Next Article in Journal
Prediction of Premature Termination Codon Suppressing Compounds for Treatment of Duchenne Muscular Dystrophy Using Machine Learning
Next Article in Special Issue
Influence of Membrane Phase on the Optical Properties of DPH
Previous Article in Journal
Valuing Bioactive Lipids from Green, Red and Brown Macroalgae from Aquaculture, to Foster Functionality and Biotechnological Applications
Previous Article in Special Issue
Integral Representation of Electrostatic Interactions inside a Lipid Membrane
 
 
Search for Articles:
Title / Keyword
Author / Affiliation / Email
Journal
Article Type
 
 
Advanced Search
 
Section
Special Issue
Volume
Issue
Number
Page
 
Journals
Molecules
Volume 25
Issue 17
10.3390/molecules25173885
molecules-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

Structure and Lateral Organization of Phosphatidylinositol 4,5-bisphosphate

by
Luís Borges-Araújo
1,* and
Fabio Fernandes
1,2
1
iBB—Institute for Bioengineering and Biosciences, Instituto Superior Técnico, Universidade de Lisboa, 1049-001 Lisbon, Portugal
2
Department of Bioengineering, Instituto Superior Técnico, Universidade de Lisboa, 1049-001 Lisbon, Portugal
*
Author to whom correspondence should be addressed.
Molecules 2020, 25(17), 3885; https://doi.org/10.3390/molecules25173885
Submission received: 31 July 2020 / Revised: 22 August 2020 / Accepted: 23 August 2020 / Published: 26 August 2020
(This article belongs to the Special Issue Membrane Structure and Function)
Browse Figures
Versions Notes

Abstract

:
Phosphatidylinositol 4,5-bisphosphate (PI(4,5)P2) is a minor but ubiquitous component of the inner leaflet of the plasma membrane of eukaryotic cells. However, due to its particular complex biophysical properties, it stands out from its neighboring lipids as one of the most important regulators of membrane-associated signaling events. Despite its very low steady-state concentration, PI(4,5)P2 is able to engage in a multitude of simultaneous cellular functions that are temporally and spatially regulated through the presence of localized transient pools of PI(4,5)P2 in the membrane. These pools are crucial for the recruitment, activation, and organization of signaling proteins and consequent regulation of downstream signaling. The present review showcases some of the most important PI(4,5)P2 molecular and biophysical properties as well as their impact on its membrane dynamics, lateral organization, and interactions with other biochemical partners.

Graphical Abstract

1. Introduction

The plasma membrane is a complex structure tasked with enclosing the cell and separating it from the surrounding environment. While biomembranes provide structure and define the boundaries of the cell, their dynamic biochemical and biophysical characteristics also allow them to regulate traffic and communication to and from the cytosol, organize reaction sequences, and promote cellular processes. These biophysical properties are defined not only by the intrinsic physical and chemical properties of the lipids, proteins, and other components but also by their complex set of interactions. This complexity holds the key to many key cellular processes. A lipid that stands out in the landscape of the eukaryotic plasma membrane is phosphatidylinositol 4,5-bisphosphate (PI(4,5)P2). PI(4,5)P2 is the most abundant phosphoinositide in mammalian cells and is found primarily in the inner leaflet of the plasma membrane. It has also been found in endosomes, in the endoplasmic reticulum, and in the nucleus [1]. While its role as a source of secondary messengers during signaling events is known for decades [2], evidence has accumulated through time of its importance as an intact phospholipid for defining plasma membrane identity in eukaryotic cells. Due to its very large headgroup and multivalent negative charge, PI(4,5)P2 acts almost like an electrostatic beacon, interacting specifically or non-specifically with several molecular entities such as membrane proteins, other lipids, cellular cations, etc. As a result of its particular biophysical properties, it is a major regulator of a wide spectrum of plasma membrane events, including cell adhesion and motility [3,4], ion channel transport [5,6], vesicle endocytosis [7,8,9,10,11], and exocytosis [8,12,13,14] (Figure 1).
This wide-ranging reach of PI(4,5)P2 as a critical functional lipid has made it an important research focus over the last decades in cell biology and more specifically in areas such as neuroscience, virology, and biophysics. In this review, we will focus on the physical, chemical, and structural properties of PI(4,5)P2. The impact of these properties on membrane dynamics and interactions with PI(4,5)P2 biochemical partners will also be described. We will give particular focus to PI(4,5)P2 conformation dynamics, lateral organization, and the monodisperse PI(4,5)P2–PI(4,5)P2 nanodomain duality. As mentioned above, PI(4,5)P2 is also found in the nuclear membrane, where it is thought to contribute to compartmentalization [15,16], as well as on membraneless organelles within the nucleus [15,16]. However, this review will focus on the behavior and properties of PI(4,5)P2 in the plasma membrane (PM) and PM mimicking membranes.

2. The Phosphoinositide Family

PI(4,5)P2 is a member of the phosphoinositide (PI) lipid family. PIs are a small group of glycerophospholipids derived from phosphatidylinositol. These lipids consist of a characteristic inositol headgroup, which can undergo reversible phosphorylation and dephosphorylation, leading to the formation of seven distinct phosphorylated species. While the parent lipid phosphatidylinositol represents roughly 10% of total membrane phospholipids in the eukaryotic cell, the phosphorylated derivatives account only for around 2–3% [1], with PI(4)P and PI(4,5)P2 representing the bulk of these lipids [17]. Each of these seven species has a distinct subcellular distribution with predominant localization in subsets of membranes. Additionally, within a given membrane the localization of a specific PI can be heterogeneous. Many PIs are overall in low abundance in the membrane but they can be found at high local concentrations in membrane domains not readily detected by conventional techniques [3,17]. For a historical review on inositol lipids, see Irvine (2016) [18]. Over the last couple of decades, PIs have been found to be one of the most ubiquitous signaling entities in eukaryotic metabolism. Their reach extends from controlling organelle biology to regulating cellular growth. Due to this all-encompassing reach, they have also been linked to a number of human diseases. In fact, the inositide signaling pathway is considered a promising pharmaceutical target. For an excellent review on the major developments on PI cellular biology and their impact on disease, see Balla (2013) [3].

3. PI(4,5)P2 Structure

3.1. Headgroup Conformation

The core PI(4,5)P2 structure descends from its “parent” lipid, phosphatidylinositol. At the core, it consists of a myo-inositol headgroup. There are 9 existing isomers of inositol but the myo-inositol isomer is the most commonly found in eukaryotic cells. In its most stable conformation, it assumes the chair conformation where every hydroxyl substituent is at the equatorial position except for the hydroxyl in the position 2 of the ring, which is in an axial position. The myo-inositol moiety is typically linked to the diacylglycerol (DAG) backbone via a phosphodiester bond in position 1. This leaves the hydroxyl groups in positions 2 to 6 open. However, only positions 3, 4, and 5 can be enzymatically phosphorylated to yield the 7 phosphorylated PI species. PI(4,5)P2 is the result of phosphorylation in positions 4 and 5 of the headgroup by specific kinases and phosphatases (Figure 2A).
In mammals, the majority of PI(4,5)P2 in the plasma membrane is synthesized from PI(4)P by type I phosphatidylinositol-4-phosphate 5-kinases (PIP5Ks) (α, β, and γ) [20]. Type II phosphatidylinositol 5-phosphate 4-kinase (PIP4K) (α, β, and γ) phosphorylate PI(5)P2 to synthesize a quantitatively minor pool of PI(4,5)P2 localized in the Golgi [1,21,22]. It can also be produced by the dephosphorylation of PI(3,4,5)P3 catalyzed by phosphatase and tensin homolog protein (PTEN) and phosphatidylinositol 3,4,5-trisphosphate 3-phosphatase (TPIP) (α, β, and γ) [23,24]. PI(4,5)P2 hydrolysis is controlled by specific 4’- or 5’-phosphatases or by phospholipase breakdown in response to various stimuli. Dephosphorylation by specific phosphatases (primarily 5’-phosphatases) controls PI(4,5)P2 steady-state levels and controls the extent of its signaling. Additionally, cleavage by phospholipases, such as phospholipase C (PLC), control PI(4,5)P2 levels and originate metabolites that propagate and amplify cellular signaling. PI(4,5)P2 levels, in general, are the result of a complex interplay of many cellular enzymes. While PI(4,5)P2 metabolism falls out of the scope of this review, more information can be found elsewhere [3,25].

