myopathy; NEM3: Nemaline myopathy type 3; SMA: Spinal muscular atrophy; SPSMA: Scapuloperoneal spinal muscular atrophy; SR: sarcoplasmic reticulum; STRMK: Stormorken syndrome; TAM: Tubular aggregate myopathy).
Cells 10 01521 g002
Cells 10 01521 g003 550
Figure 3. A schematic representation of the potassium channels involved in skeletal muscle myopathies. Potassium channel subunits are represented in lateral view embedded in the membrane, while multimeric assemblies are represented from the top view. The inward-rectifier K+ channels are heterotetrameric assemblies of Kir subunits. The ATP-sensitive K+ channels are made by the octameric association of four Kir6.x subunits with four sulfonylurea receptors (SUR) containing nucleotide-binding domains (NBD). The voltage-dependent K+ channel Kv1.1 is expressed in neurons, but a number of EA1 patients may present with predominant muscular phenotypes. The pathogenicity of the K+ channel auxiliary subunit MirP2 in hypoPP is still debated.
Figure 3. A schematic representation of the potassium channels involved in skeletal muscle myopathies. Potassium channel subunits are represented in lateral view embedded in the membrane, while multimeric assemblies are represented from the top view. The inward-rectifier K+ channels are heterotetrameric assemblies of Kir subunits. The ATP-sensitive K+ channels are made by the octameric association of four Kir6.x subunits with four sulfonylurea receptors (SUR) containing nucleotide-binding domains (NBD). The voltage-dependent K+ channel Kv1.1 is expressed in neurons, but a number of EA1 patients may present with predominant muscular phenotypes. The pathogenicity of the K+ channel auxiliary subunit MirP2 in hypoPP is still debated.
Cells 10 01521 g003
Cells 10 01521 g004 550
Figure 4. Pathomechanisms of CLCN1-related myotonia congenita (MC). (A) Presumed mechanism of inheritance in MC. The ClC-1 channel is a dimeric protein with a double barrel-like structure: two subunits assemble to form two parallel ion-conducting pores. In the case of heterozygosity, wild-type (WT) and mutated (MUT) ClC-1 subunits can assemble as homodimers, WT–WT and MUT–MUT, and heterodimers (WT–MUT). In autosomal dominant Thomsen’s disease, the mutated subunit is expected to exert a dominant-negative effect (*) on the associated wild-type subunit in the WT–MUT channel. This results in the reduction of sarcolemma chloride conductance (gCl) by more than 50%, leading to muscle fiber hyperexcitability and muscle stiffness. In autosomal recessive Becker’s disease, the recessive mutation is expected to have no effect on the associated WT subunit. The co-expression of the recessive mutation with the wild-type ClC-1 results at maximum in a 50% reduction of the sarcolemmal chloride conductance, which is not enough to cause myotonia. The occurrence of recessive mutations in homozygosity or in compound heterozygosity is required to reduce the sarcolemmal chloride conductance by more than 50% and to induce myotonia. (+: functional ClC-1 subunit, -: impaired ClC-1 subunit). (B). The main molecular defects of ClC-1 mutants associated with MC consist of either a defect in ClC-1 proteostasis (protein synthesis, cell trafficking, or proteolysis) or a defect in ClC-1 channel gating. Knowledge of molecular pathomechanism may guide the development of efficient mutant-targeted pharmacological treatments to restore ClC-1 function.
Figure 4. Pathomechanisms of CLCN1-related myotonia congenita (MC). (A) Presumed mechanism of inheritance in MC. The ClC-1 channel is a dimeric protein with a double barrel-like structure: two subunits assemble to form two parallel ion-conducting pores. In the case of heterozygosity, wild-type (WT) and mutated (MUT) ClC-1 subunits can assemble as homodimers, WT–WT and MUT–MUT, and heterodimers (WT–MUT). In autosomal dominant Thomsen’s disease, the mutated subunit is expected to exert a dominant-negative effect (*) on the associated wild-type subunit in the WT–MUT channel. This results in the reduction of sarcolemma chloride conductance (gCl) by more than 50%, leading to muscle fiber hyperexcitability and muscle stiffness. In autosomal recessive Becker’s disease, the recessive mutation is expected to have no effect on the associated WT subunit. The co-expression of the recessive mutation with the wild-type ClC-1 results at maximum in a 50% reduction of the sarcolemmal chloride conductance, which is not enough to cause myotonia. The occurrence of recessive mutations in homozygosity or in compound heterozygosity is required to reduce the sarcolemmal chloride conductance by more than 50% and to induce myotonia. (+: functional ClC-1 subunit, -: impaired ClC-1 subunit). (B). The main molecular defects of ClC-1 mutants associated with MC consist of either a defect in ClC-1 proteostasis (protein synthesis, cell trafficking, or proteolysis) or a defect in ClC-1 channel gating. Knowledge of molecular pathomechanism may guide the development of efficient mutant-targeted pharmacological treatments to restore ClC-1 function.
Cells 10 01521 g004
Table
Table 1. Ion channels gene mutations and related clinical muscular phenotypes.
Table 1. Ion channels gene mutations and related clinical muscular phenotypes.
ProteinGeneInheritanceClinical PhenotypePhenotype MIMAge at OnsetMuscle BiopsySpecific FeaturesTreatment
