Next Article in Journal
Risk of Cardiovascular Events in Adults Aged 40 to 79 Years with Diagnosed Hypertension, High Cholesterol, and/or Diabetes but Not on Medications: Findings from Nationwide Cross-Sectional Studies
Next Article in Special Issue
Direct Cardiac Reprogramming in the Age of Computational Biology
Previous Article in Journal
Hypertension-Mediated Organ Damage in Relation to Severity of Chronic Low Back Pain in Hypertensive Patients
Previous Article in Special Issue
The Functional Significance of Cardiac Looping: Comparative Embryology, Anatomy, and Physiology of the Looped Design of Vertebrate Hearts
 
 
Search for Articles:
Title / Keyword
Author / Affiliation / Email
Journal
Article Type
 
 
Advanced Search
 
Section
Special Issue
Volume
Issue
Number
Page
 
Journals
JCDD
Volume 11
Issue 9
10.3390/jcdd11090267
jcdd-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

Developmental Changes in the Excitation–Contraction Mechanisms of the Ventricular Myocardium and Their Sympathetic Regulation in Small Experimental Animals

by
Shogo Hamaguchi
,
Naoki Agata
,
Maika Seki
,
Iyuki Namekata
and
Hikaru Tanaka
*
Department of Pharmacology, Faculty of Pharmaceutical Sciences, Toho University, Funabashi 274-8510, Japan
*
Author to whom correspondence should be addressed.
J. Cardiovasc. Dev. Dis. 2024, 11(9), 267; https://doi.org/10.3390/jcdd11090267
Submission received: 15 May 2024 / Revised: 2 August 2024 / Accepted: 11 August 2024 / Published: 29 August 2024
(This article belongs to the Special Issue 10th Anniversary of JCDD—'Cardiac Development and Regeneration' Section — from Development to Regeneration)
Browse Figures
Versions Notes

Abstract

:
The developmental changes in the excitation–contraction mechanisms of the ventricular myocardium of small animals (guinea pig, rat, mouse) and their sympathetic regulation will be summarized. The action potential duration monotonically decreases during pre- and postnatal development in the rat and mouse, while in the guinea pig it decreases during the fetal stage but turns into an increase just before birth. Such changes can be attributed to changes in the repolarizing potassium currents. The T-tubule and the sarcoplasmic reticulum are scarcely present in the fetal cardiomyocyte, but increase during postnatal development. This causes a developmental shift in the Ca2+ handling from a sarcolemma-dependent mechanism to a sarcoplasmic reticulum-dependent mechanism. The sensitivity for beta-adrenoceptor-mediated positive inotropy decreases during early postnatal development, which parallels the increase in sympathetic nerve innervation. The alpha-adrenoceptor-mediated inotropy in the mouse changes from positive in the neonate to negative in the adult. This can be explained by the change in the excitation–contraction mechanism mentioned above. The shortening of the action potential duration enhances trans-sarcolemmal Ca2+ extrusion by the Na+-Ca2+ exchanger. The sarcoplasmic reticulum-dependent mechanism of contraction in the adult allows Na+-Ca2+ exchanger activity to cause negative inotropy, a mechanism not observed in neonatal myocardium. Such developmental studies would provide clues towards a more comprehensive understanding of cardiac function.

1. Introduction

Small experimental animals are indispensable for the studies of the basic mechanisms of the heart and the creation of novel therapeutic agents. They are easy to handle, and their small body weight is of advantage for the in vivo screening of medicinal seeds. The hearts of small animals in general are known to have relatively high heart rates. Their myocardial contraction shares basic mechanisms such as the action potential and the Ca2+ transient, but difference exists in the process of repolarization and dependence on sarcoplasmic reticulum. The heart of the mouse is probably in the most extreme position among commonly used mammalian experimental animal species. The guinea pig heart has properties relatively close to those of larger animals and humans. The rat heart appears to have properties intermediate between the guinea pig and mouse. Such differences between animal species are small in the fetal stage and gradually appear during pre- and postnatal development. Understanding the similarities and difference among experimental animal species and developmental stages would provide insights into the factors involved in myocardial function. In this review, we will summarize the developmental changes in the myocardial excitation–contraction mechanisms and their sympathetic regulation, focusing on the ventricular myocardium of the guinea pig, rat, and mouse.

2. Action Potential Configuration and Membrane Currents in the Adult

Animals of smaller size generally have higher heart rate and higher metabolic rate compared with larger animals and humans. The order among small experimental animals is mouse > rat > guinea pig [1,2,3,4,5,6,7,8]. While the maximum beating rate of the rat and mouse is as fast as 500 beats/minute and 800 beats/minute, respectively, the guinea pig heart has a beating rate of about 300 bpm, which is relatively close to larger animals and humans. The action potential of the guinea pig ventricular myocardium has an obvious plateau phase resembling those of larger animals (Figure 1(Ac)); the action potential duration is 200 to 300 ms. The plateau phase plays important roles in myocardial contraction, such as the trans-sarcolemmal influx of Ca2+ to trigger contraction and the formation of the refractory period to prevent arrhythmic excitation of the myocardium. Action potential duration is mainly determined by the balance between the L-type Ca2+ current (ICa) and repolarizing potassium currents. Voltage clamp analyses of ventricular cardiomyocytes revealed that the ICa is relatively similar among experimental animal species in terms of current density and kinetics [5]. On the other hand, there is a large species difference in repolarizing outward currents [9]. The major repolarizing current in the dog, rabbit, and guinea pig is the delayed rectifier potassium current (IK), which requires a few hundred milliseconds for maximum activation [10,11,12,13]; this delay causes a delay until the start of the repolarization and results in the typical action potential duration. Thus, the guinea pig has repolarization properties relatively similar to larger animals and humans, and is widely used in physiological and pharmacological studies oriented towards application in humans.
The mouse and rat heart, which beats faster than the guinea pig, as mentioned above, shows rapid contraction and relaxation. Thus, the myocardium of these animal species should have characteristic excitation–contraction mechanisms to support its rapid contraction and relaxation. The mouse and rat ventricular myocardium have an action potential with a very short duration at depolarized membrane potentials and a late slowly repolarizing phase. The mouse ventricular action potential is very short, with an action potential duration at 50% repolarization of 3 to 5 ms (Figure 1(Bc)) [14,15,16,17,18,19,20,21,22]. Although very different from the human myocardium, the use of genetically modified mice enables exploration at the molecular level. Also, the dramatic change during development makes them suitable for studies such as the relation between action potential and inotropy (Table 1).
The repolarizing current in the mouse and rat is the transient outward current (Ito), which activates and inactivates much faster than IK. The Ito is composed of voltage-dependent K+ channel current and the Ca2+-activated Cl− current [38]. The Ito in the ventricular myocytes of the mouse and rat has a high current density, which leads to rapid repolarization following the initial upstroke of the action potential. Following the rapid repolarization, a slow repolarizing phase, which is also referred to as the late plateau phase, is present in the mouse and rat ventricular myocardium. This phase is considered to reflect the inward current on the extrusion of Ca2+ by the sodium–calcium exchanger (NCX). The major role of NCX is the trans-sarcolemmal extrusion of Ca2+. NCX transports one Ca2+ ion in exchange for three Na+ ions, so the extrusion of intracellular Ca2+ results in the generation of an inward current that may cause membrane depolarization. In the case of the mouse and rat ventricle, this process occurs just after the rapid repolarization by Ito to form the late plateau. In fact, the late plateau phase is abolished by ryanodine, which inhibits Ca2+ release from the sarcoplasmic reticulum (SR) and is not observed in cells internally dialyzed with EGTA-containing solution [39]. Further, SEA0400, a highly selective inhibitor of myocardial NCX [40,41], as well as a low-Na+ extracellular solution, largely reduced the late plateau [18].
The action potential plateau at depolarized membrane potentials has functional roles in myocardial excitation, and the mouse and rat ventricular myocardium lacking this phase appear to have compensatory mechanisms. Firstly, a longer plateau results in a larger volume of depolarized myocardium at the excitation wavefront, which electrotonically supports forward propagation of the action potential. Shorter action potential duration of the mouse and rat action potential means less electrotonic support from behind at the excitation wavefront. We have observed that the maximum rate of rise of the mouse ventricular action potential is significantly larger than that of other species [17], which may indicate larger sodium current density in the mouse ventricular myocyte. A larger depolarizing current at the excitation wavefront would provide larger depolarizing power and might compensate for less electrotonic support from behind in this species. Secondly, Ca2+ entering the cell through the L-type Ca2+ channel during the plateau phase activates the contractile proteins and elicits myocardial contraction either directly or through triggering of SR Ca2+ release. The short action potential of the mouse and rat allows less Ca2+ to enter the cell. This appears to be compensated by elevated SR function, as described in the next section. Thirdly, action potential duration parallels the length of the refractory period, which prevents the myocardium from premature firing in response to arrhythmogenic stimuli from ectopic foci or re-entry circuits. The short action potential duration, and thus a short refractory period of the mouse ventricular myocardium, means that it is susceptible to arrhythmogenic stimuli. We notice that isolated mouse myocardial tissue preparations tend to show arrhythmic contractions when driven at low frequencies in vitro. However, this susceptibility to arrhythmogenic stimuli can probably be masked in the in vivo mouse heart by its high beating rate.

