Here, there, and everywhere: The importance of ER membrane contact sites

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Science  03 Aug 2018:
Vol. 361, Issue 6401, eaan5835
DOI: 10.1126/science.aan5835

It's all about your contacts

Membrane contact sites have recently come to the fore of our understanding of interorganelle communication. Wu et al. review how these important structures help to promote a variety of key functions, including organelle division and lipid transfer. Focusing on contacts between the endoplasmic reticulum and a variety of organelles or the plasma membrane reveals the generality and importance of these contacts in cellular homeostasis and organismal health.

Science, this issue p. eaan5835

Structured Abstract


The defining feature of eukaryotic cells is the presence of membrane-bound organelles of diverse kinds, each with specialized functions. Most organelles have multiple copies in cells. By contrast, each cell contains only one endoplasmic reticulum (ER). However, the ER consists of an elaborate network of membrane cisternae and tubules that extends throughout the cell and occupies a large fraction of the cytoplasmic volume. Though compartmentalization of biochemical reactions and processes in these organelles has obvious advantages, it also poses challenges for their coordinated activity, requiring mechanisms for regulated interorganelle communication. However, these mechanisms have remained elusive, and the quintessential textbook diagram still pictures organelles in isolation, floating in a cytoplasmic sea. The last decade has radically changed this view, and membrane contact sites (MCSs) between different organelles have been brought to center stage as prime, highly regulated routes for interorganelle communication essential for cell homeostasis.


The presence of organelle contacts was recognized long ago. However, the functions of these structures remained unclear. Recent advances in the resolution of microscopy and the development of unique fluorophores have markedly advanced our ability to study interorganelle MCSs. The three-dimensional structure of ER MCSs with other organelles and the plasma membrane (PM) can be visualized at nanometer resolution by electron microscopy (EM). Multispectral live-cell fluorescence microscopy displays the behavior of MCSs over time and in response to stimuli. Together, these data have revealed the general features of MCSs. For example, EM has revealed that MCSs are closely opposed and tethered but not fused membranes, MCSs are spaced at 10 to 30 nm, and ribosomes are excluded from the ER surface at these sites. Fluorescence microscopy demonstrates that organelles can remain attached to ER tubules as they traffic along microtubules. The combinations of these tools with classical molecular biology and biochemical tools have identified molecules implicated in several MCSs and elucidated their functions, including lipid and ion transport between organelles and organelle positioning and division.


MCSs are central to normal cell physiology. Moreover, several MCS proteins are linked to various diseases: seipin, protrudin, and spastin to hereditary spastic paraplegia; VAPA and VAPB to amyotrophic lateral sclerosis; Dnm2 and Mfn2 to Charcot-Marie-Tooth disease; STIM1 and Orai1 to tubular aggregate myopathy; and ACBD5 to retinal dystrophy. Whether defects in MCS functions cause these diseases directly or indirectly remains to be explored. Recent progress has begun to identify some of the molecular machineries that regulate MCS formation. Dissecting the roles of these factors will strengthen our understanding of the integrative nature of MCSs. The advancement of diverse microscopy techniques will allow us to track multiple factors at MCSs simultaneously in real time and at high resolution, and this may help us gain a more detailed view of the biology of MCSs and their related physiological processes.

ER MCSs with other organelles and the PM.

The ER forms MCSs with mitochondria, Golgi, endosomes, peroxisomes, lipid droplets, and the PM. These MCSs are closely opposed but not fused membranes containing various molecular machineries. Factors localized to these MCSs mediate essential cellular processes, including lipid and ion exchange, organelle positioning, and biogenesis.


Our textbook image of organelles has changed. Instead of revealing isolated cellular compartments, the picture now emerging shows organelles as largely interdependent structures that can communicate through membrane contact sites (MCSs). MCSs are sites where opposing organelles are tethered but do not fuse. MCSs provide a hybrid location where the tool kits of two different organelles can work together to perform vital cellular functions, such as lipid and ion transfer, signaling, and organelle division. Here, we focus on MCSs involving the endoplasmic reticulum (ER), an organelle forming an extensive network of cisternae and tubules. We highlight how the dynamic ER network regulates a plethora of cellular processes through MCSs with various organelles and with the plasma membrane.