SODIUM CHANNEL SUBUNITS
Nav1.4SCN4AADSodium channel myotonia (SCM; includes potassium-aggravated myotonia, myotonia fluctuans, myotonia permanens, ACZ-responsive myotonia, and SNEL)608,390Highly variable (neonatal–early childhood–adulthood)non-specific myopathic patternPredominance in cranial muscles, precipitated by cold, presence of warm-up, muscle weakness absent or mild with late-onsetMexiletine, lamotrigine, carbamazepine, ACZ, flecainide, and propafenone
ADParamyotonia congenita (PMC)168,300First decadenon-specific myopathic patternMyotonia and episodic muscle weakness precipitated by cold, paradoxical myotonia, predominant in cranial muscles, possible fixed muscle weakness in late disease stages.As for SCM
ADHyperkalemic periodic paralysis (hyperPP)170,500First decadeVacuolar and tubular aggregate myopathyEpisodic flaccid muscle weakness lasting up to 2 h accompanied by hyperkalemia > 4.5 mEq/L.
Associated with myotonia.		ACZ, diclorophenamide
ADHypokalemic periodic paralysis type 2 (hypoPP2)613,345Childhood–third decade Vacuolar and tubular aggregate myopathyEpisodic flaccid muscle weakness lasting up to 24 h accompanied by hypokalemia < 3.5 mEq/L.ACZ, K+ sparing diuretics (spironolactone, triamterene)
ARCongenital myasthenic syndrome type 16 (CMS16)614,198Neonatal or early infancynon-specific myopathic patternDecremental response of the CMAP on RNS.
Predominant involvement of bulbar and respiratory muscles.		Pyridostigmine and ACZ may be beneficial
ARCongenital myopathyn.a.Neonatal or early infancyNo evident nemaline rods or structural abnormalitiesPredominant axial and pelvic muscle weakness, delayed motor milestones, improvement in strength over timeACZ
CALCIUM CHANNEL SUBUNITS
Cav1.1CACNA1SADHypokalemic periodic paralysis type 1 (hypoPP1)170,400Childhood–second decadeVacuolar myopathy (non-rimmed)Episodic flaccid muscle weakness lasting up to 24 h accompanied by hypokalemia < 3.5 mEq/L. Fixed myopathy often developing in late disease stages.ACZ, diclorphenamide
ADMalignant hyperthermia susceptibility type 5 (MHS5)601,887When exposed to volatile anesthetics or succinylcholineNo structural abnormalitiesMHSDantrolene (antidote)
ARCongenital myopathyn.a.Neonatal or early infancyCentronuclear or core myopathyHypotonia, delayed motor milestones, facial involvement (ophthalmoplegia), progressive muscle weakness (mainly axial).ACZ
Stac3STAC3ARBailey-Bloch congenital myopathy/Native American Myopathy (NAM)255,995Neonatal or early infancynon-specific myopathic patternDysmorphic facial features and facial weakness (ptosis) susceptibility to MHS; multiple joint contracturesn.a.
Orai 1ORAI1ADTubular aggregate myopathy (TAM2)615,883Childhoodtubular aggregates in type II fibers, predominance of type I fibersSlowly progressiven.a
ARCRAC channelopathies612,782<1 year(1 patient) myopathic pattern; no evident nemaline rods or structural abnormalities.Congenital non-progressive myopathy; immunodeficiency as the main feature.n.a.
Stim 1STIM1ADStormorken syndrome (STRMK), York platelet syndrome185,070Childhood–early adulttubular aggregates in type II fibers, predominance of type I fibersThrombocytopenia, anemia, asplenia, congenital miosis, and ichthyosis, asymptomatic to slowly progressive proximal muscle weaknessn.a.
ADNon-syndromic tubular aggregate myopathy (TAM1)160,565Childhoodtubular aggregates mainly in type II fibers; predominance type I fibersSlowly progressive, elevated CPKn.a.
ARCRAC channelopathies612,783<1 yearn.a.Congenital non-progressive myopathy; immunodeficiency as the main feature.n.a.
Ryr1RYR1ADMalignant hyperthermia susceptibility type 1 (MHS1)145,600When exposed to volatile anesthetics or depolarizing muscle relaxantsCentral core, multiminicore myopathyMHSDantrolene (antidote)
AD/ARCentral core disease117,000First decade, rarely in adulthoodCentral cores in type 1 fibers, predominance of type 1 fibers Floppy infant; non-progressive/slowly progressive myopathy; joint contracturesn.a
ARMultiminicore myopathy with external ophthalmoplegia255,320Neonatal or early infancyDystrophic signs and minicoresHypotonia, delayed motor milestones, dysmorphic facial features and facial weakness, and progressive muscle weaknessn.a
Ryr3RYR3ARNemaline myopathy (NEM3)161,8001 case, infantilePerinuclear and subsarcolemmal nemaline bodies, wide variation in fiber size with type 1 fiber predominance and atrophy, increased internal nucleiDysmorphic face; normal CPK; myopathic EMG. Slowly progressive proximal limb weaknessn.a.
TRPV4TRPV4AD
(reduced penetrance)		scapuloperoneal spinal muscular atrophy (SPSMA)181,405Neonatal or early infancyGrouped type 1 and 2 fiber atrophyNon-progressive or slowly progressive scapular and peroneal muscle weakness and atrophy, and peripheral motor neuropathyn.a.
AD
(reduced penetrance)		congenital distal spinal muscular atrophy (CDSMA)600,175Neonatal or early infancyneurogenic muscle damageVariable from lower-limb muscle weakness to severe neurogenic weakness and arthrogryposisn.a.
ADHereditary motor ans sensory neuropathy (HMSN2C)606,071Variable (infancy, childhood, adulthood)Neurogenic muscle damage and atrophyAxonal polyneuropathy, diaphragmatic and vocal cord paresis, and distal muscle weaknessn.a.
Cav3.2CACNA1HARCongenital amyotrophy 1 case, neonataln.a.Severe amyotrophy at birthn.a.