3. Developmental Changes in the Action Potential

The maximum rate of rise of the mouse ventricle gradually increases during pre- and postnatal development [19], which correlates with an increase in the expression of voltage-dependent Na+ channels [28,29]. While the adult ventricular myocardium of the mouse and rat has characteristic action potentials of short duration, the fetal and neonatal myocardium of these species have an action potential with a longer duration: developmental shortening is observed during pre- and postnatal development. We reported that the action potential duration of the mouse ventricular myocardium is longer than 70 milliseconds at fetal day 16, about 15 milliseconds in the neonate, and shortens to a few milliseconds in the adult [19] (Figure 1B). Similar results have been repeatedly reported in ventricular myocardium from pre- and postnatal mice [15,16,19,20]. The major cause of this shortening is the developmental increase in repolarizing potassium currents. The neonatal mouse ventricular myocytes have a much lower current density of the Ito than the adult. Instead, the IK is present, resulting in a longer action potential duration. A similar developmental shortening of the action potential reflecting an increase in Ito was observed in the pre- and postnatal rat ventricle [21]. Concerning ICa, the current amplitude [30,32], as well as its expression level [28,31] increases during development; the time course of the current appears to be unchanged. Developmental changes in the Ca2+-dependent inactivation of the ICa has not been reported, and experimental evidence for and against the presence of such mechanisms have been reported [42,43,44].
In the guinea pig, shortening of the ventricular action potential is observed during the late-fetal and early-postnatal period [10]. Action potential duration reaches its minimum at around 5 days after birth, and a gradual increase is observed until adulthood (Figure 1A). Voltage-clamp analysis of isolated ventricular myocytes revealed developmental increase in both IK and ICa, but the time course was different. Increase in IK occurred during the late-fetal period, while the increase in ICa occurred postnatally. This could explain the biphasic developmental change in action potential duration in the guinea pig ventricle [11]. The ATP-sensitive potassium channel current was shown to be present in the guinea-pig ventricular myocardium as early as on the 35th day of fetal development [45,46], as confirmed by both shortening of the action potential by the ATP-sensitive potassium channel opener, cromakalim, and by direct measurement of the channel current by voltage clamp experiments. However, experimental hypoxia induced only a slight decrease in contractile force, as well as the action potential duration in the fetus. This was because the fetal myocardium was much less dependent on the oxidative metabolism than the adult, but rather dependent on ATP provided by glycolysis. Electron microscopic images of fetal myocardium have demonstrated the presence of glycogen granules [47]. Confocal microscopy revealed that the mitochondria were less abundant and tended to localize in the cell center, relatively far from the sarcolemma. Thus, the function of ion channels involved in the formation of the action potential is not only one of influencing each other electrically but also being influenced by intracellular metabolic properties.

4. Excitation–Contraction Mechanisms in the Adult

Ventricular myocytes from the adult mammalian heart have a well-developed T-tubular system throughout the cell. During the action potential plateau, Ca2+ influx through the sarcolemma and T-tubules triggers Ca2+ release from ryanodine receptors located on the adjacent SR membrane. This results in a higher Ca2+ concentration at the Z-band region of the ventricular myocyte only for several milliseconds during the early phase of contraction, and at about 10 milliseconds after the onset of action potential, Ca2+ concentration is uniform throughout the whole cytoplasm [48]. In contrast, in atrial cardiomyocytes, which lacks the T-tubular system, trans-sarcolemmal Ca2+ influx triggers Ca2+ release only at the subsarcolemmal SR. This Ca2+ triggers Ca2+ release from the neighboring SR, and a wave of Ca2+-induced Ca2+ release propagates towards the cell interior as a Ca2+ wave [48].
The Ca2+ for the initial triggering of the Ca2+-induced Ca2+ release is provided by the ICa, and the amount correlates with the APD at about 0mV or at 20% repolarization (APD20). In a voltage-clamped rat ventricular cardiomyocyte, the total Ca2+ influx elicited by an action potential with a duration at 0mV of 44 ms and 6 ms was 33 and 16 pC, respectively [49]. Under an action potential of short duration, the peak amplitude of the Ca2+ influx is large, due to the larger inward driving force, but the Ca2+ channel rapidly deactivates, resulting in less total Ca2+ influx. In the mouse ventricular myocardium, the action potential duration at 20% depolarization decreases during development from about 45 ms in the fetus to less than 3ms in the adult, indicating a decrease in the Ca2+ to trigger contraction [19]. The adult mouse ventricular myocardium probably compensates for this by its elevated SR function. When the effects of nicardipine and ryanodine on isolated myocardial tissue from mouse, rat, and guinea pig were compared to evaluate the relative role of trans-sarcolemmal Ca2+ influx and SR Ca2+ release, the potency order for negative inotropy nicardipine, which reflects dependence on trans-sarcolemmal Ca2+ entry, was guinea pig > rat > mouse [19,50,51]. This correlated with the species difference in action potential duration. On the other hand, the potency order for the negative inotropy by ryanodine, which reflects dependence on SR Ca2+ release, was mouse > rat > guinea pig.
Hearts with higher beating rate require faster contraction and relaxation for sufficient refilling before the subsequent heartbeat. The rate of ventricular relaxation measured under the same conditions in our laboratory was in the order of mouse > rat > guinea pig [19,50,51], which was the same as the order of higher heart rate and lower heart weight. This could be accomplished by increasing Ca2+ release and uptake by the SR. Comparative studies with various mammals revealed hearts of smaller weight have a higher resting heart rate and higher SR Ca2+. The mouse heart, which had the smallest weight, had the highest beating rate and SR Ca2+ ATPase activity [3]. The potency of the negative inotropy of cyclopiazonic acid, which impairs SR function through inhibition of Ca2+ uptake into the SR by the Ca2+ ATPase, was also in the order of mouse > rat > guinea pig.

5. Developmental Changes in Excitation–Contraction Mechanisms

The developing cardiomyocyte is not only smaller in size than the adult cardiomyocyte, but is also structurally very different. At the early stage of development, the t-tubules are very sparse and were present at the subsarcolemmal region mainly in a longitudinal orientation [52,53,54,55]. A progressive invagination of the t-tubules from the surface sarcolemma and alignment into a more transverse orientation takes place during postnatal development of the ventricular myocardium. The development of the t-tubular system is regulated by several key proteins including caveolin 3, junctophilin 2, ryanodine receptor, dysferin, bridging integrator-1 and protein phosphatase nonreceptor type 23 [53,56,57,58]. The SR is sparse in the fetus and neonate, and is present in the cell interior [19,50]; it expresses functional ryanodine receptors [59,60] localized to the Z-line prior to t-tubule formation [54,55]. Functional coupling of the t-tubules and the SR Ca2+ release units are formed progressively during postnatal development. In diseased myocardium such as that under heart failure, the integrity of the t-tubules as well as their coupling with the SR is impaired [54,61,62]. Increase in cardiac pre- and afterload has both increasing and decreasing effects on the t-tubular density, which appears to be related to compensatory mechanisms during heart failure [63]. The density of the t-tubular network in the adult tends to be denser in smaller animals than in larger animals [64,65]; among experimental animals, the mouse appears to have the highest t-tubular density. The t-tubular density of the mouse ventricular myocardium is very low in the fetal and neonatal myocardium and increases during the first and second postnatal week. The SR is present in the fetal cardiomyocyte and gradually increases during pre and early postnatal development [19]. These changes in cellular structure (Figure 2) and the concomitant changes in action potential configuration affects the functional properties of the murine myocardium.
Concerning the developmental changes in the mouse ventricle, negative inotropic sensitivity to nicardipine and verapamil was significantly higher in the neonate than in the adult, which indicates that trans-sarcolemmal Ca2+ influx through the L-type Ca2+ channel becomes a progressively less-potent determinant of contractile force during postnatal development. The density of Ca2+ channels on the myocardial cell membrane as determined by specific binding sites for nicardipine was reported to increase two-fold during postnatal development [66]. The density of ICa on the cell membrane of the late-fetal mouse cardiomyocytes is comparable to that of the adult [67]. Thus, the developmental decrease in dependence of contraction on Ca2+ influx is not accompanied by a decrease in the number of functional Ca2+ channels themselves. It rather correlates with the shortening of the action potential duration due to developmental changes in the repolarizing potassium currents [15,16]. Similar shortening of the action potential duration [21] and a decrease in the inotropic sensitivity to nicardipine and verapamil have also been reported in the rat ventricular myocardium [50,68]. The postnatal changes appear to be larger in the mouse than in the rat. As the action potential duration of the neonatal mouse is much shorter than that of the neonatal rat, the corresponding developmental changes might be taking place earlier during the fetal period in the case of the mouse. In the case of the guinea pig, the Ca2+ channel blocker nicardipine was similarly effective in the ventricle from fetal, neonatal, and adult ventricle [51]. This appears to reflect the changes in action potential duration; the developmental shortening of the duration was less prominent in the guinea pig than in the mouse and rat (Figure 1).
The negative inotropic sensitivity to ryanodine and cyclopiazonic acid was higher in the adult mouse than in the neonate, indicating that the role of SR in myocardial contraction and relaxation increases during postnatal development of the mouse [19]. Shortening of the late-plateau phase of action potentials by ryanodine, which reflects the amount of Ca2+ released from the SR, was observed in the adult mouse [19]. A three-fold developmental increase in the amount of the SR Ca2+ ATPase and its regulatory protein, phospholamban, has been reported in mouse myocardia [34]. The amount of both proteins was regulated at the transcriptional level, and the changes were accompanied by a developmental increase in the Ca2+ uptake velocity of SR vesicles. The SR Ca2+ ATPase determines the maximum uptake capacity, while phospholamban negatively regulates its sensitivity; the coordinated regulation of the expression levels of these two SR proteins may be necessary for maintaining Ca2+ homeostasis in the developing heart. Changes in cell morphology related to Ca2+ handling also take place during development. Fluorescence confocal microscopy revealed that the SR increases progressively during pre- and postnatal development of the mouse ventricle [19]. T-tubules were absent in the fetus and neonate, were present only in the subsarcolemmal region at 1 week after birth and were present throughout the cell by 2 weeks after birth. The amplitude of Ca2+ transients, as well as its ryanodine-sensitive component, increased gradually with age. In the neonate and 1-week-old mice, Ca2+ concentration at the cell center showed slower rise than in the subsarcolemmal region. In 2- and 4-week-old mice, Ca2+ concentration increased simultaneously across the entire width of the cell. These results indicated that the shortening of the action potential duration during the late-fetal period and the development of T-tubule-SR coupling during the second postnatal week largely contribute to the developmental increase in the dependence of contraction on SR function. Similar developmental increases in inotropic responses to ryanodine [50,68,69,70,71] and cyclopiazonic acid [72] have been observed in the postnatal rat. Developmental increases in negative inotropic sensitivity to ryanodine have also been reported in postnatal rabbit [73], late-fetal guinea pig [51], and middle-aged chick embryos, although the decrease in contractile force by ryanodine of these species was smaller than in the adult mouse ventricle. The effectiveness of ryanodine and cyclopiazonic acid on the SR in neonatal myocardia was confirmed with skinned myocardial fibers and rapid scanning confocal microscopy on cardiomyocytes.