3.2. Membrane Conformation Dynamics

In terms of molecular structure when inserted into the membrane, there are surprisingly very few experimental studies probing PI(4,5)P2 dynamics. Since the dynamics of phosphatidylinositol or of the mono-phosphorylated PI(4)P has been addressed to some extent, we can estimate some of PI(4,5)P2 properties from the behavior of these closely related precursors. At the insertion depth of phosphatidylinositol and PI(4)P, when inserted into the membrane and in the absence of any interactions with other chemical partners, it is believed that the phosphodiester bond is located roughly at the same depth as the phosphodiester of phosphatidylcholine. Additionally, evidence points out that the phosphodiester bond remains roughly parallel when compared to the membrane normal [26,27,28,29].
PI(4,5)P2 headgroup tilt seems to be significantly impacted by phosphorylation. For the case of phosphatidylinositol, the headgroup is roughly perpendicular to the membrane plane, with the C4 hydroxyl as the most exposed to the water layer despite a slight tilt being observed arising from an intramolecular hydrogen bond established between the C2 hydroxyl and the pro-R-oxygen of the phosphodiester phosphate [26,27,28,30]. This is the result of the glyceryl-phosphate-inositol link being always very close to a trans, trans, trans, gauche-conformation, which brings the two hydrogen bond partners together. Interestingly, the formation of this hydrogen bond appears to be crucial for the recognition by PLC, however, it is not yet clear if it is formed when phosphatidylinositol is aggregated [27]. In the case of PI(4)P, the headgroup tilt is more significant [26,28,29], and authors suggest it might be also due to the establishment of electrostatic interactions between the negatively charged phosphate and the positively charged choline headgroups from the neighboring lipids. For PI(4)P, due to this more significant tilt, the C5 hydroxyl is the most accessible to the water layer.
In a Variable Angle Sample Spinning NMR study [29], PI(4,5)P2 membrane conformation was studied in a membrane-like environment consisting of neutral alkyl-poly(ethylene)glycol and long-chain alcohols. All possible conformations obtained showed a much more pronounced headgroup tilt for PI(4,5)P2 than for PI(4)P, where the PI(4,5)P2 headgroup would be laying almost parallel to the membrane surface. As this cannot arise from specific electrostatic interactions in this membrane model, it is likely that this is the result of more subtle effects such as water- or alcohol-mediated hydrogen bonding. As the analysis of NMR measurements of complex systems (such as PIs) is error-prone and the “membrane matrix” used is far from being biological relevant, the authors of this study could not be definitive in their conclusions regarding PI(4,5)P2 orientation. Nevertheless, they were able to replicate what had been previously observed for PI(4)P in other membrane mimetics. If these observations are replicated in more relevant conditions, they will challenge the more established “concept” of how PI(4,5)P2 is structurally displayed in the membrane and how it interacts with protein partners. All-atom molecular dynamics simulations of PI(4,5)P2 in lipid membranes show a well-defined average head-tail angle of roughly 100°, indicating that the headgroup would lie mostly flat along the membrane in agreement with the previous studies [31] (Figure 3). Poisson Boltzmann MD simulations, however, show a more conservative tilt of roughly 40°.
Overall, there are strong hints that, in the absence of interactions with other biochemical partners, PI(4,5)P2 when inserted into a membrane has its headgroup lying tilted over the membrane, however, the extent of this tilt is still yet to be fully understood and likely depends not only on PI(4,5)P2 intrinsic properties but also on the interactions with the neighboring lipid molecules.

3.3. Headgroup Charge

An important aspect that is closely related to the conformation of PI(4,5)P2 is the charge state of each of its headgroup phosphate groups. Whilst the charge state of the headgroup linking phosphate group is well defined at physiological pH (pKa between 1 to 3) [32], the headgroup phosphate charges are much more volatile. The charge state of these groups has mostly been studied experimentally for PI(4,5)P2 in micelles and small unilamellar vesicles (SUVs), via 31P–NMR and the dependency of the chemical shift on the pH. Typically, PI(4,5)P2 is considered to have approximately four negative charges at cytosolic pH. This result was inferred from the determination of the pKa of each headgroup phosphate in either pure or mixed vesicles of PI(4,5)P2 using 31P–NMR [33]. These experiments determined a pKa value for the first protonation of roughly 6.7 and 7.7 for the phosphomonoester groups at position 4 and 5, respectively. In terms of potential charge, this would mean that at pH 7.2, the 5-phosphomonoester would be partially protonated at charge −1, the 4-phosphomonoester would be fully deprotonated with charge −2, and the phosphodiester would have charge −1.
However, studies have since shown that the PI(4,5)P2 headgroup ionization behavior (as well as for other phosphoinositides) cannot be accurately described by a Henderson-Hasselbalch mechanism [19]. In the more detailed mechanism that was proposed by the authors [19], at pH values close to 4–5, both phosphomonoester groups are mono-protonated as previously described. Upon increasing the pH, one proton dissociates, whilst the remaining one is shared between the two vicinal phosphomonoester groups (Figure 2B). In terms of potential charge this means that, at pH 7.0, the charges would be −1.58 and −1.41 for the phosphomonoester groups at positions 4 and 5, respectively. The lower charge of the 5-phosphomonoester group is attributed to the fact that it establishes a hydrogen bond interaction with the hydroxyl group in the position 6, which in turn, is also forming a long-range hydrogen bond with the phosphodiester group in the position 1. This weakens the first hydrogen bond slightly and thus the proton binds to the 5-phosphomonoester more tightly. These results gave a much more detailed look at the charge distribution of PI(4,5)P2 and at the complex network of intra- and intermolecular hydrogen bonds that lead to the dissipation of the headgroup charge and are, very likely, part of the reason for why repulsion between phosphoinositides is much weaker than expected.
A fact that is often overlooked is how the interaction of PI(4,5)P2 with neighboring molecules influences its charge distribution. In vivo, PI(4,5)P2 is constantly in interaction not only with its neighboring lipids but also with proteins and cationic ions. The complex network of interactions formed by PI(4,5)P2 with these partners leads to a greater distribution of its charge, effectively altering its headgroup charge. A study has shown that, in the absence of divalent cations, lipids with hydrogen bond donor capabilities could influence PI(4,5)P2 headgroup charge [34]. Phosphatidylethanolamine (PE) was shown to influence the first step of deprotonation of the PI(4,5)P2 headgroup, most likely by interacting preferably with the 5-phosphate. In the presence of PI, the first step of deprotonation was not affected, however, a lower degree of ionization was observed for both phosphomonoester groups for the removal of the last shared proton. Curiously, phosphatidylserine (PS) was not shown to affect PI(4,5)P2 headgroup ionization significantly. This study clearly showcases how the PI(4,5)P2 local environment can affect PI(4,5)P2 headgroup charge, a crucial feature responsible for a lot of its biological function.

3.4. Acyl-Chain Composition

The acyl-chain composition of lipids often plays an important functional role. These roles can be defined by specific interactions with proteins or by simply changing the overall biophysical properties of the surrounding membrane. In general, fatty acid profiles vary between phospholipid classes, tissues, and species and can also vary over time with dietary habits, stimuli, or disease. Like many other lipids, PI(4,5)P2 is also subject to these effects. In mammals, the phosphorylated myo-inositol headgroup is typically bound to a DAG moiety, which consists of two fatty acid chains bonded to a glycerol molecule via ester bonds at positions sn1 and sn2. The major fatty acid profile observed for PI(4,5)P2 in mammals consists of 1-stearoyl-2-arachidonyl (18:0/20:4) [23]. Curiously, inositol-phosphate headgroups coupled to ceramide have also been identified in fungi, plants, and protozoa [35], however, we will focus only on the mammal relevant DAG-bound species in this review.
The 18:0/20:4 acyl-chain profile consists of up to 70% of the total PI(4,5)P2 lipid pool in some cell lines, especially in brain tissue. This enrichment is likely the combined outcome of substrate specificity for 1-stearoyl-2-arachidonyl-glycerol in several enzymes in the phosphatidylinositol cycle and the remodeling of phosphoinositide acyl-chains via the Land’s cycle [36]. A more detailed look at how the cell might maintain this enrichment can be seen in this review by D’Souza et al. (2014) [36]. However, PI(4,5)P2 still has a broad distribution profile ranging from highly unsaturated chains to fully saturated ones [37]. These less abundant species become more prevalent in response to certain stimuli [38], stress [37,38], aging [37], or in cancer [39]. In these cases, fully saturated and mono-unsaturated compositions increase significantly in concentration, in some cases even surpassing the canonical 1-stearoyl-2-arachidonyl (18:0/20:4) composition [38].
However, why do cells spend so many resources in maintaining this particular acyl-chain composition? And why does the acyl-chain profile shift, sometimes dramatically, in specific conditions? The biological functions behind the enrichment in 18:0/20:4 are still not very clear. The enrichment in this configuration seems to be particularly prevalent in brain cells, where PI(4,5)P2 has been associated with several stages of both endocytosis and exocytosis and has been considered an important mediator of synaptic vesicle trafficking [40]. It has been shown that arachidonate, and other polyunsaturated fatty acids such as docosahexaenoate (22:6), at the sn2 position, facilitate membrane shaping and fission activities. Additionally, asymmetric sn1-saturated-sn2-polyunsaturated phospholipids have been shown to provide efficient membrane vesiculation whilst maintaining lower membrane permeability [41]. These properties might provide significant mechanical benefits in these particular tissues. Of course, arachidonic acid in particular has biological activity of its own in addition to serving as the precursor for the synthesis of eicosanoids, such as prostaglandins and leukotrienes [42]. Overall, this particular theme has been given little attention thus far, however, it could be the key for some of PI(4,5)P2 multifunctionality.

4. Lateral Organization of PI(4,5)P2

Having looked at the core structural properties of PI(4,5)P2 we now turn to its organization in the plasma membrane. As PI(4,5)P2 is engaged in a multitude of cellular functions occurring in parallel, its levels must be tightly regulated to avoid significant fluctuations of its total plasma membrane concentration. This implies that the simultaneous regulation of these cellular functions by PI(4,5)P2 must occur through the presence of multiple localized pools of this phospholipid in the plasma membrane [43]. PI(4,5)P2 lateral organization in cells has been studied through a variety of techniques from fluorescence correlation spectroscopy (FCS) and fluorescence recovery after photobleaching (FRAP) to atomic force microscopy (AFM). In FCS experiments carried out in Rat1 fibroblasts and HEK cells, researchers microinjected micelles of fluorescent labelled-PI(4,5)P2 into cells and showed that the diffusion coefficient of PI(4,5)P2 in these cells is significantly lower than expected for free phospholipids. The simplest interpretation of this result is that approximately two-thirds of PI(4,5)P2 in the inner leaflet of the plasma membrane is somehow sequestered [44]. Studies in PC12 cells have also shown, using Stimulated emission depletion (STED) microscopy [45] and Stochastic optical reconstruction microscopy (STORM) imaging techniques [46], that PI(4,5)P2 is highly enriched in nanometer-sized membrane domains, specific to this cellular model.
In fact, while the presence of segregated PI(4,5)P2 pools can be partly explained by localized PI(4,5)P2 synthesis and degradation through several kinases and phosphatases [47], it is also evident that membrane diffusion rates, in the absence of significant obstacles for diffusion, will always be higher than concentration changes due to enzymatic activity causing PI(4,5)P2 to diffuse away faster than it can be produced. This means that it is unlikely that local synthesis can result in significant changes in the submicroscopic organization of PI(4,5)P2 in the membrane [43]. PI(4,5)P2 interactions with other cellular binding partners could alternatively explain the observed lateral organization of this phosphoinositide. Interactions with proteins, divalent cations, cholesterol, and the cytoskeleton are the ones most likely to have such an impact. In this review, we will give particular attention to the often neglected effect of divalent cations on the lateral organization of PI(4,5)P2.