POTASSIUM CHANNEL SUBUNITS
Kir2.1KCNJ2ADAndersen–Tawil syndrome type 1
(ATS1, LQT7)		170,390Variable onset of periodic paralysis (early childhood-adulthood)non-specific myopathic pattern (few cases)Potassium-sensitive periodic paralysis, cardiac arrhythmia, and facial and skeletal malformations. Prolonged QT (plus other arrhythmias). Episodic flaccid paralysis lasting up to 24h and more, usually accompanied by hypokalemia. ACZ, dichlorphenamide,
ß-blockers,
If hypokaliemic, K+ supplementation or K+ sparing diuretics. If hyperkaliemic, be careful with K+ wasting diuretics for cardiac risk.
Kir3.4KCNJ5ADAndersen–Tawil syndrome type 2 (ATS2, LQT13)613,785Variable onset of periodic paralysis as for ATS1n.a.Same triad of symptoms of ATS1As for ATS1
Kir2.6KCNJ18ADSusceptibility to thyrotoxic periodic paralysis type 2 (TTPP2)613,239Early adulthoodVariable, vacuolation, mitochondrial changes, glycogen granules accumulation.Episodic flaccid paralysis during thyrotoxicosis and hypokalemia. More frequent in Asian males.Treatment of hyperthyroidism
Sur2ABCC9ARIntellectual disability myopathy syndrome (IDMS)n.a.Variable onset of muscle symptoms (childhood-adulthood)(1 patient) non-specific changes (mitochondrial aggregation, fiber caliber variation)Hypotonia, muscle weakness and fatigability, dysmorphic features, intellectual disability and developmental delay, and cardiac systolic dysfunctionn.a.
Kv1.1KCNA1ADEpisodic ataxia/myokymia syndrome (EA1)160,120Childhoodnon-specific, denervation findingsMuscle symptoms (preponderant in a few patients): constant myokymia and acute episodes of muscle contractions (face and limbs), stiffness, cramps, weakness, and episodic cerebellar ataxia, seizures, and hypomagnesemia.ACZ antiepileptic drugs
CHLORIDE CHANNEL SUBUNITS
ClC-1CLCN1ADMyotonia congenita, Thomsen’s disease160,800First decadeNo structural abnormalitiesMyotonia with the warm-up phenomenon, cold sensitivity, predominant in limb muscles.Mexiletine lamotrigine, carbamazepine, ACZ
ARRecessive generalized myotonia, Becker’s disease255,700First decadeNo structural abnormalitiesMore severe than Thomsen’s disease; transient weakness and “Herculean” appearanceAs for Thomsen’s disease
NICOTINIC RECEPTOR
AChRCHRNEARCongenital myasthenic syndrome (CMS4C) associated with AChR deficiency608,931Variable, infancy–adulthoodnon-specificVariable, from arthrogryposis multiplex congenital and fetal akinesia, ocular, bulbar and respiratory symptoms, delayed motor milestones, to mild adult muscle weakness.
Slowly progressive with possible exacerbations.
Decremental CMAP in response to RNS-EMG.		Pyridostigmine,
3,4 diaminopyridine, salbutamol/albuterol, and ephedrine
AD/AR (rare)Slow-channel CMS (CMS4A)605,809Infancy–young adultnon-specificNeonatal hypotonia; ocular, bulbar, respiratory muscle involvement, with predominant weakness of cervical, wrist, finger, and finger extensor muscles. Double CMAP on single nerve stimuli ENG.Quinidine, fluoxetine,
Worsening with pyridostigmine
ARFast-channel CMS (CMS4B)616,324Infancynon-specificNeonatal hypotonia, recurrent respiratory crises. Ocular, neck, and limb progressive muscle weakness and fatigability. Decremental CMAP in response to RNS-EMG.Pyridostigmine,
3,4 diaminopyridine
CHRNA1ADSlow-channel CMS (CMS1A)601,462Infancy–young adultnon-specificOcular, bulbar, and respiratory muscle involvement, with predominant weakness of cervical, wrist, finger, and finger extensor muscles. Double CMAP on single nerve stimuli ENG.Quinidine, fluoxetine,
Worsening with pyridostigmine
AD (rare)/ARFast-channel CMS (CMS1B)608,930Infancynon-specificNeonatal hypotonia; ocular, bulbar (dysarthria), neck, recurrent respiratory crises, and limb progressive muscle weakness and fatigability. Decremental CMAP in response to RNS-EMG.Pyridostigmine,
3,4 diaminopyridine
CHRNB1ARCMS2C associated with AChR deficiency616,314Birthnon-specificNeonatal hypotonia; respiratory and limb progressive muscle weakness.
Decremental CMAP in response to RNS-EMG		Pyridostigmine
ADSlow-channel CMS2A616,313Infancy–young adultnon-specificOcular, bulbar, respiratory muscle involvement, with predominant weakness of cervical, wrist, finger, and finger extensor muscles. Double CMAP on single nerve stimuli ENG.Quinidine, fluoxetine,
Worsening with pyridostigmine
CHRNDADSlow-channel CMS3A616,321Infancy—young adultnon-specificOcular, bulbar, respiratory muscle involvement, with predominant weakness of cervical, wrist, finger, and finger extensor muscles. Double CMAP on single nerve stimuli ENGQuinidine, fluoxetine,
Worsening with pyridostigmine
ARCMS3C associated with AChR deficiency616,323Birthnon-specificNeonatal hypotonia; ocular, episodic respiratory insufficiency, bulbar (swallowing), and proximal limb muscle weakness. Decremental CMAP in response to RNS-EMG.Pyridostigmine
ARFast-channel CMS3B616,322Infancynon-specificNeonatal hypotonia; ocular, neck, respiratory, muscle weakness and fatigability. Decremental CMAP in response to RNS-EMG.Pyridostigmine,
3,4-diaminopyridine
References are given in the text. Abbreviations: ACZ: Acetazolamide; CMAP: Compound Muscle Action Potential; CPK: creatine phosphate kinase; n.a.: not available; RNS-EMG: Repetitive nerve stimulation electromyography.
Publisher’s Note: MDPI stays neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Share and Cite