6. Adrenoceptor-Mediated Inotropy in the Adult

The sympathetic nervous system is the major accelerator of the heart, and the positive chronotropic and inotropic responses to the transmitter, noradrenaline, are mainly mediated by β-adrenoceptor-induced increase in intracellular cAMP. The subsequent activation of protein kinase A results in several events, such as enhancement of Ca2+ influx through the sarcolemmal Ca2+ channel, acceleration of Ca2+ uptake into the SR, enhanced activity of the SR Ca2+ release channel, and changes in the Ca2+ sensitivity of the myofilaments. In addition to the β-adrenoceptor-mediated inotropy, α-adrenoceptors are present in the myocardium, and their stimulation generally produces no or weak positive inotropy through mechanisms different from those for β-adrenoceptor stimulation [25,74,75]). Sustained positive inotropy is observed in the rabbit, guinea pig, and rat ventricle, but in the guinea pig and rat, a transient negative phase is observed before the positive phase (Figure 3A). The adult mouse right ventricle showed a characteristic sustained negative inotropic response to α-adrenoceptor stimulation (Figure 3(Ba)) [28]. Similar sustained negative inotropy was observed in the mouse ventricle with endothelin-1 and angiotensin II [67]. The negative inotropic response to α-adrenoceptor stimulation in the mouse was accompanied by shortening of the slowly repolarizing phase of the action potential [17]. As this phase reflects extrusion by the NCX of Ca2+ released from the SR, it was probable that Ca2+ release from the SR was decreased by α-adrenoceptor stimulation. In fact, the amplitude of post-rest contraction, which reflects Ca2+ released from the SR, was attenuated after α-adrenoceptor stimulation. Attenuation of the Ca2+ transient by endothelin-1 was reported with mouse ventricular strips [76]. α-Adrenoceptor-mediated negative inotropy was not affected by ryanodine and cyclopiazonic acid. The time course of contraction and relaxation was not affected by α-adrenoceptor stimulation. These results indicated that α -adrenoceptor-mediated decrease in SR Ca2+ release was due to indirect effect through trans-sarcolemmal Ca2+ movements. α-Adrenoceptor-mediated negative inotropy was not affected by nicardipine, ouabain, and dimethylamiloride but was concentration-dependently inhibited by SEA0400, a selective inhibitor of NCX (Figure 3(Cb)) [17]. It was also attenuated under elevated external Ca2+ or decreased external Na+ conditions, which inhibit Ca2+ extrusion by the NCX. In voltage-clamped mouse ventricular myocytes, α-adrenoceptor stimulation increased the NCX current in both outward and inward directions. These results suggested that α-adrenoceptor stimulation decreased SR Ca2+ content through enhancement of Ca2+ extrusion by the NCX and resulted in negative inotropy. In isolated mouse ventricular myocytes excited at low frequencies, α-adrenoceptor stimulation was reported to reduce cell shortening, with no significant reduction in Ca2+ transient amplitude [77]. This suggests that factors other than the above-mentioned NCX-mediated decrease in Ca2+ transient amplitude, such as decrease in Ca2+ sensitivity of the contractile proteins [78], may also be involved in the α-adrenoceptor-mediated negative inotropy in the mouse ventricle.

7. Developmental Changes in β-Adrenoceptor-Mediated Regulation

Developmental changes occur not only in the excitation–contraction mechanisms, but also in the response to autonomic transmitters and various endogenous substances. The mouse heart starts to beat on the 9th day of fetal life [79], and its responsiveness to noradrenaline [80] and acetylcholine [81] is reported to increase rapidly during the late-fetal period. Further modifications of the response to transmitters occur during the early postnatal period. We have found that although noradrenaline produces a positive chronotropic and inotropic response during all stages of pre-and postnatal development, the sensitivity (pD2 values) to noradrenaline is higher in the neonatal mouse than in the adult [82]. This phenomenon was also observed in the developing rat, and appeared to be related to the increase in autonomic innervation, which occurs postnatally [83,84]. Increase in the sympathetic innervation of the ventricle was confirmed with the increase in inotropic responsiveness to tyramine, which releases noradrenaline from sympathetic nerve terminals. We investigated the mechanisms for the 10-fold postnatal decrease in the inotropic sensitivity to noradrenaline of the mouse and rat ventricle and found that two different mechanisms were involved. Firstly, increased uptake of the transmitter by sympathetic nerve terminals decreases the effective transmitter concentration at the receptor site and results in an apparent decrease in the sensitivity to applied noradrenaline (pre-junctional mechanism). This was confirmed by the observation that the sensitivity to noradrenaline is increased in the adult ventricle in the presence of desipramine, which inhibits neuronal uptake of the transmitter; this effect of desipramine was not observed in the neonate. Secondly, there was a decrease in the sensitivity to β-adrenoceptor-mediated intracellular mechanisms (post-junctional mechanisms). This was suggested by the observation that the sensitivity to noradrenaline was higher in the neonate than in the adult when compared in the presence of desipramine and that the sensitivity to isoproterenol, which is not taken up into nerve terminals, was also higher in the neonate. Such developmental decrease in sensitivity to noradrenaline was also observed in the late-fetal and neonatal rat heart, and both pre- and post-junctional mechanisms were involved. As no developmental change in sensitivity to dibutyryl cAMP and forskolin was observed, the developmental decrease in sensitivity in the rat heart to β-adrenoceptor stimulation was attributed to changes in the mechanisms prior to cAMP, such as β-adrenoceptor density and G-protein-mediated coupling of the receptor to adenylate cyclase [85]. The observed parallelism between the developmental increase in innervation and the decrease in post-junctional sensitivity to β-adrenoceptor stimulation suggested the presence of a causal relationship. Surgical [86] and chemical [87] denervation of the rat heart resulted in elevated post-junctional sensitivity to noradrenaline. Isolation of the rat atria from sympathetic influence by organ culture resulted in high sensitivity to noradrenaline, similar to that observed in the fetal period prior to the development of sympathetic innervation; this was reversed by application of the neurotransmitter, noradrenaline, in the culture medium, suggesting that constant stimulation of the β-adrenoceptor by endogenous transmitter is important for the maintenance of sensitivity [84]. These results indicate that sympathetic innervation exerts influence on the myocardium to regulate its sensitivity to the neurotransmitter. Such a relationship has also been suggested for the response of the rat vas deferens to α-adrenergic stimulation [88,89]. The developmental decrease in sensitivity to β-adrenoceptor stimulation was accompanied by both a decrease in receptor density and the coupling of the receptor with adenylate-cyclase [85]. This is similar to the case of heart failure, which is characterized with an impaired β-adrenoceptor-mediated inotropy accompanied by decreases in sarcolemmal β-adrenoceptor density (down-regulation) and coupling with intracellular mechanisms (desensitization) [90,91,92]. Such a condition of reduced β-adrenoceptor responsiveness is induced by the hyperactivity of the sympathetic nervous system to compensate for the reduced cardiac function. Experimentally, a similar condition of cardiac remodeling can be created by administration of β-adrenoceptor agonists [93].

8. Developmental Changes in α-Adrenoceptor-Mediated Regulation

As mentioned above, the adult mouse right ventricle shows a characteristic negative inotropic response to α-adrenoceptor stimulation. In contrast, the α-adrenoceptor mediated inotropy in mouse ventricle is positive during the first postnatal week [26]. It gradually decreases and is converted to negative by the third postnatal week. The α-adrenoceptor-mediated component contributes to the overall inotropic response to noradrenaline, both in the neonate and adult. Inotropic response to endothelin-1 and angiotensin II was also positive in the neonate, and developmentally converted to negative. As the developmental time course of the conversion of α-adrenoceptor-mediated inotropy from positive to negative paralleled the increase in sympathetic innervation density, we performed chemical denervation of the postnatal mouse to clarify whether there is any causal relationship [94]. The conversion of inotropy from positive to negative was not inhibited, but the sensitivity of the response to α-adrenoceptor stimulation was rather increased in denervated myocardia. These findings provide additional evidence for the above-mentioned view that sympathetic innervation is causally involved in the adjustment of the sensitivity of the effector organ to the neurotransmitter.
Concerning the cellular mechanisms for the developmental conversion of α-adrenoceptor-mediated inotropy from positive to negative, we are considering the positive and negative components of inotropy separately, and both appear to be related to the developmental shortening of the action potential. As mentioned above, the negative inotropy in the adult could be attributed to enhanced NCX leading to the reduction of intracellular Ca2+ involved in contraction. NCX counter-transports three Na+ ions for a single Ca2+ ion, and the direction and amount are determined by the trans-sarcolemmal concentration gradient of these ions and the membrane potential. The short action potential in the adult mouse ventricle favors the NCX operating in the Ca2+ extruding direction, so that enhancement of NCX by α-adrenoceptor stimulation results in a reduction of intracellular Ca2+. Such a mechanism would be less favored in the neonatal myocardium, which has a longer action potential duration. On the other hand, the α-adrenoceptor-mediated positive inotropy observed in the neonate is mediated by enhanced influx of Ca2+ through Ca2+ channels [27]. The positive inotropy was not affected by SEA0400, or by low Na+ extracellular solution, but was significantly reduced by nifedipine (Figure 3(Ca)), which inhibits Ca2+ influx through Ca2+ channels. In voltage-clamped cardiomyocytes from the neonatal ventricle, α-adrenoceptor stimulation results in an increase in the Ca2+ channel current amplitude with no changes in the voltage for activation. The outward potassium current was not affected by α-adrenoceptor stimulation. The positive inotropy was accompanied by an increase in action potential duration, which appeared to be an enhancing factor for the inotropy. The observation that pharmacological inhibition of the action potential prolongation by cromakalim, an ATP-sensitive K+-channel opener, significantly reduced the positive inotropy, supports this view. Such a mechanism is less favored in the adult myocardium in which an extremely strong repolarization takes place. Thus, the developmental change in inotropy is closely related to the developmental change in excitation–contraction mechanisms.