4.1. Sequestration by Proteins

One way to explain PI(4,5)P2 lateral organization in the plasma membrane of cells is that proteins can act as reversible buffers, binding much of the PI(4,5)P2 present and then releasing it locally in response to specific signals [48]. Theoretical simulations predict that such sequestration can be achieved not only through specific interactions with PI(4,5)P2 but also through nonspecific electrostatic interactions. In fact, polybasic proteins are able to sequester a lipid with a valence of ~4 (such as PI(4,5)P2) 1000-fold more effectively than a lipid with a valence of ~1 (such as PS) [49,50]. Due to its highly negatively charged headgroup, PI(4,5)P2 was confirmed to interact strongly with polybasic stretches of amino acid residues [43,51]. Through these polybasic stretches, several proteins were found to laterally sequester PI(4,5)P2 molecules in a reversible manner [52,53]. For an efficient buffering of PI(4,5)P2 levels, these proteins would have to be present at a concentration comparable to PI(4,5)P2, localize to the plasma membrane and be able to bind PI(4,5)P2 with high affinity while being able to release it in response to stimuli. Proteins such as myristoylated alanine-rich C-kinase substrate (MARCKS) [50,53,54], Growth Associated Protein 43 (GAP43) [48,55], CAP23 [48], among many others, have been shown to be able to sequester PI(4,5)P2 in such a manner. In the case described above of PI(4,5)P2 domains detected in PC12 cells, these were found to be associated with the sequestration of PI(4,5)P2 to clusters of the SNARE protein syntaxin-1 [45,56,57]. This sequestration by syntaxin-1 is critical for the regulation of SNARE-dependent membrane fusion [58,59].
Employing fluorescence and electron paramagnetic resonance spectroscopic tools, McLaughlin, Cafiso, and co-workers [50,52] showed that a 24 aa peptide corresponding to the effector domain of MARCKS was able to efficiently sequester an average of 3 PI(4,5)P2 molecules through non-specific electrostatic interactions. Importantly, this sequestration occurred even in the presence of physiological concentrations of the monovalent acidic phospholipid PS, confirming theoretical predictions. MARCKS sequestration of PI(4,5)P2 has been shown to be important in the PI(4,5)P2 mediated activation of TRPC-family Ca2+ channels [60], in the endocytosis of the amyloid precursor protein (APP) [61], and in the synaptic clustering of PI(4,5)P2 [62].

4.2. PI(4,5)P2 Interactions with Divalent Cations

Several studies have shown that PIs and PI(4,5)P2, in particular, are able to establish strong electrostatic interactions between their negatively charged headgroups and divalent cations. In the cellular PI(4,5)P2 context, calcium and magnesium stand out. Calcium is a common player in signal transduction and a second messenger in cells. Its levels are strictly controlled and maintained at low levels in the cytosol, with normal intracellular levels at around 100 nM (20,000 fold lower than extracellular levels) [63]. Upon stimulation, however, several signal transduction pathways can lead to transient increases of intracellular calcium concentration up to around 1 μM, with local concentrations in the vicinity of open calcium channels reaching hundreds of μM, before being regulated back to normal levels [64]. In fact, PI(4,5)P2 has been reported to be associated with a variety of Ca2+ channels and a great number of these require PI(4,5)P2 for proper function [3]. Magnesium, on the other hand, is a less studied modulator of cell function. Magnesium levels are well buffered in a narrow millimolar range between 0.25 mM and 1 mM [65,66] and are thus kept at a much higher concentration than those of calcium. Both divalent cations have been shown to bind strongly to PI(4,5)P2 and influence its lateral organization dramatically as discussed below.
Through hybrid Quantum mechanics/molecular mechanics (QM/MM) experiments we can get an insight on the molecular basis for cation binding to PI(4,5)P2 [31]. From a molecular point of view, when binding to a single PI(4,5)P2 lipid, both calcium and magnesium bind to PI(4,5)P2 either in between the phosphomonoester groups (Figure 4B) or solely near the 4-phophomonoester (Figure 4A). However, simultaneous binding between the two phosphomonoester groups is approximately 10 kcal/mol more unfavorable [31]. Divalent cation binding to the phosphodiester group has also been observed [67].
When analyzing the free energy associated with the removal of each divalent cation from its binding position, significantly more energy is required to remove calcium into the bulk water than it is for magnesium. The difference in free energy could come from the fact that, in contrast to calcium, magnesium appears to retain its first hydration shell in its equilibrium binding position. This causes its equilibrium binding position to be further away from the headgroup and leads to the formation of fewer hydrogen bonds, on average, between the headgroup and the surrounding water molecules. Interestingly, it was also shown that upon binding to calcium, the remaining PI(4,5)P2 headgroup proton at physiological pH could be favorably displaced and that the effective size of the PI(4,5)P2 headgroup would significantly decrease [31]. In the presence of magnesium, the dissociation of the remaining proton was not favorable, however, the decrease in effective headgroup surface area was also observed albeit to a lesser extent. All of these cation-induced changes can and will affect PI(4,5)P2 dynamics, thus influencing local membrane dynamics as well as its interactions with protein binding partners.
Apart from simply binding to PI(4,5)P2, both divalent cations also have the ability to crosslink PI(4,5)P2 lipids. This induces the formation of very stable cation-induced PI(4,5)P2 nanodomains. It has been shown through different experimental techniques that divalent cations, and especially calcium, are able to induce the formation of PI(4,5)P2 nanodomains, even at physiological concentrations of cation and lipid. In lipid monolayers, these clusters can be detected through AFM [68,69] (Figure 5). Through the use of fluorescent analogs of PI(4,5)P2 , calcium-induced clusters were shown to occur in model membranes at physiologically relevant concentrations of both calcium and PI(4,5)P2 [70]. Other phosphoinositides have also shown some propensity to form cation-induced clusters. PI(3,5)P2 has been found to form nanodomains by itself in the presence of physiological concentrations of calcium cations, however, in the presence of magnesium clustering was negligible [71]. On top of that, the clusters formed by PI(3,5)P2 were much smaller and likely less stable than those formed by PI(4,5)P2 [71]. On the other hand, when the monophosphorylated PI(4)P was tested in the same type of experiments, no calcium-induced clusters were observed [71].
From a molecular point of view, a single divalent cation can likely crosslink up to 2 PI(4,5)P2 lipids by simultaneously binding each lipid phosphodiester and/or headgroup phosphomonoester groups via strong electrostatic interactions [72]. A single PI(4,5)P2 lipid, however, can simultaneously bind up to 3 divalent cations, and thus be complexed with 3 other PI(4,5)P2 lipids (Figure 6). This net of PI(4,5)P2—cation interactions can thus induce the formation of a grid of tightly crosslinked lipids. Whilst the main driving force behind the clustering appears to be cation crosslinking, the formation of a complex network of intermolecular hydrogen bonds, between the headgroup hydroxyl and phosphomonoester groups, very likely plays a role in thermodynamically favoring clustering. Due to the electrostatic nature of the cation interactions, the propensity to crosslink PI(4,5)P2 lipids appears to be highly correlated with the affinity towards the divalent cation. Thus, Ca2+ shows a much greater clustering propensity than magnesium. In fact, Ca2+ induced clusters have been shown to be significantly larger than those induced by magnesium at the same experimental conditions [68]. However, although magnesium has a much weaker affinity for PI(4,5)P2 when compared to calcium, its steady-state levels are several orders of magnitude higher than those of calcium, and at these mM concentrations, it is also able to induce comparable PI(4,5)P2 clustering [71].
As the formation of these clusters is driven mainly by the crosslinking of the phosphate groups, the nanodomains formed are composed of almost only PI(4,5)P2. Studies have shown that other phosphorylated PI species can co-cluster with PI(4,5)P2, albeit to a lesser degree, but that the parent lipid phosphatidylinositol cannot [73]. Incorporation into clusters also seems to be independent from acyl-chain composition [73], however, it is very likely that different acyl-chain compositions induce the formation of nanodomains with different biophysical properties.
These cation-induced PI(4,5)P2 nanodomains are much more than simply the sum of their elements. While calcium is known to directly regulate the interaction of different protein domains to PI(4,5)P2 [74], the structure and dynamics of the phospholipid within the divalent cation-induced cluster present markedly distinct biophysical characteristics than the monodisperse lipid. As mentioned previously, binding of divalent cations, and in particular calcium, can alter PI(4,5)P2 headgroup exposure leading to a decrease in solvent-accessible area [31]. Additionally, as divalent cations accumulate, significant screening of the headgroup charges occurs, essentially shielding the large negatively charged headgroup from potential binding partners [75]. As PI(4,5)P2 lipids are forced to accumulate in an enclosed area, further reorganization of the headgroups occurs, promoted by the molecular interactions of the divalent cations with the 3 phosphate groups [76], effectively altering the headgroup conformation. This local accumulation likely influences PI(4,5)P2 acyl-chain dynamics and, therefore, local membrane order. Studies have shown that PI(4,5)P2 nanodomains have significantly reduced lateral dynamics [70] and that PI(4,5)P2, which as a single lipid has a strong preference for disordered domains, displays significantly less affinity for disordered domains upon clustering [71]. All of these altered biophysical properties can, and most likely will, influence downstream PI(4,5)P2 signaling by modulating its interactions with protein and lipid partners.
Altogether, these findings show that divalent cation-mediated clustering can lead to the formation of specific sites in the membrane highly enriched in PI(4,5)P2 while depleting the rest of the membrane [70]. PI(4,5)P2 is likely constitutively clustered in the membrane, crosslinked by Mg2+ ions alongside other minor phosphoinositide lipids. In the vicinity of active calcium channels, where calcium concentrations increase significantly upon opening of a channel, both ions will simultaneously contribute to the formation of the nanodomains, to form larger and more stable PI(4,5)P2 nanodomains. These cation-induced nanodomains can influence not only PI(4,5)P2 lateral organization and biophysical properties but also the way proteins interact with PI(4,5)P2, by modulating their localization in the plasma membrane, their target recognition and binding affinity to PI(4,5)P2, and even further downstream interactions with other proteins. Therefore, beyond the impact of calcium on PI(4,5)P2 levels in the membrane through activation of phospholipase activity, the direct interaction of divalent cations with PI(4,5)P2 is expected to play a crucial role in the regulation of the biological activity of this phospholipid.