MDPI and ACS Style

Maggi, L.; Bonanno, S.; Altamura, C.; Desaphy, J.-F. Ion Channel Gene Mutations Causing Skeletal Muscle Disorders: Pathomechanisms and Opportunities for Therapy. Cells 2021, 10, 1521. https://doi.org/10.3390/cells10061521

AMA Style

Maggi L, Bonanno S, Altamura C, Desaphy J-F. Ion Channel Gene Mutations Causing Skeletal Muscle Disorders: Pathomechanisms and Opportunities for Therapy. Cells. 2021; 10(6):1521. https://doi.org/10.3390/cells10061521

Chicago/Turabian Style

Maggi, Lorenzo, Silvia Bonanno, Concetta Altamura, and Jean-François Desaphy. 2021. "Ion Channel Gene Mutations Causing Skeletal Muscle Disorders: Pathomechanisms and Opportunities for Therapy" Cells 10, no. 6: 1521. https://doi.org/10.3390/cells10061521

APA Style

Maggi, L., Bonanno, S., Altamura, C., & Desaphy, J. -F. (2021). Ion Channel Gene Mutations Causing Skeletal Muscle Disorders: Pathomechanisms and Opportunities for Therapy. Cells, 10(6), 1521. https://doi.org/10.3390/cells10061521

Note that from the first issue of 2016, this journal uses article numbers instead of page numbers. See further details here.

Article Metrics

Back to TopTop