9. Resemblance of the Diseased Myocardium to the Developing Myocardium

The phenotypes of diseased myocardium appear to resemble those of the developing myocardium [95,96]. In the failing myocardium, the structure of the t-tubules and the SR that formed gradually during development are partly disrupted. The effective coupling between the t-tubule and the SR decreases. This results in a less-synchronized release of Ca2+ from the SR; some of the Ca2+ release channels are activated not directly by the influx Ca2+ from the t-tubules, but by the Ca2+ released from the neighboring Ca2+ release units [97], which is similar to the pattern in the neonatal myocardium [19,70]. In the diabetic myocardium of the mouse, these changes in cell structure are relatively modest, but a reduction in SR Ca2+ content is caused by the decreased expression of the SR Ca2+ pump and increased Ca2+ leak from the Ca2+ release channel, due to changes in its phosphorylation [98,99,100]. This results in a reduced amplitude and prolonged duration of the Ca2+ transient, decreased contractile force and slower relaxation of the myocardium [98,99,101]. This is accompanied by a prolongation of the action potential duration, which may be a mechanism to compensate for the decrease in contractile force. Further, the degree of α-adrenoceptor-mediated negative inotropy is reduced [102]. It appears as if the excitation–contraction properties of the myocardium reverted to the neonatal stage, as described above. To normalize the impaired SR function, the search for compounds which activate the SR Ca2+ pump is now in progress [101,103,104,105,106,107].
α-Adrenoceptor-mediated positive inotropy observed in heart failure is probably a compensatory mechanism to maintain cardiac output under impaired β-adrenoceptor mediated inotropy [25,75]. Among the three subtypes, α1A, α1B and α1D, the α1A subtype is most abundantly expressed in the cardiomyocyte both in mice and humans. Further, the abundance of the α1A subtype is maintained under heart failure. Thus, the mouse appears to be a suitable model to study human heart failure. α1A receptor-induced positive inotropy is accompanied by increases in cytoplasmic pH, the phosphorylation of the myosin light chain, and the Ca2+ sensitivity of the myofilaments. Under experimental heart failure induced by administration of a β-adrenergic agonist to mice, additional administration of an α-agonist induced an establishment of an α-adrenoceptor-mediated positive inotropy [93]. Thus, α-adrenergic stimuli not only induced positive inotropy, but also caused an enhancement in the α-adrenergic sensitivity itself. This was opposite in direction to the sympathetic nerve-induced decrease in sensitivity observed in the neonate mentioned above [94]. Thus, although positive inotropy is observed both in the neonatal and failing heart, the influence of α-adrenoceptor stimulation on the sensitivity of α-adrenoceptor-mediated inotropy appears to differ between the neonatal heart and the failing adult heart. Studies on the effectiveness of α-adrenoceptor agonists against heart failure are performed in mice and in human patients, and positive results are reported [108,109,110].

10. Functional Significance of the Developmental Changes

In this review, we summarized the action potential and excitation–contraction properties of the ventricular myocardium and their regulation through α- and β-adrenoceptor stimulation in small experimental animals, the guinea pig, rat, and mouse. The myocardium of the adult guinea pig had properties relatively close to those of larger animals and humans, such as a relatively low beating rate, an action potential with a plateau phase, a balanced dependence on contraction on both trans-sarcolemmal Ca2+ influx and SR Ca2+ release, and positive inotropic responses to both α- and β-adrenoceptor stimulation. In contrast, the myocardium of the adult mouse, and to a lesser extent, the adult rat, has different characteristics, such as high beating rate, extremely short action potential, and high dependence on SR Ca2+ release. The adult mouse myocardium showed a unique negative inotropic response to α-adrenoceptor stimulation. Such species difference was not so evident in the fetal stage. A shortening of the action potential and increase in the dependence on SR function took place during pre- and postnatal development. Such changes in the basic excitation–contraction properties of the myocardium appeared to be closely related to the changes in inotropic responses, especially to α-adrenoceptor stimulation in the mouse. The developmental changes, as well as the species difference, probably have physiological significance. For example, the high sensitivity to β-adrenoceptor stimulation of fetal myocardia would be of advantage in responding to circulating catecholamines in the absence of direct sympathetic innervation. The developmental conversion of α-adrenoceptor-induced inotropy from positive to negative in the mouse may be a mechanism to attenuate and optimize cardiac performance under the high beating rate in the adult. Studying the developmental changes in myocardial excitation–contraction mechanisms and their regulation would provide clues for a more comprehensive understanding of cardiac function.

Author Contributions

Conceptualization, S.H., N.A., M.S., I.N. and H.T.; writing—original draft preparation, S.H., N.A., M.S., I.N. and H.T.; writing—review and editing, S.H., N.A., M.S., I.N. and H.T.; funding acquisition, S.H., I.N. and H.T. All authors have read and agreed to the published version of the manuscript.

Funding

This study was supported in part by JSPS KAKENHI, grant numbers JP20K16013, JP20K07299, and JP20K07091.

Data Availability Statement

No new data were created or analyzed in this study.

Conflicts of Interest

The authors declare no conflicts of interest.