4.3. Effect of Cholesterol on PI(4,5)P2 Properties and Distribution

Cholesterol is a crucial membrane component, implicated in a myriad of membrane processes. However, its most noted role is in the regulation of plasma membrane biophysical properties as a “fluidity buffer”. Whilst its effects can vary with different cholesterol contents, cholesterol, in general, decreases membrane fluidity by increasing lipid packing even leading to the cholesterol-dependent formation of coexisting liquid phases [77]. Like all the other phospholipids in the plasma membrane, PI(4,5)P2 is also subject to these cholesterol-dependent effects.
Unsurprisingly, given its large negatively charged headgroup and highly unsaturated acyl chain, PI(4,5)P2 was shown to preferentially partition into the less ordered cholesterol-poor phases of biphasic monolayers containing PI(4,5)P2:SOPC:Chol [78]. However, after the addition of calcium, the subsequent cation-induced PI(4,5)P2 nanodomains were shown to have increased the miscibility of the coexisting domains in the cholesterol-containing monolayers [78]. Related results have been observed, in a study with fluorescent derivatives of PI(4,5)P2 incorporated in ternary mixtures of POPC:SM:Chol. In this study, monodisperse PI(4,5)P2 presented low miscibility in more ordered lipid phases, yet, after cation-induced clustering, the preference for disordered domains decreased by more than two-fold [78]. Importantly, the lipid composition of this ternary mixture was shown to have a marked influence both on the extent of PI(4,5)P2 calcium-induced clustering and on the size of clusters formed (Figure 7) [78]. Since the dimensions of PI(4,5)P2 clusters were heavily dependent on temperature, it was concluded that the major factor regulating PI(4,5)P2 clustering was membrane order and not the presence of a specific molecular partner in the membrane. This suggests that the insertion of PI(4,5)P2 in more ordered domains is stabilized by the formation of cation-induced nanodomains. In a cellular context, the effect of cholesterol on PI(4,5)P2 appears to be heavily dependent on cell type. In fibroblasts [79] and cultured pancreatic β-cells [80], cholesterol depletion leads to decreased levels of free PI(4,5)P2, whilst in HEK293 [81] cholesterol enrichment was shown to promote PI(4,5)P2 depletion.
Altogether, the findings we have previously discussed appear to be in agreement with theories that associate PI(4,5)P2 with the controversial cholesterol-rich microdomains, such as “lipid rafts” and caveolae, which are said to be involved in regulating a variety of membrane functions. PI(4,5)P2 has been found to be enriched in detergent-resistant membranes [82]. Moreover, while detergent extraction has been put into question on whether it induces an artefactual enrichment in PI(4,5)P2 [83], studies have shown PI(4,5)P2 to colocalize with more ordered membrane domains [84,85,86,87] and to be sensitive to membrane curvature [87,88], both associated with these types of structures. Interestingly, in a study where a PI(4,5)P2-specific phosphatase was targeted to either the “raft” or the “nonraft” membrane fractions of T cells, the authors were able to show clear evidence of compartmentalization of PI(4,5)P2-dependent signaling in each of the fractions. When depleting the “nonraft” fraction of PI(4,5)P2, T cells showed an increase in cell filopodia and cell spreading, whilst in contrast, when depleting the “raft” fraction of PI(4,5)P2, T cells showed smooth membranes free of ruffling and filopodia among other effects. Findings also appear to suggest that roughly half of the PI(4,5)P2 content is synthesized preferentially in these cholesterol-enriched domains [82]. Nonetheless, this is still an area of great controversy amongst researchers, and there is a lot yet to uncover before significant conclusions can be drawn on the importance of these microdomains for PI(4,5)P2 lateral organization.

4.4. Effect of the Cytoskeleton and Curvature on PI(4,5)P2 Lateral Organization

PI(4,5)P2 has been shown to be a major player in cytoskeleton dynamics, by interacting and regulating the activity of numerous enzymes and cytoskeletal proteins [89,90]. However, the cytoskeleton can also regulate PI(4,5)P2, and in particular its lateral organization, via corralling by the cortical actin network. Cortical actin networks have been shown to be able to induce spatio-temporal confinement of phospholipids in the plasma membrane of living cells [91]. PI(4,5)P2 should be no exception to this effect and, in fact, due to its close proximity with a variety of actin-binding proteins [90], one can suspect it could be even more susceptible to these effects. Studies have shown that the cytoskeleton is responsible for some of the low mobility of PI(4,5)P2 in atrial myocytes [92].
Curvature can also greatly influence PI(4,5)P2 lateral organization. PI(4,5)P2 has been found to undergo a transient increase at the phagocytic cup during the initiation of phagocytosis [93,94]. More recently, it was found that the curvature induced by the engagement of non-biological solid particles with the plasma membrane was enough to increase PI(4,5)P2 concentrations at the site of contact. Additionally, as we previously discussed, PI(4,5)P2 has been associated with several stages of endocytosis and exocytosis, where curvature effects are paramount [40]. As a monodisperse lipid, PI(4,5)P2 has an inverted cone-shaped structure [95] due to its very large inositol headgroup. As such, it is associated with positive membrane curvature. After interacting with divalent cations, however, PI(4,5)P2 presents a cone-shaped structure [95], likely due to the decrease in headgroup area as well as the aggregation of the headgroups after complexation with the cations. In this case, it would be associated with negative membrane curvature. Whether local curvature at the plasma membrane plays a major role in dictating PI(4,5)P2 lateral organization or PI(4,5)P2 lateral organization contributes to local curvature is not entirely clear. In a cellular context, it is likely dependent on the process in question and the overall result of both effects.

5. Concluding Remarks

Despite having been discussed separately in this review, all the complex biophysical properties we discussed previously are tightly interlinked processes. Furthermore, it is the combined effect of these properties that allows PI(4,5)P2 to be a major regulator of membrane dynamics despite being present at very low overall concentrations. While a lot of research has been conducted on these effects, many are still to be fully characterized, especially those associated with cation-induced nanodomains, such as the lipid conformation in these structures, the extent of charge dissipation, and the effect of these nanodomains on the local bilayer properties. A good molecular understanding of these effects is fundamental in order to better understand how PI(4,5)P2 carries out its role as a major plasma membrane regulator.
Over the last decades, extensive research efforts have uncovered a multitude of different cellular roles of PI(4,5)P2. However, the current view on the majority of the mechanisms associated with these functions neglects the almost certain presence of a highly significant, if not dominant, pool of this phospholipid that is not monodispersed. Special consideration should be given to the fact that in the plasma membrane, PI(4,5)P2 must be either protein-bound or constitutively complexed with divalent cations within small clusters. PI(4,5)P2 within these structures is bound to have significantly different properties from the monodisperse lipid. These properties can influence PI(4,5)P2 interactions with its binding partners (such as proteins) as well as downstream protein-protein interactions. It is conceivable that many of PI(4,5)P2 cellular functions are also regulated by the extent of this effect.

Funding

L.B.A. thanks to The Medical Biochemistry and Biophysics Doctoral Programme (M2B-PhD) and the Portuguese Science and Technology Foundation (FCT) for a PhD fellowship (PD/BD/137492/2018). Authors acknowledge funding by FCT project reference IF/00386/2015/CP1272/CT0010 and PTDC/BTM-SAL/31057/2017.

Conflicts of Interest

The authors declare no conflict of interest. The funders had no role in the writing of the manuscript.

