Understanding lipid rafts and other related membrane domains

Abstract

Evidence in support of the classical lipid raft hypothesis has remained elusive. Data suggests that transmembrane proteins and the actin-containing cortical cytoskeleton can organize lipids into short-lived nanoscale assemblies that can be assembled into larger domains under certain conditions. This supports an evolving view in which interactions between lipids, cholesterol, and proteins create and maintain lateral heterogeneity in the cell membrane.

Introduction and context

Differential lipid composition between the apical and basolateral membrane domains of epithelial cell plasma membranes [1,2] made it clear that membrane lipids are not laterally distributed in a homogeneous fashion. The lipid raft hypothesis was developed to explain lateral separation of bilayer lipids, and this idea quickly found applications in viral budding, endocytosis, and signal transduction (reviewed in [3]). In model membranes, lipids can separate into microscopically resolvable raft-like domains [4]. Plasma membrane surrogates formed by chemical membrane blebbing or cell swelling procedures also show phase behaviour [5-8]. Similar domains are not evident upon direct observation of unperturbed plasma membranes in living cells, but the non-equilibrium nature of cell membranes, including endocytosis, exocytosis, and other motile processes, may prevent overt phase separation. Likewise, quantitative analysis of lipid-anchored protein and lipid diffusion in cell membranes by fluorescence recovery after photobleaching (FRAP), Förster resonance energy transfer (FRET), and fluorescence correlation spectroscopy (FCS) [9-11] indicated that rafts in the plasma membrane of resting cells must be very small or ephemeral (or both), forcing an evolution of the lipid raft hypothesis. These tiny clusters do not represent lipid phase separations but are probably short-range ordering imposed upon lipids by transmembrane proteins and cortical actin structures. Thus, the current challenge for the field is to understand the interplay between protein and lipid that converts the exceedingly small, unstable clusters of components into larger, more stable membrane microdomains required for function [3,12].

Major recent advances

The recent development of sensitive quantitative microscopy methods has advanced our knowledge of lipid dynamics in resting cells. The diffusion of raft lipids (e.g., sphingomyelin) and non-raft lipids (e.g., phosphatidylethanolamine) was measured by an elegant FCS technique within regions as small as 30 nm in diameter using stimulation emission depletion fluorescence microscopy. The results indicate that raft lipids, but not non-raft lipids, are indeed preferentially trapped, albeit for short distances (<20 nm) and for short periods (10-20 ms) [13]. HomoFRET measurements, combining FRAP, emission anisotropy, and theoretical model fitting to test models of lateral organization in the membrane, were used determine the degree of clustering of glycosylphosphatidylinositol (GPI)-anchored proteins in the plasma membrane [14,15]. The formation of GPI-anchored protein nanoclusters (of ~4 molecules or even less) [14] is an active process involving both actin and myosin, and these nanoclusters are nonrandomly distributed into larger domains of <450 nm [15]. Additionally, high-speed single-particle tracking (50 kHz) revealed that GPI-anchored proteins, along with other membrane proteins, undergo rapid hop diffusion between 40 nm actin-regulated compartments, with a compartment dwell time of 1-3 ms on average [16]. However, when GPI-anchored proteins were deliberately cross-linked by gold or quantum dot particles, they underwent transient confinement or ‘STALL’ (stimulation-induced temporary arrest of lateral diffusion) from a cholesterol-dependent nanodomain in a Src family kinase mediated manner [17-19]. A recent study identified a transmembrane protein (carboxyl-terminal Src kinase [Csk]-binding protein) involved in the linkage between the particle-cross-linked GPI-anchored protein, Thy1, and the cytoskeleton (Figure 1) [20].

Figure 1. EBP50-ERM assembly is the common adaptor complex for linking cholesterol-dependent Thy-1 clusters to the membrane apposed cytoskeleton.

The glycosylphosphatidylinositol (GPI)-anchored protein Thy-1 engages membrane lipids and proteins for transmembrane signaling. Thy-1 crosslinking by streptavidin-coated quantum dots aggregates GPI lipid tails in the outer leaflet of the plasma membrane in a cholesterol-dependent manner. Carboxyl-terminal Src kinase (Csk)-binding protein (CBP), a transmembrane protein, is recruited to or captured by Thy-1 clusters along with Src-family kinase substrates (KS). CBP or KS (or both) are phosphorylated by Src-family kinases (SFK), enabling CBP to bind to actin filaments via an EBP50-ERM (ezrin/radixin/moesin-binding phosphoprotein 50-ezrin/radixin/moesin) adaptor linkage resulting in a transient anchorage. When either CBP or the adaptors are dephosphorylated by an unspecified protein tyrosine phosphatase (PTP) the anchorage is terminated. Image adapted from [20]; Chen et al., J Cell Sci 2009.

Larger microdomains involve raft lipids and specific membrane proteins. The lipid envelope of influenza and HIV virions, but not those of the vesicular stomatitis virus (VSV) or Semliki Forest virus (SFV), is enriched in raft-like lipids, leading to the notion that these viruses bud from lipid microdomains in the plasma membrane [21-25]. By contrast, the lipidomes of VSV and SFV are very similar to each other and to that of the plasma membrane suggesting that these viruses do not select or generate lipid raft domains for budding [25].

The protein and lipid environment of the budding domains of hemagglutinin (HA) and HIV has been the source of several recent papers examining the process of viral budding using quantitative live-cell imaging techniques. Influenza buds from HA clusters (ranging up to micrometers in diameter) [26] regulated by HA transmembrane region length and palmitoylation [27]. Recent fluorescence lifetime imaging microscopy (FLIM)-FRET experiments in living cells indicate that HA colocalizes with lipid microdomain markers, further supporting the role of lipid-protein interactions in influenza virus budding [28,29]. Proton magic angle spinning nuclear magnetic resonance was used to detect a minor fraction (~10-15%) of liquid-ordered membrane phospholipids in HA virions and virion lipid extracts at 37°C. While lipid ordering increased at lower temperatures, it was not required for virion fusion with target membranes [30].