References

  1. Barth, E.; Stämmler, G.; Speiser, B.; Schaper, J. Ultrastructural quantitation of mitochondria and myofilaments in cardiac muscle from 10 different animal species including man. J. Mol. Cell. Cardiol. 1992, 24, 669–681. [Google Scholar] [CrossRef]
  2. Blank, S.; Chen, V.; Hamilton, N.; Salerno, T.A.; Ianuzzo, C.D. Biochemical characteristics of mammalian myocardia. J. Mol. Cell. Cardiol. 1989, 21, 367–373. [Google Scholar] [CrossRef] [PubMed]
  3. Hamilton, N.; Lanuzzo, C.D. Contractile and calcium regulating capacities of myocardia of different sized mammals scale with resting heart rate. Mol. Cell. Biochem. 1991, 106, 133–141. [Google Scholar] [CrossRef]
  4. Milani-Nejad, N.; Janssen, P.M.L. Small and large animal models in cardiac contraction research: Advantages and disadvantages. Pharmacol. Ther. 2014, 141, 235–249. [Google Scholar] [CrossRef]
  5. Varro, A.; Lathrop, D.A.; Hester, S.B.; Nanasi, P.P.; Papp, J.G.Y. Ionic currents and action potentials in rabbit, rat, and guinea pig ventricular myocytes. Basic. Res. Cardiol. 1993, 88, 93–102. [Google Scholar] [CrossRef] [PubMed]
  6. Binah, O.; Arieli, R.; Beck, R.; Rosen, M.R.; Palti, Y. Ventricular electrophysiological properties: Is interspecies variability related to thyroid state? Am. J. Physiol. 1987, 252, H1265–H1274. [Google Scholar] [CrossRef]
  7. Joukar, S. A comparative review on heart ion channels, action potentials and electrocardiogram in rodents and human: Extrapolation of experimental insights to clinic. Lab. Anim. Res. 2021, 37, 25. [Google Scholar] [CrossRef] [PubMed]
  8. Salameh, S.; Ogueri, V.; Posnack, N.G. Adapting to a new environment: Postnatal maturation of the human cardiomyocyte. J. Physiol. 2023, 601, 2593–2619. [Google Scholar] [CrossRef]
  9. Nerbonne, J.M. Molecular basis of functional voltage-gated K+ channel diversity in the mammalian myocardium. J. Physiol. 2000, 525, 285–298. [Google Scholar] [CrossRef]
  10. Agata, N.; Tanaka, H.; Shigenobu, K. Developmental changes in action potential properties of the guinea-pig myocardium. Acta. Physiol. Scand. 1993, 149, 331–337. [Google Scholar] [CrossRef]
  11. Kato, Y.; Masumiya, H.; Agata, N.; Tanaka, H. Developmental changes in action potential and membrane currents in fetal, neonatal and adult guinea-pig ventricular myocytes. J. Mol. Cell. Cardiol. 1996, 28, 1515–1522. [Google Scholar] [CrossRef]
  12. Sun, L.S.; Rosen, M.R. The electrophysiologic effects of bupivacaine on adult, neonatal, and fetal guinea pig papillary muscles. Anesthesiology 1991, 74, 893–899. [Google Scholar] [CrossRef]
  13. Matsuoka, S.; Sarai, N.; Kuratomi, S.; Ono, K.; Noma, A. Role of individual ionic current systems in ventricular cells hypothesized by a model study. Jpn. J. Physiol. 2003, 53, 105–123. [Google Scholar] [CrossRef] [PubMed]
  14. Nilius, B.; Boldt, W.; Benndorf, K. Properties of aconitine-modified sodium channels in single cells of mouse ventricular myocardium. Gen. Physiol. Biophys. 1986, 5, 473–484. [Google Scholar]
  15. Wang, L.; Feng, Z.P.; Kondo, C.S.; Sheldon, R.S.; Duff, H.J. Developmental changes in the delayed rectifier K+ channels in mouse heart. Circ. Res. 1996, 79, 79–85. [Google Scholar] [CrossRef] [PubMed]
  16. Wang, L.; Duff, H. Developmental changes in transient outward current in mouse ventricle. Circ. Res. 1997, 81, 120–127. [Google Scholar] [CrossRef]
  17. Nishimaru, K.; Kobayashi, M.; Matsuda, T.; Tanaka, Y.; Tanaka, H.; Shigenobu, K. Alpha-Adrenoceptor stimulation-mediated negative inotropism and enhanced Na+/Ca2+ exchange in mouse ventricle. Am. J. Physiol. 2001, 280, H132–H141. [Google Scholar]
  18. Tanaka, H.; Namekata, I.; Takeda, K.; Kazama, A.; Shimizu, Y.; Moriwaki, R.; Hirayama, W.; Sato, A.; Kawanishi, T.; Shigenobu, K. Unique excitation-contraction characteristics of mouse myocardium as revealed by SEA0400, a specific inhibitor of Na+-Ca2+ exchanger. Naunyn Schmiedebergs Arch. Pharmacol. 2005, 371, 526–534. [Google Scholar] [CrossRef] [PubMed]
  19. Hamaguchi, S.; Kawakami, Y.; Honda, Y.; Nemoto, K.; Sano, A.; Namekata, I.; Tanaka, H. Developmental changes in excitation-contraction mechanisms of the mouse ventricular myocardium as revealed by functional and confocal imaging analyses. J. Pharmacol. Sci. 2013, 123, 167–175. [Google Scholar] [CrossRef]
  20. Grandy, S.A.; Trepanier-Boulay, V.; Fiset, C. Postnatal development has a marked effect on ventricular repolarization in mice. Am. J. Physiol. Heart Circ. Physiol. 2007, 293, H2168–H2177. [Google Scholar] [CrossRef]
  21. Kilborn, M.J.; Fedida, D. A study of the developmental changes in outward currents of rat ventricular myocytes. J. Physiol. 1990, 430, 37–60. [Google Scholar] [CrossRef]
  22. Demir, S.S. Computational modeling of cardiac ventricular action potentials in rat and mouse: Review. Jpn. J. Physiol. 2004, 54, 523–530. [Google Scholar] [CrossRef]
  23. Chen, B.; Guo, A.; Zhang, C.; Chen, R.; Zhu, Y.; Hong, J.; Kutschke, W.; Zimmerman, K.; Weiss, R.M.; Zingman, L.; et al. Critical roles of junctophilin-2 in T-tubule and excitation-contraction coupling maturation during postnatal development. Cardiovasc. Res. 2013, 100, 54–62. [Google Scholar] [CrossRef] [PubMed]
  24. Reynolds, J.O.; Chiang, D.Y.; Wang, W.; Beavers, D.L.; Dixit, S.S.; Skapura, D.G.; Landstrom, A.P.; Song, L.S.; Ackerman, M.J.; Wehrens, X.H. Junctophilin-2 is necessary for T-tubule maturation during mouse heart development. Cardiovasc. Res. 2013, 100, 44–53. [Google Scholar] [CrossRef] [PubMed]
  25. Endoh, M. Cardiac α1-adrenoceptors and inotropy: Myofilament Ca2+ sensitivity, intracellular Ca2+ mobilization, signaling pathway, and pathophysiological relevance. Circ. Res. 2016, 119, 587–590. [Google Scholar] [CrossRef] [PubMed]
  26. Tanaka, H.; Manita, S.; Matsuda, T.; Adachi, M.; Shigenobu, K. Sustained negative inotropism mediated by alpha-adrenoceptors in adult mouse myocardia: Developmental conversion from positive response in the neonate. Br. J. Pharmacol. 1995, 114, 673–677. [Google Scholar] [CrossRef]
  27. Hamaguchi, S.; Morinou, I.; Shiseki, Y.; Mikami, A.; Seki, M.; Namekata, I.; Tanaka, H. Mechanisms for the α-adrenoceptor-mediated positive inotropy in mouse ventricular myocardium: Enhancing effect of action potential prolongation. Int. J. Mol. Sci. 2023, 24, 3926. [Google Scholar] [CrossRef]
  28. Harrell, M.D.; Harbi, S.; Hoffman, J.F.; Zavadil, J.; Coetzee, W.A. Large-scale analysis of ion channel gene expression in the mouse heart during perinatal development. Physiol. Genomics 2007, 28, 273–283. [Google Scholar] [CrossRef]
  29. Domínguez, J.N.; de la Rosa, A.; Navarro, F.; Franco, D.; Aránega, A.E. Tissue distribution and subcellular localization of the cardiac sodium channel during mouse heart development. Cardiovasc. Res. 2008, 78, 45–52. [Google Scholar] [CrossRef]
  30. Liu, W.; Yasui, K.; Opthof, T.; Ishiki, R.; Lee, J.K.; Kamiya, K.; Yokota, M.; Kodama, I. Developmental changes of Ca2+ handling in mouse ventricular cells from early embryo to adulthood. Life Sci. 2002, 71, 1279–1292. [Google Scholar] [CrossRef]
  31. Takemura, H.; Yasui, K.; Opthof, T.; Niwa, N.; Horiba, M.; Shimizu, A.; Lee, J.K.; Honjo, H.; Kamiya, K.; Ueda, Y.; et al. Subtype switching of L-Type Ca2+ channel from Cav1.3 to Cav1.2 in embryonic murine ventricle. Circ. J. 2005, 69, 1405–1411. [Google Scholar] [CrossRef] [PubMed]
  32. Sagawa, H.; Hoshino, S.; Yoshioka, K.; Ding, W.G.; Omatsu-Kanbe, M.; Nakagawa, M.; Maruo, Y.; Matsuura, H. Postnatal developmental changes in the sensitivity of L-type Ca2+ channel to inhibition by verapamil in a mouse heart model. Pediatr. Res. 2018, 83, 1207–1217. [Google Scholar] [CrossRef]
  33. Yasui, K.; Niwa, N.; Takemura, H.; Opthof, T.; Muto, T.; Horiba, M.; Shimizu, A.; Lee, J.K.; Honjo, H.; Kamiya, K.; et al. Pathophysiological significance of T-type Ca2+ channels: Expression of T-type Ca2+ channels in fetal and diseased heart. J. Pharmacol. Sci. 2005, 99, 205–210. [Google Scholar] [CrossRef] [PubMed]
  34. Harrer, J.M.; Haghighe, K.; Kim, H.; Ferguson, D.; Kranias, E. Coordinate regulation of SR Ca2+-ATPase and phospholamban expression in developing murine heart. Am. J. Physiol. 1997, 272, H57–H66. [Google Scholar] [PubMed]
  35. Piquereau, J.; Novotova, M.; Fortin, D.; Garnier, A.; Ventura-Clapier, R.; Veksler, V.; Joubert, F. Postnatal development of mouse heart: Formation of energetic microdomains. J. Physiol. 2010, 588, 2443–2454. [Google Scholar] [CrossRef]
  36. de Diego, C.; Chen, F.; Xie, L.H.; Dave, A.S.; Thu, M.; Rongey, C.; Weiss, J.N.; Valderrábano, M. Cardiac alternans in embryonic mouse ventricles. Am. J. Physiol. Heart Circ. Physiol. 2008, 294, H433–H440. [Google Scholar] [CrossRef]
  37. Reppel, M.; Reuter, H.; Sasse, P.; Hescheler, J.; Fleischmann, B.K. NCX current in the murine embryonic heart: Development-dependent regulation by Na+. Ann. N. Y. Acad. Sci. 2007, 1099, 175–182. [Google Scholar] [CrossRef]
  38. Xu, Y.; Dong, P.H.; Zhang, Z.; Ahmmed, G.U.; Chiamvimonvat, N. Presence of a calcium-activated chloride current in mouse ventricular myocytes. Am. J. Physiol. Heart Circ. Physiol. 2002, 283, H302–H314. [Google Scholar] [CrossRef]
  39. Mitchel, M.R.; Powell, T.; Terrar, D.A.; Twist, V.W. The effects of ryanodine, EGTA and low-sodium on action potentials in rat and guinea-pig ventricular myocytes: Evidence for two inward currents during the plateau. Br. J. Pharmacol. 1984, 81, 543–550. [Google Scholar] [CrossRef]
  40. Kimura, J.; Watano, T.; Kawahara, M.; Sakai, E.; Yatabe, J. Direction-independent block of bi-directional Na+/Ca2+ exchange current by KB-R7943 in guinea-pig cardiac myocytes. Br. J. Pharmacol. 1999, 128, 969–974. [Google Scholar] [CrossRef]
  41. Matsuda, T.; Arakawa, N.; Takuma, K.; Kishida, Y.; Kawasaki, Y.; Sakaue, M.; Takahashi, K.; Takahashi, T.; Suzuki, T.; Takahashi, A.; et al. SEA0400, a novel and selective inhibitor of the Na+-Ca2+ exchanger, attenuates reperfusion injury in the in vitro and in vivo cerebral ischemic models. J. Pharmacol. Exp. Ther. 2001, 298, 249–256. [Google Scholar] [PubMed]
  42. Gadeberg, H.C.; Kong, C.H.T.; Bryant, S.M. Sarcolemmal distribution nof ICa and INCX and Ca2+ autoregulation in mouse ventricular myocytes. Am. J. Physiol. Heart Circ. Physiol. 2017, 313, H190–H199. [Google Scholar] [CrossRef]
  43. Brette, F.; Sallé, L.; Orchard, C.H. Differential modulation of L-type Ca2+ current by SR Ca2+ release at the T-tubules and surface membrane of rat ventricular myocytes. Circ. Res. 2004, 95, e1–e7. [Google Scholar] [CrossRef]
  44. Ramos-Franco, J.; Aguilar-Sanchez, Y.; Escobar, A.L. Intact Heart Loose Patch Photolysis Reveals Ionic Current Kinetics During Ventricular Action Potentials. Circ. Res. 2016, 118, 203–215. [Google Scholar] [CrossRef]