References

  1. Viaud, J.; Mansour, R.; Antkowiak, A.; Mujalli, A.; Valet, C.; Chicanne, G.; Xuereb, J.M.; Terrisse, A.D.; Séverin, S.; Gratacap, M.P.; et al. Phosphoinositides: Important lipids in the coordination of cell dynamics. Biochimie 2016, 125, 250–258. [Google Scholar] [CrossRef]
  2. Berridge, M.J. Inositol Trisphosphate and Diacylglycerol: Two Interacting Second Messengers. Annu. Rev. Biochem. 1987, 56, 159–193. [Google Scholar] [CrossRef] [PubMed]
  3. Ballac, T. Phosphoinositides: Tiny lipids with giant impact on cell regulation. Physiol. Rev. 2013, 93, 1019–1137. [Google Scholar] [CrossRef] [PubMed]
  4. Tsujita, K.; Itoh, T. Phosphoinositides in the regulation of actin cortex and cell migration. Biochim. Biophys. Acta Mol. Cell Biol. Lipids 2015, 1851, 824–831. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  5. Hilgemann, D.W.; Feng, S.; Nasuhoglu, C. The complex and intriguing lives of PIP2 with ion channels and transporters. Sci. STKE 2001, 2001, re19. [Google Scholar] [CrossRef]
  6. Hille, B.; Dickson, E.J.; Kruse, M.; Vivas, O.; Suh, B.C. Phosphoinositides regulate ion channels. Biochim. Biophys. Acta 2015, 1851, 844–856. [Google Scholar] [CrossRef]
  7. Höning, S.; Ricotta, D.; Krauss, M.; Späte, K.; Spolaore, B.; Motley, A.; Robinson, M.; Robinson, C.; Haucke, V.; Owen, D.J. Phosphatidylinositol-(4,5)-Bisphosphate Regulates Sorting Signal Recognition by the Clathrin-Associated Adaptor Complex AP2. Mol. Cell 2005, 18, 519–531. [Google Scholar] [CrossRef] [Green Version]
  8. Wenk, M.R.; De Camilli, P. Protein-lipid interactions and phosphoinositide metabolism in membrane traffic: Insights from vesicle recycling in nerve terminals. Proc. Natl. Acad. Sci. USA 2004, 101, 8262–8269. [Google Scholar] [CrossRef] [Green Version]
  9. Simonsen, A.; Wurmser, A.E.; Emr, S.D.; Stenmark, H. The role of phosphoinositides in membrane transport. Curr. Opin. Cell Biol. 2001, 13, 485–492. [Google Scholar] [CrossRef]
  10. Posor, Y.; Eichhorn-Grünig, M.; Haucke, V. Phosphoinositides in endocytosis. Biochim. Biophys. Acta 2015, 1851, 794–804. [Google Scholar] [CrossRef]
  11. Levin, R.; Grinstein, S.; Schlam, D. Phosphoinositides in phagocytosis and macropinocytosis. Biochim. Biophys. Acta Mol. Cell Biol. Lipids 2015, 1851, 805–823. [Google Scholar] [CrossRef] [PubMed]
  12. Holz, R.W.; Hlubek, M.D.; Sorensen, S.D.; Fisher, S.K.; Balla, T.; Ozaki, S.; Prestwich, G.D.; Stuenkel, E.L.; Bittner, M.A. A pleckstrin homology domain specific for phosphatidylinositol 4,5-bisphosphate (PtdIns-4,5-P 2) and fused to green fluorescent protein identifies plasma membrane PtdIns-4,5-P 2 as being important in exocytosis. J. Biol. Chem. 2000, 275, 17878–17885. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  13. Martin, T.F. PI(4,5)P(2) regulation of surface membrane traffic. Curr. Opin. Cell Biol. 2001, 13, 493–499. [Google Scholar] [CrossRef]
  14. Martin, T.F.J. PI(4,5)P2-binding effector proteins for vesicle exocytosis. Biochim. Biophys. Acta Mol. Cell Biol. Lipids 2015, 1851, 785–793. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  15. Sztacho, M.; Sobol, M.; Balaban, C.; Escudeiro Lopes, S.E.; Hozák, P. Nuclear phosphoinositides and phase separation: Important players in nuclear compartmentalization. Adv. Biol. Regul. 2019, 71, 111–117. [Google Scholar] [CrossRef] [PubMed]
  16. Fiume, R.; Faenza, I.; Sheth, B.; Poli, A.; Vidalle, M.C.; Mazzetti, C.; Abdul, S.H.; Campagnoli, F.; Fabbrini, M.; Kimber, S.T.; et al. Nuclear Phosphoinositides: Their Regulation and Roles in Nuclear Functions. Int. J. Mol. Sci. 2019, 20, 2991. [Google Scholar] [CrossRef] [Green Version]
  17. Di Paolo, G.; De Camilli, P. Phosphoinositides in cell regulation and membrane dynamics. Nature 2006, 443, 651–657. [Google Scholar] [CrossRef]
  18. Irvine, R.F. Thematic review series: Living history of lipids: A short history of inositol lipids. J. Lipid Res. 2016, 57, 1987–1994. [Google Scholar] [CrossRef] [Green Version]
  19. Kooijman, E.E.E.; King, K.E.E.; Gangoda, M.; Gericke, A. Ionization properties of phosphatidylinositol polyphosphates in mixed model membranes. Biochemistry 2009, 48, 9360–9371. [Google Scholar] [CrossRef]
  20. Ishihara, H.; Shibasaki, Y.; Kizuki, N.; Wada, T.; Yazaki, Y.; Asano, T.; Oka, Y. Type I phosphatidylinositol-4-phosphate 5-kinases. Cloning of the third isoform and deletion/substitution analysis of members of this novel lipid kinase family. J. Biol. Chem. 1998, 273, 8741–8748. [Google Scholar] [CrossRef] [Green Version]
  21. Clarke, J.H.; Emson, P.C.; Irvine, R.F. Localization of phosphatidylinositol phosphate kinase IIgamma in kidney to a membrane trafficking compartment within specialized cells of the nephron. Am. J. Physiol. Renal Physiol. 2008, 295, F1422–F1430. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  22. Bunce, M.W.; Boronenkov, I.V.; Anderson, R.A. Coordinated activation of the nuclear ubiquitin ligase Cul3-SPOP by the generation of phosphatidylinositol 5-phosphate. J. Biol. Chem. 2008, 283, 8678–8686. [Google Scholar] [CrossRef] [Green Version]
  23. De Craene, J.-O.; Bertazzi, D.; Bär, S.; Friant, S. Phosphoinositides, Major Actors in Membrane Trafficking and Lipid Signaling Pathways. Int. J. Mol. Sci. 2017, 18, 634. [Google Scholar] [CrossRef] [PubMed]
  24. Liu, Y.; Bankaitis, V.A. Progress in Lipid Research Phosphoinositide phosphatases in cell biology and disease. Prog. Lipid Res. 2010, 49, 201–217. [Google Scholar] [CrossRef] [Green Version]
  25. Dickson, E.J.; Hille, B. Understanding phosphoinositides: Rare, dynamic, and essential membrane phospholipids. Biochem. J. 2019, 476, 1–23. [Google Scholar] [CrossRef] [PubMed]
  26. Bradshaw, J.P.; Bushby, R.J.; Giles, C.C.; Saunders, M.R.; Saxena, A. The headgroup orientation of dimyristoylphosphatidylinositol-4-phosphate in mixed lipid bilayers: A neutron diffraction study. Biochim. Biophys. Acta Biomembr. 1997, 1329, 124–138. [Google Scholar] [CrossRef] [Green Version]
  27. Zhou, C.; Garigapati, V.; Roberts, M.F. Short-chain phosphatidylinositol conformation and its relevance to phosphatidylinositol-specific phospholipase C. Biochemistry 1997, 36, 15925–15931. [Google Scholar] [CrossRef]
  28. Bradshaw, J.P.; Bushby, R.J.; Giles, C.C.; Saunders, M.R. Orientation of the headgroup of phosphatidylinositol in a model biomembrane as determined by neutron diffraction. Biochemistry 1999, 38, 8393–8401. [Google Scholar] [CrossRef]
  29. Kishore, A.I.; Prestegard, J.H. Molecular Orientation and Conformation of Phosphatidylinositides in Membrane Mimetics Using Variable Angle Sample Spinning (VASS) NMR. Biophys. J. 2003, 85, 3848–3857. [Google Scholar] [CrossRef] [Green Version]
  30. Hansbro, P.M.; Byard, S.J.; Bushby, R.J.; Turnbull, P.J.; Boden, N.; Saunders, M.R.; Novelli, R.; Reid, D.G. The conformational behaviour of phosphatidylinositol in model membranes: 2H-NMR studies. Biochim. Biophys. Acta 1992, 1112, 187–196. [Google Scholar] [CrossRef]
  31. Slochower, D.R.; Huwe, P.J.; Radhakrishnan, R.; Janmey, P.A. Quantum and all-atom molecular dynamics simulations of protonation and divalent ion binding to phosphatidylinositol 4,5-bisphosphate (PIP 2 ). J. Phys. Chem. B 2013, 117, 8322–8329. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  32. Brown, W.H. Organic Chemistry; Brooks/Cole Cengage Learning: Boston, MA, USA, 2009; ISBN 0495388572. [Google Scholar]
  33. van Paridon, P.A.; de Kruijff, B.; Ouwerkerk, R.; Wirtz, K.W.A. Polyphosphoinositides undergo charge neutralization in the physiological pH range: A 31P-NMR study. Biochim. Biophys. Acta BBA Lipids Lipid Metab. 1986, 877, 216–219. [Google Scholar] [CrossRef]
  34. Graber, Z.T.T.; Jiang, Z.; Gericke, A.; Kooijman, E.E.E. Phosphatidylinositol-4,5-bisphosphate ionization and domain formation in the presence of lipids with hydrogen bond donor capabilities. Chem. Phys. Lipids 2012, 165, 696–704. [Google Scholar] [CrossRef] [PubMed]
  35. Björkbom, A.; Ohvo-Rekilä, H.; Kankaanpää, P.; Nyholm, T.K.M.; Westerlund, B.; Slotte, J.P. Characterization of membrane properties of inositol phosphorylceramide. Biochim. Biophys. Acta Biomembr. 2010, 1798, 453–460. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  36. D’Souza, K.; Epand, R.M. Enrichment of phosphatidylinositols with specific acyl chains. Biochim. Biophys. Acta Biomembr. 2014, 1838, 1501–1508. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  37. Traynor-Kaplan, A.; Kruse, M.; Dickson, E.J.; Dai, G.; Vivas, O.; Yu, H.; Whittington, D.; Hille, B. Fatty-acyl chain profiles of cellular phosphoinositides. Biochim. Biophys. Acta 2017, 1862, 513–522. [Google Scholar] [CrossRef] [Green Version]