Progressive recruitment of cytoplasmic HIV-1 Gag to the membrane, via post-translational acyl lipid modification and PIP₂/basic residue interactions, forms membrane domains that culminate in virion budding [31-33]. While the HIV-1 lipid envelope composition indicates enrichment in lipids and proteins associated with ‘rafts’ [21], paradoxically, one report has failed to observe an enrichment of enhanced green fluorescent protein (EGFP)-GPI at Gag domains in living cells [32], suggesting that the local lipid microenvironment may not exactly parallel the classic raft lipid composition. Recent work has implicated the tetraspanin family of proteins in Gag domain formation and function. Tetraspanins, a widely expressed and highly conserved class of transmembrane proteins (reviewed in [34]), form tetraspanin-enriched microdomains (TEMs) through lateral tetraspanin-tetraspanin interactions and binding to non-tetraspanin membrane proteins. HIV-1 Gag is targeted to TEMs and virus buds from these domains [35,36]. Tetraspanins can be palmitoylated [37] and the lipid environment within TEMs contains cholesterol, but GPI-anchored proteins and caveolin are not enriched in TEMs (reviewed in [38]). Recently, cholesterol and tetraspanin palmitoylation were implicated in the confined diffusion and co-diffusion (of two tetraspanin molecules) of the tetraspanin CD9 [39]. Tetraspanins appear to induce order in the plasma membrane by virtue of protein clustering, but they likely also stabilize lipid microenvironments in the plasma membrane allowing for lateral organization of HIV-1 Gag and virion budding.

Some lectin-based membrane domains form in the absence of post-translational lipid modifications or known lipid binding activity. Dendritic cell-specific intracellular adhesion molecule-3-grabbing non-integrin (DC-SIGN), a tetrameric C-type lectin with affinity for high-mannose glycans, forms microdomains on the plasma membrane [40-42] that serve as high-avidity binding sites for numerous pathogens. A previous report suggested that DC-SIGN interacts with lipid rafts [40], but this was based on detergent insolubility and cholera toxin colocalization assays, which generally do not faithfully report on intrinsic membrane lateral heterogeneity. Also, DC-SIGN domains do not depend on cholesterol (unpublished data). Surprisingly, DC-SIGN domains do not recover following photobleaching [42]. This result implies that DC-SIGN within domains does not exchange with the surrounding membrane. The source of this stability remains a mystery, and its cause may not reside in the membrane-apposed cytoskeleton but in extracellular cross-linking factors such as galectins (reviewed in [43]). DC-SIGN membrane domains that are multiplexed with another C-type lectin, CD206 (unpublished data), appear to mediate the formation of fungipods, novel cellular protrusive structures involved in fungal recognition by dendritic cells (Figure 2) [44]. Thus, the lateral heterogeneity in membranes provided by rafts and other microdomains continues to provide surprising functional consequences.

Figure 2. C-type lectin domains and fungipod formation.

C-type lectins (CLRs) form a type of plasma membrane domain that is not dependent on cholesterol. (A) Plasma membrane domains containing mixtures (yellow) of dendritic cell-specific intracellular adhesion molecule-3-grabbing non-integrin (DC-SIGN) (green) and CD206 (red) are observed on a monocyte-derived dendritic cell (DC) by immunofluorescence. DC-SIGN domains are known sites of binding and entry for a range of pathogens including HIV-1. (B) Yeast cell wall material is sensed by these CLR membrane domains, triggering a unique protrusive response, the fungipod. The image shows an example of a DC fungipod formed via CD206 ligation by a fixed Saccharomyces cerevisiae particle (zymosan), visualized by scanning electron microscopy (9500×). Figure 2B was reproduced from [44], Neumann & Jacobson, PLoS Pathog 2010.

Future directions

A variety of membrane domain forming systems have a wide gamut of lipid and protein constituents and possess a correspondingly broad range of functions. Recent advances have shown that preferential lipid trapping or confinement in the resting plasma membrane occurs only on very small spatiotemporal scales. Critical attention must be paid when determining if and when such confinement becomes biologically meaningful for processes such as endocytosis and signal transduction. While lipid ordering can be stabilized by oligomerization of membrane-associated proteins (i.e., GM1 crosslinking, influenza HA clustering), the lipids in these domains may still exchange between domain and surrounding membranes, making even these stabilized raft-like domains dynamic environments. At what point does a membrane domain become stable enough to be biologically relevant? What is the range of protein and lipid turnover rates seen in membrane domains and are there different turnover rates for each constituent? It is likely that a spectrum of membrane microdomains exists with different compositions and physical characteristics suited to their diverse purposes. The lipid species and their ordering within raft-like complexes appear to be key factors in determining intradomain cohesiveness and resultant domain size and lifetime.

Abbreviations

DC-SIGN

dendritic cell-specific intracellular adhesion molecule-3-grabbing non-integrin

FCS

fluorescence correlation spectroscopy

FRAP

fluorescence recovery after photobleaching

FRET

Förster resonance energy transfer

GPI

glycosylphosphatidylinositol

HA

hemagglutinin

PIP₂

phosphatidylinositol 4,5-bisphosphate

SFV

Semliki Forest virus

TEM

tetraspanin-enriched microdomain

VSV

vesicular stomatitis virus

Competing interests

The authors declare that they have no competing interests.

The electronic version of this article is the complete one and can be found at: http://f1000.com/reports/b/2/31