  45. Agata, N.; Tanaka, H.; Shigenobu, K. Differential effects of hypoxia on electrical and mechanical activities of isolated ventricular muscles from fetal and adult guinea-pigs. Gen. Pharmacol. 1994, 25, 15–18. [Google Scholar] [CrossRef]
  46. Agata, N.; Kato, Y.; Hamaguchi, S.; Namekata, I.; Tanaka, H. Resistance of fetal guinea pig ventricular myocardium to hypoxia: Maintained intracellular ATP prevents the opening of ATP-sensitive potassium channels. Biol. Pharm. Bull. 2019, 42, 268–272. [Google Scholar] [CrossRef]
  47. Hirakow, R.; Goto, T. Quantitative studies on the ultrastructural differentiation and growth of mammalian cardiac muscle cells. II. The atria and ventricles of the guinea pig. Acta Anat. 1980, 108, 230–237. [Google Scholar] [CrossRef] [PubMed]
  48. Tanaka, H.; Kawanishi, T.; Shigenobu, K. Optical bioimaging: From living tissue to a single molecule: Atrio-ventricular difference in myocardial excitation-contraction coupling--sequential versus simultaneous activation of SR Ca2+ release units. J. Pharmacol. Sci. 2003, 93, 248–252. [Google Scholar] [CrossRef] [PubMed]
  49. Bouchard, R.A.; Clark, R.B.; Giles, W.R. Effects of Action Potential Duration on Excitation-Contractio Couplig in Rat Ventricular Myocytes. Action Potential Voltage-Clamp Measurements. Circ. Res. 1995, 76, 790–801. [Google Scholar] [CrossRef]
  50. Tanaka, H.; Shigenobu, K. Effect of ryanodine on neonatal and adult rat heart: Developmental increase in sarcoplasmic reticulum function. J. Mol. Cell. Cardiol. 1989, 21, 1305–1313. [Google Scholar] [CrossRef]
  51. Agata, N.; Tanaka, H.; Shigenobu, K. Inotropic effects of ryanodine and nicardipine on fetal, neonatal and adult guinea-pig myocardium. Eur. J. Pharmacol. 1994, 260, 47–55. [Google Scholar] [CrossRef]
  52. Orchard, C.; Brette, F. t-Tubules and sarcoplasmic reticulum function in cardiac ventricular myocytes. Cardiovasc. Res. 2008, 77, 237–244. [Google Scholar] [CrossRef] [PubMed]
  53. Dibb, K.M.; Louch, W.E.; Trafford, A.W. Cardiac Transverse Tubules in Physiology and Heart Failure. Annu. Rev. Physiol. 2022, 84, 229–255. [Google Scholar] [CrossRef]
  54. Lipsett, D.B.; Frisk, M.; Aronsen, J.M.; Nordén, E.S.; Buonarati, O.R.; Cataliotti, A.; Hell, J.W.; Sjaastad, I.; Christensen, G.; Louch, W.E. Cardiomyocyte substructure reverts to an immature phenotype during heart failure. J. Physiol. 2019, 597, 1833–1853. [Google Scholar] [CrossRef] [PubMed]
  55. Ziman, A.P.; Gómez-Viquez, N.L.; Bloch, R.J.; Lederer, W.J. Excitation-contraction coupling changes during postnatal cardiac development. J. Mol. Cell. Cardiol. 2010, 48, 379–386. [Google Scholar] [CrossRef] [PubMed]
  56. Perdreau-Dahl, H.; Lipsett, D.B.; Frisk, M.; Kermani, F.; Carlson, C.R.; Brech, A.; Shen, X.; Bergan-Dahl, A.; Hou, Y.; Tuomainen, T.; et al. BIN1, Myotubularin, and Dynamin-2 Coordinate T-Tubule Growth in Cardiomyocytes. Circ. Res. 2023, 132, e188–e205. [Google Scholar] [CrossRef]
  57. Xu, C.; Zhang, G.; Wang, X.; Huang, X.; Zhang, J.; Han, S.; Wang, J.; Hall, D.D.; Xu, R.; He, F.; et al. Ptpn23 Controls Cardiac T-Tubule Patterning by Promoting the Assembly of Dystrophin-Glycoprotein Complex. Circulation 2024, 149, 1375–1390. [Google Scholar] [CrossRef]
  58. Hofhuis, J.; Bersch, K.; Wagner, S.; Molina, C.; Fakuade, F.E.; Iyer, L.M.; Streckfuss-Bömeke, K.; Toischer, K.; Zelarayán, L.C.; Voigt, N.; et al. Dysferlin links excitation-contraction coupling to structure and maintenance of the cardiac transverse-axial tubule system. Europace 2020, 22, 1119–1131. [Google Scholar] [CrossRef]
  59. Kawamura, Y.; Ishiwata, T.; Takizawa, M.; Ishida, H.; Asano, Y.; Nonoyama, S. Fetal and neonatal development of Ca2+ transients and functional sarcoplasmic reticulum in beating mouse hearts. Circ. J. 2010, 74, 1442–1450. [Google Scholar] [CrossRef]
  60. Takizawa, M.; Ishiwata, T.; Kawamura, Y.; Kanai, T.; Kurokawa, T.; Nishiyama, M.; Ishida, H.; Asano, Y.; Nonoyama, S. Contribution of sarcoplasmic reticulum Ca2+ release and Ca2+ transporters on sarcolemmal channels to Ca2+ transient in fetal mouse heart. Pediatr. Res. 2011, 69, 306–311. [Google Scholar] [CrossRef]
  61. Ko, C.Y.; Smith, C.E.R.; Grandi, E. Calcium-Dependent Signaling in Cardiac Myocytes. In Cardiovascular Signaling in Health and Disease [Internet]; Parinandi, N.L., Hund, T.J., Eds.; Springer: Cham, Switzerland, 2022. [Google Scholar] [CrossRef]
  62. Pásek, M.; Bébarová, M.; Šimurdová, M.; Šimurda, J. Functional consequences of changes in the distribution of Ca2+ extrusion pathways between t-tubular and surface membranes in a model of human ventricular cardiomyocyte. J. Mol. Cell. Cardiol. 2024, 193, 113–124. [Google Scholar] [CrossRef] [PubMed]
  63. Ruud, M.; Frisk, M.; Melleby, A.O.; Norseng, P.A.; Mohamed, B.A.; Li, J.; Aronsen, J.M.; Setterberg, I.E.; Jakubiczka, J.; van Hout, I.; et al. Regulation of cardiomyocyte t-tubule structure by preload and afterload: Roles in cardiac compensation and decompensation. J. Physiol. 2024; Online ahead of print. [Google Scholar] [CrossRef]
  64. Heinzel, F.R.; Bito, V.; Volders, P.G.; Antoons, G.; Mubagwa, K.; Sipido, K.R. Spatial and temporal inhomogeneities during Ca2+ release from the sarcoplasmic reticulum in pig ventricular myocytes. Circ. Res. 2002, 91, 1023–1130. [Google Scholar] [CrossRef] [PubMed]
  65. Biesmans, L.; Macquaide, N.; Heinzel, F.R.; Bito, V.; Smith, G.L.; Sipido, K.R. Subcellular heterogeneity of ryanodine receptor properties in ventricular myocytes with low T-tubule density. PLoS ONE. 2011, 6, e25100. [Google Scholar] [CrossRef] [PubMed]
  66. Erman, R.; Yamamura, H.; Roeske, W. The ontogeny of specific binding sites for the calcium channel antagonist, nitrendipine, in mouse heart and brain. Brain Res. 1983, 278, 327–331. [Google Scholar] [CrossRef]
  67. An, R.H.; Davies, M.F.; Doevendans, P.; Kubalak, S.W.; Bangalore, R.; Chien, K.R.; Kass, R.S. Developmental changes in beta-adrenergic modulation of L-type Ca2+ channels in embryonic mouse heart. Circ. Res. 1996, 78, 371–378. [Google Scholar] [CrossRef]
  68. Wibo, M.; Bravo, G.; Godfraind, T. Postnatal maturation of excitation-contraction coupling in rat ventricle in relation to the subcellular localization and surface density of 1,4-dihydropyridine and ryanodine receptors. Circ. Res. 1991, 66, 662–673. [Google Scholar] [CrossRef]
  69. Seki, S.; Nagashima, M.; Yamada, Y.; Tsutsuura, M.; Kobayashi, T.; Namiki, A.; Tohse, N. Fetal and postnatal development of Ca2+ transients and Ca2+ sparks in rat cardiomyocytes. Cardiovasc. Res. 2003, 58, 535–548. [Google Scholar] [CrossRef]
  70. Tohse, N.; Seki, S.; Kobayashi, T.; Tsutsuura, M.; Nagashima, M.; Yamada, Y. Development of excitation-contraction coupling in cardiomyocytes. Jpn. J. Physiol. 2004, 54, 1–6. [Google Scholar] [CrossRef]
  71. Kobayashi, T.; Maeda, S.; Ichise, N.; Sato, T.; Iwase, T.; Seki, S.; Yamada, Y.; Tohse, N. The beginning of the calcium transient in rat embryonic heart. J. Physiol. Sci. 2011, 61, 141–149. [Google Scholar] [CrossRef]
  72. Agata, N.; Tanaka, H.; Shigenobu, K. Possible action of cyclopiazonic acid on myocardial sarcoplasmic reticulum: Inotropic effects on neonatal and adult rat heart. Br. J. Pharmacol. 1993, 108, 571–572. [Google Scholar] [CrossRef]
  73. Seguchi, M.; Harding, J.A.; Jarmakani, J.M. Developmental change in the function of sarcoplasmic reticulum. J. Mol. Cell. Cardiol. 1986, 18, 189–195. [Google Scholar] [CrossRef] [PubMed]
  74. Terzic, A.; Puceat, M.; Vassort, G.; Vogel, S.M. Cardiac alpha 1-adrenoceptors: An overview. Pharmacol. Rev. 1993, 45, 147–175. [Google Scholar]
  75. Jensen, B.C.; O’Connell, T.D.; Simpson, P.C. Alpha-1-adrenergic receptors in heart failure: The adaptive arm of the cardiac response to chronic catecholamine stimulation. J. Cardiovasc. Pharmacol. 2014, 63, 291–301. [Google Scholar] [CrossRef] [PubMed]
  76. Izumi, M.; Miyamoto, S.; Hori, M.; Ozaki, H.; Karaki, H. Negative inotropic effect of endothelin-1 in the mouse right ventricle. Eur. J. Pharmacol. 2000, 396, 109–117. [Google Scholar] [CrossRef] [PubMed]
  77. Sakurai, K.; Norota, I.; Tanaka, H.; Kubota, I.; Tomoike, H.; Endo, M. Negative inotropic effects of angiotensin II, endothelin-1 and phenylephrine in indo-1 loaded adult mouse ventricular myocytes. Life Sci. 2002, 70, 1173–1184. [Google Scholar] [CrossRef] [PubMed]
  78. Hirano, S.; Kusakari, Y.; O-Uchi, J.; Morimoto, S.; Kawai, M.; Hongo, K.; Kurihara, S. Intracellular mechanism of the negative inotropic effect induced by alpha1-adrenoceptor stimulation in mouse myocardium. J. Physiol. Sci. 2006, 56, 297–304. [Google Scholar] [CrossRef]
  79. Sissman, N.J. Developmental landmarks in cardiac morphogenesis: Comparative chronology. Am. J. Cardiol. 1970, 25, 141–148. [Google Scholar] [CrossRef]
  80. Chen, F.; Yamamura, H.; Roeske, W. Ontogeny of mammalian myocardial beta-adrenergic receptors. Eur. J. Pharmacol. 1979, 58, 255–264. [Google Scholar] [CrossRef]
  81. Roeske, W.; Yamamura, H. Maturation of mammalian myocardial muscarinic cholinergic receptors. Life Sci. 1978, 23, 127–132. [Google Scholar] [CrossRef]
  82. Tanaka, H.; Manita, S.; Shigenobu, K. Increased sensitivity of neonatal mouse myocardia to autonomic transmitters. J. Auton. Pharmacol. 1994, 14, 123–128. [Google Scholar] [CrossRef]
  83. Shigenobu, K.; Tanaka, H.; Kasuya, Y. Changes in sensitivity of rat heart to norepinephrine and isoproterenol during pre- and postnatal development and its relation to sympathetic innervation. Dev. Pharmacol. Ther. 1988, 11, 226–236. [Google Scholar] [CrossRef] [PubMed]
  84. Shigenobu, K. Electrophysiological properties of chick embryonic heart and some pharmacological studies with rat myocardium during pre- and postnatal development. In Developmental Cardiology: Morphogenesis and Function; Clark, E.B., Takao, A., Eds.; Futura Publishing Co.: London, UK, 1990; pp. 273–289. [Google Scholar]
  85. Tanaka, H.; Shigenobu, K. Role of beta-adrenoceptor-adenylate cyclase system in the developmental decrease in sensitivity to isoprenaline in foetal and neonatal rat heart. Br. J. Pharmacol. 1990, 100, 138–142. [Google Scholar] [CrossRef]
  86. Goto, K.; Longhurst, P.A.; Cassis, L.A.; Head, R.J.; Taylor, D.A.; Rice, P.J.; Fleming, W.W. Surgical sympathectomy of the heart in rodents and its effect on sensitivity to agonists. J. Pharmacol. Exp. Ther. 1985, 234, 280–287. [Google Scholar] [PubMed]
  87. Ishii, K.; Shigenobu, K.; Kasuya, Y. Postjunctional supersensitivity in young rat heart produced by immunological and chemical sympathectomy. J. Pharmacol. Exp. Ther. 1982, 220, 209–215. [Google Scholar] [PubMed]
  88. Goto, K.; Masaki, T.; Saito, A.; Kasuya, Y. Denervation-like supersensitivity in the rat vas deferens induced by local application of colchicine to the hypogastric plexus. J. Pharmacol. Exp. Ther. 1979, 209, 376–381. [Google Scholar]