  38. Mujalli, A.; Chicanne, G.; Bertrand-Michel, J.; Viars, F.; Stephens, L.; Hawkins, P.; Viaud, J.; Gaits-Iacovoni, F.; Severin, S.; Gratacap, M.P.; et al. Profiling of phosphoinositide molecular species in human and mouse platelets identifies new species increasing following stimulation. Biochim. Biophys. Acta 2018, 1863, 1121–1131. [Google Scholar] [CrossRef]
  39. Koizumi, A.; Narita, S.; Nakanishi, H.; Ishikawa, M.; Eguchi, S.; Kimura, H.; Takasuga, S.; Huang, M.; Inoue, T.; Sasaki, J.; et al. Increased fatty acyl saturation of phosphatidylinositol phosphates in prostate cancer progression. Sci. Rep. 2019, 9, 13257–13258. [Google Scholar] [CrossRef] [Green Version]
  40. Koch, M.; Holt, M. Coupling exo- and endocytosis: An essential role for PIP 2 at the synapse. Biochim. Biophys. Acta Mol. Cell Biol. Lipids 2012, 1821, 1114–1132. [Google Scholar] [CrossRef]
  41. Manni, M.M.; Tiberti, M.L.; Pagnotta, S.; Barelli, H.; Gautier, R.; Antonny, B. Acyl chain asymmetry and polyunsaturation of brain phospholipids facilitate membrane vesiculation without leakage. Elife 2018, 7, e34394. [Google Scholar] [CrossRef]
  42. Nelson, D.L.; Cox, M.M. Lehninger Principles of Biochemistry Sixth Edition, 6th ed.; Macmillan Learning: London, UK, 2013. [Google Scholar]
  43. Mclaughlin, S.; Wang, J.; Gambhir, A.; Murray, D. Pip(2) and Proteins: Interactions, Organization, and Information Flow. Annu. Rev. Biophy. Biomol. Struct. 2002, 31, 171–175. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  44. Golebiewska, U.; Nyako, M.; Woturski, W.; Zaitseva, I.; McLaughlin, S. Diffusion coefficient of fluorescent phosphatidylinositol 4,5-bisphosphate in the plasma membrane of cells. Mol. Biol. Cell 2008, 19, 1663–1669. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  45. van den Bogaart, G.; Meyenberg, K.; Risselada, H.J.; Amin, H.; Willig, K.I.; Hubrich, B.E.; Dier, M.; Hell, S.W.; Grubmüller, H.; Diederichsen, U.; et al. Membrane protein sequestering by ionic protein–lipid interactions. Nature 2011, 479, 552–555. [Google Scholar] [CrossRef]
  46. Wang, J.; Richards, D.A. Segregation of PIP2 and PIP3 into distinct nanoscale regions within the plasma membrane. Biol. Open 2012, 1, 857–862. [Google Scholar] [CrossRef] [Green Version]
  47. Payrastre, B.; Missy, K.; Giuriato, S.; Bodin, S.; Plantavid, M.; Gratacap, M. Phosphoinositides: Key players in cell signalling, in time and space. Cell. Signal. 2001, 13, 377–387. [Google Scholar] [CrossRef]
  48. Laux, T.; Fukami, K.; Thelen, M.; Golub, T.; Frey, D.; Caroni, P. Gap43, Marcks, and Cap23 modulate Pi(4,5)p2 at mlasmalemmal rafts, and regulate cell cortex actin dynamics through a common mechanism. J. Cell Biol. 2000, 149, 1455–1472. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  49. Wang, J.; Gambhir, A.; McLaughlin, S.; Murray, D. A Computational Model for the Electrostatic Sequestration of PI(4,5)P2 by Membrane-Adsorbed Basic Peptides. Biophys. J. 2004, 86, 1969–1986. [Google Scholar] [CrossRef] [Green Version]
  50. Gambhir, A.; Hangyás-Mihályné, G.; Zaitseva, I.; Cafiso, D.S.; Wang, J.; Murray, D.; Pentyala, S.N.; Smith, S.O.; McLaughlin, S. Electrostatic sequestration of PIP2 on phospholipid membranes by basic/aromatic regions of proteins. Biophys. J. 2004, 86, 2188–2207. [Google Scholar] [CrossRef] [Green Version]
  51. McLaughlin, S.; Murray, D. Plasma membrane phosphoinositide organization by protein electrostatics. Nature 2005, 438, 605–611. [Google Scholar] [CrossRef]
  52. Rauch, M.E.; Ferguson, C.G.; Prestwich, G.D.; Cafiso, D.S. Myristoylated alanine-rich C kinase substrate (MARCKS) sequesters spin-labeled phosphatidylinositol 4,5-bisphosphate in lipid bilayers. J. Biol. Chem. 2002, 277, 14068–14076. [Google Scholar] [CrossRef] [Green Version]
  53. Wang, J.; Gambhir, A.; Hangyás-Mihályné, G.; Murray, D.; Golebiewska, U.; McLaughlin, S. Lateral sequestration of phosphatidylinositol 4,5-bisphosphate by the basic effector domain of myristoylated alanine-rich C kinase substrate is due to nonspecific electrostatic interactions. J. Biol. Chem. 2002, 277, 34401–34412. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  54. Dietrich, U.; Krüger, P.; Gutberlet, T.; Käs, J.A. Interaction of the MARCKS peptide with PIP2 in phospholipid monolayers. Biochim. Biophys. Acta Biomembr. 2009, 1788, 1474–1481. [Google Scholar] [CrossRef] [PubMed]
  55. Tong, J.; Nguyen, L.; Vidal, A.; Simon, S.A.; Skene, J.H.P.; McIntosh, T.J. Role of GAP-43 in sequestering phosphatidylinositol 4,5-bisphosphate to Raft bilayers. Biophys. J. 2008, 94, 125–133. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  56. Aoyagi, K.; Sugaya, T.; Umeda, M.; Yamamoto, S.; Terakawa, S.; Takahashi, M. The activation of exocytotic sites by the formation of phosphatidylinositol 4,5-bisphosphate microdomains at syntaxin clusters. J. Biol. Chem. 2005, 280, 17346–17352. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  57. Murray, D.H.; Tamm, L.K. Clustering of syntaxin-1A in model membranes is modulated by phosphatidylinositol 4,5-bisphosphate and cholesterol. Biochemistry 2009, 48, 4617–4625. [Google Scholar] [CrossRef] [Green Version]
  58. James, D.J.; Khodthong, C.; Kowalchyk, J.A.; Martin, T.F.J. Phosphatidylinositol 4,5-bisphosphate regulates SNARE-dependent membrane fusion. J. Cell Biol. 2008, 182, 355–366. [Google Scholar] [CrossRef] [Green Version]
  59. Milosevic, I.; Sørensen, J.B.; Lang, T.; Krauss, M.; Nagy, G.; Haucke, V.; Jahn, R.; Neher, E. Plasmalemmal phosphatidylinositol-4,5-bisphosphate level regulates the releasable vesicle pool size in chromaffin cells. J. Neurosci. 2005, 25, 2557–2565. [Google Scholar] [CrossRef]
  60. Shi, J.; Birnbaumer, L.; Large, W.A.; Albert, A.P. Myristoylated alanine-rich C kinase substrate coordinates native TRPC1 channel activation by phosphatidylinositol 4,5-bisphosphate and protein kinase C in vascular smooth muscle. FASEB J. 2014, 28, 244–255. [Google Scholar] [CrossRef] [Green Version]
  61. Su, R.; Han, Z.-Y.; Fan, J.-P.; Zhang, Y.-L. A possible role of myristoylated alanine-rich C kinase substrate in endocytic pathway of Alzheimer’s disease. Neurosci. Bull. 2010, 26, 338–344. [Google Scholar] [CrossRef] [Green Version]
  62. Trovò, L.; Ahmed, T.; Callaerts-Vegh, Z.; Buzzi, A.; Bagni, C.; Chuah, M.; VandenDriessche, T.; Balschun, D.; Dotti, C.G. Low hippocampal PI(4,5)P2 contributes to reduced cognition in old mice as a result of loss of MARCKS. Nat. Publ. Gr. 2013, 16, 449–455. [Google Scholar] [CrossRef]
  63. Clapham, D.E. Calcium signaling. Cell 1995, 80, 259–268. [Google Scholar] [CrossRef] [Green Version]
  64. Berridge, M.J. Calcium microdomains: Organization and function. Cell Calcium 2006, 40, 405–412. [Google Scholar] [CrossRef] [PubMed]
  65. Grubbs, R.D. Intracellular magnesium and magnesium buffering. BioMetals 2002, 15, 251–259. [Google Scholar] [CrossRef] [PubMed]
  66. Trapani, V.; Farruggia, G.; Marraccini, C.; Iotti, S.; Cittadini, A.; Wolf, F.I. Intracellular magnesium detection: Imaging a brighter future. Analyst 2010, 135, 1855–1866. [Google Scholar] [CrossRef] [PubMed]
  67. Slochower, D.R.; Wang, Y.-H.; Radhakrishnan, R.; Janmey, P.A. Physical chemistry and membrane properties of two phosphatidylinositol bisphosphate isomers. Phys. Chem. Chem. Phys. 2015, 17, 12608–12615. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  68. Wang, Y.-H.; Collins, A.; Guo, L.; Smith-Dupont, K.B.; Gai, F.; Svitkina, T.; Janmey, P.A. Divalent cation-induced cluster formation by polyphosphoinositides in model membranes. J. Am. Chem. Soc. 2012, 134, 3387–3395. [Google Scholar] [CrossRef] [Green Version]
  69. Ellenbroek, W.G.; Wang, Y.H.; Christian, D.A.; Discher, D.E.; Janmey, P.A.; Liu, A.J. Divalent cation-dependent formation of electrostatic PIP2 clusters in lipid monolayers. Biophys. J. 2011, 101, 2178–2184. [Google Scholar] [CrossRef] [Green Version]
  70. Sarmento, M.J.; Coutinho, A.; Fedorov, A.; Prieto, M.; Fernandes, F. Ca2 + induces PI(4,5)P2 clusters on lipid bilayers at physiological PI(4,5)P2 and Ca2 + concentrations. Biochim. Biophys. Acta Biomembr. 2014, 1838, 822–830. [Google Scholar] [CrossRef] [Green Version]
  71. Sarmento, M.J.; Coutinho, A.; Fedorov, A.; Prieto, M.; Fernandes, F. Membrane Order Is a Key Regulator of Divalent Cation-Induced Clustering of PI(3,5)P2 and PI(4,5)P2. Langmuir 2017, 33, 12463–12477. [Google Scholar] [CrossRef]
  72. Cohen, J.A.; Cohen, M. Adsorption of monovalent and divalent cations by phospholipid membranes. The monomer-dimer problem. Biophys. J. 1981, 36, 623–651. [Google Scholar] [CrossRef] [Green Version]
  73. Wen, Y.; Vogt, V.M.; Feigenson, G.W. Multivalent Cation-Bridged PI(4,5)P2 Clusters Form at Very Low Concentrations. Biophys. J. 2018, 114, 2630–2639. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  74. Monteiro, M.E.; Sarmento, M.J.; Fernandes, F. Role of calcium in membrane interactions by PI(4,5)P2-binding proteins. Biochem. Soc. Trans. 2014, 42, 1441–1446. [Google Scholar] [CrossRef] [PubMed]
  75. Seo, J.B.; Jung, S.R.; Huang, W.; Zhang, Q.; Koh, D.S. Charge shielding of PIP2 by cations regulates enzyme activity of phospholipase C. PLoS ONE 2015, 10, 1–22. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  76. Bilkova, E.; Pleskot, R.; Rissanen, S.; Sun, S.; Czogalla, A.; Cwiklik, L.; Rog, T.; Vattulainen, I.; Cremer, P.S.; Jungwirth, P.; et al. Calcium directly regulates phosphatidylinositol 4,5-bisphosphate headgroup conformation and recognition. J. Am. Chem. Soc. 2017, 139, 4018–4024. [Google Scholar] [CrossRef]
  77. Subczynski, W.K.; Pasenkiewicz-Gierula, M.; Widomska, J.; Mainali, L.; Raguz, M. High Cholesterol/Low Cholesterol: Effects in Biological Membranes: A Review. Cell Biochem. Biophys. 2017, 75, 369–385. [Google Scholar] [CrossRef]
  78. Levental, I.; Christian, D.A.; Wang, Y.-H.H.; Madara, J.J.; Discher, D.E.; Janmey, P.A. Calcium-dependent lateral organization in phosphatidylinositol 4,5-bisphosphate (PIP2)- and cholesterol-containing monolayers. Biochemistry 2009, 48, 8241–8248. [Google Scholar] [CrossRef] [Green Version]
  79. Kwik, J.; Boyle, S.; Fooksman, D.; Margolis, L.; Sheetz, M.P.; Edidin, M. Membrane cholesterol, lateral mobility, and the phosphatidylinositol 4,5-bisphosphate-dependent organization of cell actin. Proc. Natl. Acad. Sci. 2003, 100, 13964–13969. [Google Scholar] [CrossRef] [Green Version]
  80. Hao, M.; Bogan, J.S. Cholesterol regulates glucose-stimulated insulin secretion through phosphatidylinositol 4,5-bisphosphate. J. Biol. Chem. 2009, 284, 29489–29498. [Google Scholar] [CrossRef] [Green Version]
  81. Epand, R.M. Proteins and cholesterol-rich domains. Biochim. Biophys. Acta Biomembr. 2008, 1778, 1576–1582. [Google Scholar] [CrossRef] [Green Version]
  82. Pike, L.J.; Miller, J.M. Cholesterol depletion delocalizes phosphatidylinositol bisphosphate and inhibits hormone-stimulated phosphatidylinositol turnover. J. Biol. Chem. 1998, 273, 22298–22304. [Google Scholar] [CrossRef] [Green Version]
  83. Van Rheenen, J.; Achame, E.M.; Janssen, H.; Calafat, J.; Jalink, K. PIP2 signaling in lipid domains: A critical re-evaluation. EMBO J. 2005, 24, 1664–1673. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  84. Mu, L.; Tu, Z.; Miao, L.; Ruan, H.; Kang, N.; Hei, Y.; Chen, J.; Wei, W.; Gong, F.; Wang, B.; et al. A phosphatidylinositol 4,5-bisphosphate redistribution-based sensing mechanism initiates a phagocytosis programing. Nat. Commun. 2018, 9, 1–16. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  85. Ponuwei, G.A. A glimpse of the ERM proteins. J. Biomed. Sci. 2016, 23, 35. [Google Scholar] [CrossRef] [Green Version]
  86. Taglieri, D.M.; Delfín, D.A.; Monasky, M.M. Cholesterol regulation of PIP2: Why cell type is so important. Front. Physiol. 2013, 3, 492. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  87. Chierico, L.; Joseph, A.S.; Lewis, A.L.; Battaglia, G. Live cell imaging of membrane/cytoskeleton interactions and membrane topology. Sci. Rep. 2014, 4, 6056. [Google Scholar] [CrossRef] [Green Version]
  88. Johnson, C.; Rodgers, W. Spatial Segregation of Phosphatidylinositol 4,5-Bisphosphate (PIP2) Signaling in Immune Cell Functions. Immunol. Endocr. Metab. Agents Med. Chem. 2009, 8, 349–357. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  89. Nebl, T.; Oh, S.W.; Luna, E.J. Membrane cytoskeleton: PIP2 pulls the strings. Curr. Biol. 2000, 10, R351–R354. [Google Scholar] [CrossRef] [Green Version]
  90. Zhang, L.; Mao, Y.S.; Janmey, P.A.; Yin, H.L. Phosphatidylinositol 4, 5 bisphosphate and the actin cytoskeleton. Subcell. Biochem. 2012, 59, 177–215. [Google Scholar] [CrossRef]
  91. Andrade, D.M.; Clausen, M.P.; Keller, J.; Mueller, V.; Wu, C.; Bear, J.E.; Hell, S.W.; Lagerholm, B.C.; Eggeling, C. Cortical actin networks induce spatio-temporal confinement of phospholipids in the plasma membrane—A minimally invasive investigation by STED-FCS. Sci. Rep. 2015, 5, 1–12. [Google Scholar] [CrossRef] [Green Version]
  92. Cho, H.; Kim, Y.A.; Yoon, J.Y.; Lee, D.; Kim, J.H.; Lee, S.H.; Ho, W.K. Low mobility of phosphatidylinositol 4,5-bisphosphate underlies receptor specificity of Gq-mediated ion channel regulation in atrial myocytes. Proc. Natl. Acad. Sci. USA 2005, 102, 15241–15246. [Google Scholar] [CrossRef] [Green Version]
  93. Corbett-Nelson, E.F.; Mason, D.; Marshall, J.G.; Collette, Y.; Grinstein, S. Signaling-dependent immobilization of acylated proteins in the inner monolayer of the plasma membrane. J. Cell Biol. 2006, 174, 255–265. [Google Scholar] [CrossRef] [PubMed]
  94. Botelho, R.J.; Teruel, M.; Dierckman, R.; Anderson, R.; Wells, A.; York, J.D.; Meyer, T.; Grinstein, S. Localized biphasic changes in phosphatidylinositol-4,5-bisphosphate at sites of phagocytosis. J. Cell Biol. 2000, 151, 1353–1367. [Google Scholar] [CrossRef] [PubMed]
  95. Zimmerberg, J.; Chernomordik, L.V. Membrane fusion. Adv. Drug Deliv. Rev. 1999, 38, 197–205. [Google Scholar] [CrossRef]
Molecules 25 03885 g001 550
Figure 1. Membrane processes associated with or dependent on phosphatidylinositol 4,5-bisphosphate (PI(4,5)P2). Figure created with BioRender.com.
Figure 1. Membrane processes associated with or dependent on phosphatidylinositol 4,5-bisphosphate (PI(4,5)P2). Figure created with BioRender.com.
Molecules 25 03885 g001
Molecules 25 03885 g002 550
Figure 2. PI(4,5)P2 headgroup features. The PI(4,5)P2 headgroup consists of myo-inositol ring where every hydroxyl substituent is at the equatorial position except for the hydroxyl in the position 2 of the ring, which is in an axial position. In the case of PIP2, the hydroxyls in positions 4 and 5 are enzymatically phosphorylated. It is linked to the diacylglycerol (DAG) backbone via a phosphodiester bond in position 1 (A). At pH 7.0, one of the phosphodiester proton dissociates, and the one remaining is shared between the two vicinal phosphomonoester groups. In terms of potential charge this means that, at pH 7.0, the charges would be −1.58 and −1.41 for the phosphomonoester groups at positions 4 and 5, respectively [19]. The lower charge of the 5-phosphomonoester group is attributed to a network of intramolecular hydrogen bonds that it is engaged in, which stabilize the proton (B). Carbon atoms are colored in grey, hydrogen in white, oxygen in red, and phosphorus in orange. Snapshots obtained from a simulation of a bilayer consisting of 95:5 mol ratio 1-palmitoyl-2-oleoyl-sn-glycero-3-phosphocholine (POPC): PI(4,5)P2, using the CHARMM36m forcefield run in GROMACS2019. Images were modeled using VMD.
Figure 2. PI(4,5)P2 headgroup features. The PI(4,5)P2 headgroup consists of myo-inositol ring where every hydroxyl substituent is at the equatorial position except for the hydroxyl in the position 2 of the ring, which is in an axial position. In the case of PIP2, the hydroxyls in positions 4 and 5 are enzymatically phosphorylated. It is linked to the diacylglycerol (DAG) backbone via a phosphodiester bond in position 1 (A). At pH 7.0, one of the phosphodiester proton dissociates, and the one remaining is shared between the two vicinal phosphomonoester groups. In terms of potential charge this means that, at pH 7.0, the charges would be −1.58 and −1.41 for the phosphomonoester groups at positions 4 and 5, respectively [19]. The lower charge of the 5-phosphomonoester group is attributed to a network of intramolecular hydrogen bonds that it is engaged in, which stabilize the proton (B). Carbon atoms are colored in grey, hydrogen in white, oxygen in red, and phosphorus in orange. Snapshots obtained from a simulation of a bilayer consisting of 95:5 mol ratio 1-palmitoyl-2-oleoyl-sn-glycero-3-phosphocholine (POPC): PI(4,5)P2, using the CHARMM36m forcefield run in GROMACS2019. Images were modeled using VMD.