  89. Ono, K.; Kasuya, Y.; Shigenobu, K. Organ culture of young rat vas deferens as an in vitro model for the study of denervation supersensitivity. Eur. J. Pharmacol. 1985, 117, 159–168. [Google Scholar] [CrossRef]
  90. de Lucia, C.; Eguchi, A.; Koch, W.J. New Insights in Cardiac β-Adrenergic Signaling During Heart Failure and Aging. Front. Pharmacol. 2018, 9, 904. [Google Scholar] [CrossRef] [PubMed]
  91. Rajagopal, S.; Shenoy, S.K. GPCR desensitization: Acute and prolonged phases. Cell Signal. 2018, 41, 9–16. [Google Scholar] [CrossRef]
  92. Maaliki, D.; Jaffa, A.A.; Nasser, S.; Sahebkar, A.; Eid, A.H. Adrenoceptor Desensitization: Current Understanding of Mechanisms. Pharmacol. Rev. 2024, 76, 358–387. [Google Scholar] [CrossRef]
  93. Dewenter, M.; Pan, J.; Knödler, L.; Tzschöckel, N.; Henrich, J.; Cordero, J.; Dobreva, G.; Lutz, S.; Backs, J.; Wieland, T.; et al. Chronic isoprenaline/phenylephrine vs. exclusive isoprenaline stimulation in mice: Critical contribution of alpha1-adrenoceptors to early cardiac stress responses. Basic Res. Cardiol. 2022, 117, 15. [Google Scholar] [CrossRef]
  94. Tanaka, H.; Matsuda, T.; Adachi, M.; Shigenobu, K. Effect of sympathectomy on inotropic responsiveness to alpha-adrenoceptor stimulation in developing mouse myocardia. Can. J. Physiol. Pharmacol. 1995, 73, 1285–1288. [Google Scholar] [CrossRef] [PubMed]
  95. Louch, W.E.; Koivumäki, J.T.L.; Tavi, P. Calcium signalling in developing cardiomyocytes: Implications for model systems and disease. J. Physiol. 2015, 593, 1047–1063. [Google Scholar] [CrossRef] [PubMed]
  96. Birkedal, R.; Laasmaa, M.; Branovets, J.; Vendelin, M. Ontogeny of cardiomyocytes: Ultrastructure optimization to meet the demand for tight communication in excitation-contraction coupling and energy transfer. Philos. Trans. R. Soc. Lond. B Biol. Sci. 2022, 377, 20210321. [Google Scholar] [CrossRef]
  97. Louch, W.E.; Bito, V.; Heinzel, F.R.; Macianskiene, R.; Vanhaecke, J.; Flameng, W.; Mubagwa, K.; Sipido, K.R. Reduced synchrony of Ca2+ release with loss of T-tubules-a comparison to Ca2+ release in human failing cardiomyocytes. Cardiovasc. Res. 2004, 62, 63–73. [Google Scholar] [CrossRef] [PubMed]
  98. Shao, C.H.; Rozanski, G.J.; Patel, K.P.; Bidasee, K.R. Dyssynchronous (non-uniform) Ca2+ release in myocytes from streptozotocin-induced diabetic rats. J. Mol. Cell. Cardiol. 2007, 42, 234–246. [Google Scholar] [CrossRef] [PubMed]
  99. Stølen, T.O.; Høydal, M.A.; Kemi, O.J.; Catalucci, D.; Ceci, M.; Aasum, E.; Larsen, T.; Rolim, N.; Condorelli, G.; Smith, G.L.; et al. Interval training normalizes cardiomyocyte function, diastolic Ca2+ control, and SR Ca2+ release synchronicity in a mouse model of diabetic cardiomyopathy. Circ Res. 2009, 105, 527–536. [Google Scholar] [CrossRef]
  100. Bers, D. Cardiac Sarcoplasmic Reticulum Calcium Leak: Basis and Roles in Cardiac Dysfunction. Annu. Rev. Physiol. 2014, 76, 107–127. [Google Scholar] [CrossRef]
  101. Namekata, I.; Hamaguchi, S.; Wakasugi, Y.; Ohhara, M.; Hirota, Y.; Tanaka, H. Ellagic acid and gingerol, activators of the sarco-endoplasmic reticulum Ca²⁺-ATPase, ameliorate diabetes mellitus-induced diastolic dysfunction in isolated murine ventricular myocardia. Eur. J. Pharmacol. 2013, 706, 48–55. [Google Scholar] [CrossRef]
  102. Kanae, H.; Hamaguchi, S.; Wakasugi, Y.; Kusakabe, T.; Kato, Y.; Namekata, I.; Tanaka, H. Pathological prolongation of action potential duration as a cause of the reduced alpha-adrenoceptor-mediated negative inotropy in streptozotocin-induced diabetic mice myocardium. J. Pharmacol. Sci. 2017, 135, 131–133. [Google Scholar] [CrossRef]
  103. Arici, M.; Ferrandi, M.; Barassi, P.; Hsu, S.C.; Torre, E.; Luraghi, A.; Ronchi, C.; Chang, G.J.; Peri, F.; Ferrari, P.; et al. Istaroxime Metabolite PST3093 Selectively Stimulates SERCA2a and Reverses Disease-Induced Changes in Cardiac Function. J. Pharmacol. Exp. Ther. 2023, 384, 231–244. [Google Scholar] [CrossRef]
  104. Arici, M.; Hsu, S.C.; Ferrandi, M.; Barassi, P.; Ronchi, C.; Torre, E.; Luraghi, A.; Chang, G.J.; Ferrari, P.; Bianchi, G.; et al. Selective SERCA2a activator as a candidate for chronic heart failure therapy. J. Transl. Med. 2024, 22, 77. [Google Scholar] [CrossRef] [PubMed]
  105. Hamaguchi, S.; Abe, K.; Komatsu, M.; Kainuma, J.; Namekata, I.; Tanaka, H. Positive Lusitropic Effect of Quercetin on Isolated Ventricular Myocardia from Normal and Streptozotocin-Induced Diabetic Mice. Biol. Pharm. Bull. 2021, 44, 1894–1897. [Google Scholar] [CrossRef]
  106. Keylani, K.; Mojeni, F.A.; Khalaji, A.; Rasouli, A.; Aminzade, D.; Karimi, M.A.; Sanaye, P.M.; Khajevand, N.; Nemayandeh, N.; Poudineh, M.; et al. Endoplasmic reticulum as a target in cardiovascular diseases: Is there a role for flavonoids? Front. Pharmacol. 2023, 13, 1027633. [Google Scholar] [CrossRef]
  107. Roopnarine, O.; Yuen, S.L.; Thompson, A.R.; Roelike, L.N.; Rebbeck, R.T.; Bidwell, P.A.; Aldrich, C.C.; Cornea, R.L.; Thomas, D.D. Fluorescence lifetime FRET assay for live-cell high-throughput screening of the cardiac SERCA pump yields multiple classes of small-molecule allosteric modulators. Sci. Rep. 2023, 13, 10673. [Google Scholar] [CrossRef] [PubMed]
  108. Zhang, J.; Simpson, B.C.; Jensen, B.C. Cardiac α1A-adrenergic receptors: Emerging protective roles in cardiovascular diseases. Am. J. Physiol. Heart. Circ. Physiol. 2021, 320, H725–H733. [Google Scholar] [CrossRef] [PubMed]
  109. Cowley, P.M.; Wang, G.; Swigart, P.M.; Raghunathan, A.; Reddy, N.; Dulam, P.; Lovett, D.H.; Simpson, P.C.; Baker, A.J. Reversal of right ventricular failure by chronic α1A-subtype adrenergic agonist therapy. Am. J. Physiol. Heart Circ. Physiol. 2019, 316, H224–H232. [Google Scholar] [CrossRef]
  110. Gautam, S.; Lamichhane, S.; Sharma, N.R.; Prabal, K.C.; Basnet, A.; Kansakar, S.; Pokhrel, M.; Shetty, V.; Moskovits, N. Use of midodrine in heart failure: A review. Ann. Med. Surg. 2023, 85, 2808–2813. [Google Scholar] [CrossRef]
Jcdd 11 00267 g001
Figure 1. Action potentials of the guinea pig and mouse ventricle. Recordings were obtained in the guinea pig (A) and mouse (B) at fetal (a) neonatal (b) and adult (c) stages.
Figure 1. Action potentials of the guinea pig and mouse ventricle. Recordings were obtained in the guinea pig (A) and mouse (B) at fetal (a) neonatal (b) and adult (c) stages.
Jcdd 11 00267 g001
Jcdd 11 00267 g002
Figure 2. A schematic diagram of developmental and pathological changes in the excitation–contraction coupling of mouse ventricular cardiomyocytes. Fetus: The action potential triggers sarcolemmal Ca2+ influx through voltage-dependent Ca2+ channels, and a part of the Ca2+ diffuses towards the cell center and triggers Ca2+-induced Ca2+ release from Ca2+ release channels (ryanodine receptors) on the slightly present SR. Neonate: Partially developed T-tubular invaginations cause Ca2+-induced Ca2+ release from the coupled release channels on the SR. The released Ca2+ then triggers Ca2+ release from the neighboring Ca2+ release sites, uncoupled from the T-tubules. Adult: A well-developed T-tubular network enables simultaneous Ca2+ release from the SR in the entire cell on an action potential. Diseased: The T-tubule-SR coupling is partly disrupted and the SR Ca2+ release pattern resembles that in the immature myocardium.
Figure 2. A schematic diagram of developmental and pathological changes in the excitation–contraction coupling of mouse ventricular cardiomyocytes. Fetus: The action potential triggers sarcolemmal Ca2+ influx through voltage-dependent Ca2+ channels, and a part of the Ca2+ diffuses towards the cell center and triggers Ca2+-induced Ca2+ release from Ca2+ release channels (ryanodine receptors) on the slightly present SR. Neonate: Partially developed T-tubular invaginations cause Ca2+-induced Ca2+ release from the coupled release channels on the SR. The released Ca2+ then triggers Ca2+ release from the neighboring Ca2+ release sites, uncoupled from the T-tubules. Adult: A well-developed T-tubular network enables simultaneous Ca2+ release from the SR in the entire cell on an action potential. Diseased: The T-tubule-SR coupling is partly disrupted and the SR Ca2+ release pattern resembles that in the immature myocardium.
Jcdd 11 00267 g002
Jcdd 11 00267 g003
Figure 3. α-Adrenoceptor-mediated inotropy in the right ventricle. (A) Adult guinea pig showing positive inotropy. (B) Neonatal (a), 2-week-old (b), and 4-week-old mice (c). The inotropy changes from positive to negative during postnatal development. (C) Neonatal mice in the presence of nifedipine (a), 4-week-old mice in the presence of SEA0400 (b). The positive and negative inotropy was inhibited by nifedipine and SEA0400, respectively. Arrows indicate α-adrenergic stimulation by phenylephrine in the presence of propranolol.
Figure 3. α-Adrenoceptor-mediated inotropy in the right ventricle. (A) Adult guinea pig showing positive inotropy. (B) Neonatal (a), 2-week-old (b), and 4-week-old mice (c). The inotropy changes from positive to negative during postnatal development. (C) Neonatal mice in the presence of nifedipine (a), 4-week-old mice in the presence of SEA0400 (b). The positive and negative inotropy was inhibited by nifedipine and SEA0400, respectively. Arrows indicate α-adrenergic stimulation by phenylephrine in the presence of propranolol.
Jcdd 11 00267 g003
Table 1. Developmental changes in the excitation–contraction related parameters and the expression of excitation–contraction-related proteins of mouse ventricular cardiomyocytes.
Table 1. Developmental changes in the excitation–contraction related parameters and the expression of excitation–contraction-related proteins of mouse ventricular cardiomyocytes.
FetusNeonateAdultReferences
T-tubulenoneimmaturemature[19,23,24]
Action potential durationJcdd 11 00267 i001[15,16,19,20]
Ca2+ transient amplitudeJcdd 11 00267 i002[19]
Nifedipine sensitivity
in Ca2+ transient		Jcdd 11 00267 i003[19]
Ryanodine sensitivity
in Ca2+ transient		Jcdd 11 00267 i004[19]
α-Adrenergic inotropismpositivepositivenegative[18,25,26,27]
INaJcdd 11 00267 i005[28,29]
ItoJcdd 11 00267 i006[16,20,28]
IKJcdd 11 00267 i007[15,16,20,28]
ICa-LJcdd 11 00267 i008[28,30,31,32]
ICa-TJcdd 11 00267 i009[28,33]
RyR2Jcdd 11 00267 i010[28,30]
SERCA2Jcdd 11 00267 i011[28,30,34,35,36]
PhospholambanJcdd 11 00267 i012[28,30,34,35]
NCXJcdd 11 00267 i013[28,30,34,37]
Disclaimer/Publisher’s Note: The statements, opinions and data contained in all publications are solely those of the individual author(s) and contributor(s) and not of MDPI and/or the editor(s). MDPI and/or the editor(s) disclaim responsibility for any injury to people or property resulting from any ideas, methods, instructions or products referred to in the content.

Share and Cite

MDPI and ACS Style

Hamaguchi, S.; Agata, N.; Seki, M.; Namekata, I.; Tanaka, H. Developmental Changes in the Excitation–Contraction Mechanisms of the Ventricular Myocardium and Their Sympathetic Regulation in Small Experimental Animals. J. Cardiovasc. Dev. Dis. 2024, 11, 267. https://doi.org/10.3390/jcdd11090267

AMA Style

Hamaguchi S, Agata N, Seki M, Namekata I, Tanaka H. Developmental Changes in the Excitation–Contraction Mechanisms of the Ventricular Myocardium and Their Sympathetic Regulation in Small Experimental Animals. Journal of Cardiovascular Development and Disease. 2024; 11(9):267. https://doi.org/10.3390/jcdd11090267

Chicago/Turabian Style

Hamaguchi, Shogo, Naoki Agata, Maika Seki, Iyuki Namekata, and Hikaru Tanaka. 2024. "Developmental Changes in the Excitation–Contraction Mechanisms of the Ventricular Myocardium and Their Sympathetic Regulation in Small Experimental Animals" Journal of Cardiovascular Development and Disease 11, no. 9: 267. https://doi.org/10.3390/jcdd11090267

APA Style

Hamaguchi, S., Agata, N., Seki, M., Namekata, I., & Tanaka, H. (2024). Developmental Changes in the Excitation–Contraction Mechanisms of the Ventricular Myocardium and Their Sympathetic Regulation in Small Experimental Animals. Journal of Cardiovascular Development and Disease, 11(9), 267. https://doi.org/10.3390/jcdd11090267

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