Molecules 25 03885 g002
Molecules 25 03885 g003 550
Figure 3. Examples of PI(4,5)P2 headgroup tilt when inserted into a phospholipid membrane. PI(4,5)P2 presents a significant headgroup tilt, when inserted into a bilayer, ranging from almost parallel to the membrane plane (A) to a more conservative ~40° tilt (B). Whilst the more dramatic headgroup tilt appears to be favored from interactions between its negatively charged phosphate groups and the positively charged membrane surface, the more moderate tilt surges from the establishment of intramolecular hydrogen bonds between the C2 hydroxyl and the pro-R-oxygen of the phosphodiester phosphate. Carbon atoms are colored in grey, hydrogen in white, oxygen in red, and phosphorus in orange. Snapshots obtained from a simulation of a bilayer consisting of 95:5 mol ratio POPC: PI(4,5)P2, using the CHARMM36m forcefield run in GROMACS2019. Images were modeled using VMD.
Figure 3. Examples of PI(4,5)P2 headgroup tilt when inserted into a phospholipid membrane. PI(4,5)P2 presents a significant headgroup tilt, when inserted into a bilayer, ranging from almost parallel to the membrane plane (A) to a more conservative ~40° tilt (B). Whilst the more dramatic headgroup tilt appears to be favored from interactions between its negatively charged phosphate groups and the positively charged membrane surface, the more moderate tilt surges from the establishment of intramolecular hydrogen bonds between the C2 hydroxyl and the pro-R-oxygen of the phosphodiester phosphate. Carbon atoms are colored in grey, hydrogen in white, oxygen in red, and phosphorus in orange. Snapshots obtained from a simulation of a bilayer consisting of 95:5 mol ratio POPC: PI(4,5)P2, using the CHARMM36m forcefield run in GROMACS2019. Images were modeled using VMD.
Molecules 25 03885 g003
Molecules 25 03885 g004 550
Figure 4. Snapshots of calcium ions interacting with the PI(4,5)P2 headgroup phosphates. Calcium can bind to PI(4,5)P2 either solely near the 4-phophomonoester (A) or in between the phosphomonoester groups (B). However, simultaneous binding between the two phosphomonoester groups is approximately 10 kcal/mol more unfavorable [31]. Carbon atoms are colored in grey, hydrogen in white, oxygen in red, phosphorus in orange, and calcium in blue. Snapshots obtained from a simulation of a bilayer consisting of 95:5 mol ratio POPC: PI(4,5)P2 in the presence of calcium in a 5:1 calcium to PI(4,5)P2 ratio, using the CHARMM36m forcefield run in GROMACS2019. Images were modeled using VMD.
Figure 4. Snapshots of calcium ions interacting with the PI(4,5)P2 headgroup phosphates. Calcium can bind to PI(4,5)P2 either solely near the 4-phophomonoester (A) or in between the phosphomonoester groups (B). However, simultaneous binding between the two phosphomonoester groups is approximately 10 kcal/mol more unfavorable [31]. Carbon atoms are colored in grey, hydrogen in white, oxygen in red, phosphorus in orange, and calcium in blue. Snapshots obtained from a simulation of a bilayer consisting of 95:5 mol ratio POPC: PI(4,5)P2 in the presence of calcium in a 5:1 calcium to PI(4,5)P2 ratio, using the CHARMM36m forcefield run in GROMACS2019. Images were modeled using VMD.
Molecules 25 03885 g004
Molecules 25 03885 g005 550
Figure 5. Snapshots of experiments on mixed lipid monolayers, containing different mol % of 1-stearoyl-2-oleoyl-sn-glycero-3-phosphocholine (SOPC) and PI(4,5)P2, while exposed to calcium. Reprinted from Biophysical Journal, 101, Ellenbroek, W.G.; Wang, Y.H.; Christian, D.A.; Discher, D.E.; Janmey, P.A.; Liu, A.J. Divalent cation-dependent formation of electrostatic PIP2 clusters in lipid monolayers. 2178–2184, Copyright (2011), with permission from Elsevier [69].
Figure 5. Snapshots of experiments on mixed lipid monolayers, containing different mol % of 1-stearoyl-2-oleoyl-sn-glycero-3-phosphocholine (SOPC) and PI(4,5)P2, while exposed to calcium. Reprinted from Biophysical Journal, 101, Ellenbroek, W.G.; Wang, Y.H.; Christian, D.A.; Discher, D.E.; Janmey, P.A.; Liu, A.J. Divalent cation-dependent formation of electrostatic PIP2 clusters in lipid monolayers. 2178–2184, Copyright (2011), with permission from Elsevier [69].
Molecules 25 03885 g005
Molecules 25 03885 g006 550
Figure 6. Crosslinking of PI(4,5)P2 lipids induces the formation of PI(4,5)P2 nanodomains. As a single divalent cation can bind up to 2 PI(4,5)P2 lipids and each lipid can potentially bind 3 divalent cations, a network of electrostatic interactions can crosslink PI(4,5)P2 lipids together (A). As the number of clustered lipids increases, PI(4,5)P2 nanodomains are formed (B). Coarse grain beads representing the inositol headgroup and acyl-chains are colored in grey, the glycerol component in red, the phosphate groups in orange, and calcium in blue. Snapshots obtained from a simulation of a bilayer consisting of 95:5 mol ratio POPC: PI(4,5)P2 in the presence of calcium in a 5:1 calcium to PI(4,5)P2 ratio, using the martini 2.2 coarse-grained forcefield run in GROMACS2019. Images were modeled using VMD.
Figure 6. Crosslinking of PI(4,5)P2 lipids induces the formation of PI(4,5)P2 nanodomains. As a single divalent cation can bind up to 2 PI(4,5)P2 lipids and each lipid can potentially bind 3 divalent cations, a network of electrostatic interactions can crosslink PI(4,5)P2 lipids together (A). As the number of clustered lipids increases, PI(4,5)P2 nanodomains are formed (B). Coarse grain beads representing the inositol headgroup and acyl-chains are colored in grey, the glycerol component in red, the phosphate groups in orange, and calcium in blue. Snapshots obtained from a simulation of a bilayer consisting of 95:5 mol ratio POPC: PI(4,5)P2 in the presence of calcium in a 5:1 calcium to PI(4,5)P2 ratio, using the martini 2.2 coarse-grained forcefield run in GROMACS2019. Images were modeled using VMD.
Molecules 25 03885 g006
Molecules 25 03885 g007 550
Figure 7. Ternary diagram for the POPC:PSM:Chol lipid mixture at 25 °C (A) and 37 °C (B). Color-code depicts decrease in measured fluorescence anisotropies of a PI(4,5)P2 fluorescent analog (TF-PI(4,5)P2) upon inclusion of 100 µM Ca2+. Since the decrease reflects homo-FRET between analogs incorporated within the same clusters, darker areas correspond to more efficient PI(4,5)P2 clustering. Adapted with permission from Sarmento, M.J.; Coutinho, A.; Fedorov, A.; Prieto, M.; Fernandes, F. Membrane order is a key regulator of divalent cation-induced clustering of PI(3,5)P2 and PI(4,5)P2. Langmuir 2017, 33, 12463–12477 [78]. Copyright (2017) American Chemical Society.
Figure 7. Ternary diagram for the POPC:PSM:Chol lipid mixture at 25 °C (A) and 37 °C (B). Color-code depicts decrease in measured fluorescence anisotropies of a PI(4,5)P2 fluorescent analog (TF-PI(4,5)P2) upon inclusion of 100 µM Ca2+. Since the decrease reflects homo-FRET between analogs incorporated within the same clusters, darker areas correspond to more efficient PI(4,5)P2 clustering. Adapted with permission from Sarmento, M.J.; Coutinho, A.; Fedorov, A.; Prieto, M.; Fernandes, F. Membrane order is a key regulator of divalent cation-induced clustering of PI(3,5)P2 and PI(4,5)P2. Langmuir 2017, 33, 12463–12477 [78]. Copyright (2017) American Chemical Society.
Molecules 25 03885 g007

Share and Cite

MDPI and ACS Style

Borges-Araújo, L.; Fernandes, F. Structure and Lateral Organization of Phosphatidylinositol 4,5-bisphosphate. Molecules 2020, 25, 3885. https://doi.org/10.3390/molecules25173885

AMA Style

Borges-Araújo L, Fernandes F. Structure and Lateral Organization of Phosphatidylinositol 4,5-bisphosphate. Molecules. 2020; 25(17):3885. https://doi.org/10.3390/molecules25173885

Chicago/Turabian Style

Borges-Araújo, Luís, and Fabio Fernandes. 2020. "Structure and Lateral Organization of Phosphatidylinositol 4,5-bisphosphate" Molecules 25, no. 17: 3885. https://doi.org/10.3390/molecules25173885

APA Style

Borges-Araújo, L., & Fernandes, F. (2020). Structure and Lateral Organization of Phosphatidylinositol 4,5-bisphosphate. Molecules, 25(17), 3885. https://doi.org/10.3390/molecules25173885

Article Metrics

Back to TopTop