Membrane contact sites (MCSs) are conserved and extensive along the tubular endoplasmic reticulum (ER) membrane (Fig. 1, A and B). Thus, it was postulated that MCSs must play key roles in cell physiology. The contacts between the membrane of the ER and other organelles were first appreciated decades ago, during the early days of electron microscopy (EM). But what remained unclear was whether MCSs represented short-lived interactions made for the quick transfer of cellular material or were stable sites of tethering. The advent of various technologies, including the discovery of a wide spectrum of fluorescent proteins and the ability to image live cells at greatly improved spatial and temporal resolution by microscopy, has made it possible to image and track multiple dynamic organelles simultaneously over time, revealing the extent to which other organelles are tightly tethered to the ER (1) (Fig. 1C). Notably, MCSs with elastic ER tubules are maintained during trafficking, fusion, and fission of the attached organelles. A major research focus in cell biology is to discover the factors establishing MCSs and how MCSs regulate essential cellular processes, from lipid and ion homeostasis to organelle division and distribution.

Fig. 1 Visualizing ER MCSs with other organelles.

(A) Diagram depicting the distribution and structure of the ER and the MCSs it forms with other organelles and with the plasma membrane (PM). (B) Electron micrographs of ER MCSs with mitochondria, Golgi, LDs, and the PM. Micrographs of ER-mitochondria and ER-Golgi MCSs in rat epithelial cells were provided by M. Ladinsky. Micrographs of ER-LD MCSs in yeast cells were provided by M. Radulovic. ER-PM MCSs in a mouse neuron (left) were imaged by focused ion beam scanning electron microscopy, and the micrograph was provided by Y. Wu and P. De Camilli [adapted from (3)]. The micrograph of ER-PM MCSs in yeast (right) was provided by M. West [reproduced from (83) (CC BY-NC-SA 3.0)]. Boxed areas correspond to images on the right. (C) Mitochondria, endosomes, and peroxisomes remain tethered to the ER tubules as they traffic. Time-lapse fluorescent images of the ER relative to mitochondria, LEs, and peroxisomes in live COS-7 cells are shown. Arrows denote MCSs. t, time in seconds.

Factors and functions of ER-mitochondria MCSs

Live-cell microscopy and electron tomography have revealed that mitochondria are tightly associated with the tubular ER in yeast cells and animal cells (Fig. 1, B and C) (2). Together, these techniques have shown that ER tubules wrap around the mitochondria to form MCSs that approach distances of 10 nm, are ribosome excluded (Fig. 1B), cover 2 to 5% of the mitochondrial surface area, and substantially influence mitochondrial dynamics (2, 3).

Early cell fractionation studies showed that certain ER components copurified with mitochondria, suggesting that these MCSs could be biochemically isolated. These mitochondria-associated membranes were enriched in a subset of ER enzymes involved in lipid biosynthesis and Ca2+ signaling, hinting at the functions of the ER MCSs with mitochondria (4). ER-mitochondria MCSs can provide a conduit for transport of high concentrations of Ca2+ from the ER lumen to the mitochondrial matrix (5). Calcium is released from the ER through the tetrameric inositol 1,4,5-triphosphate receptor (IP3R) channel and funneled to the voltage-dependent anion-selective channel (VDAC) in the outer mitochondrial membrane (OMM) (610). Once Ca2+ traverses the OMM, it can use the mitochondrial calcium uniporter to translocate across the inner mitochondrial membrane (IMM) into the matrix (11, 12). Grp75 is a cytosolic regulator of the IP3R-VDAC complex that promotes the interaction between the channels to increase the efficiency of mitochondrial Ca2+ uptake (8). The OMM protein mitofusin 2 (Mfn2) is one proposed tether for regulating this Ca2+ transport at ER-mitochondria MCSs (13). Mfn2 is a dynamin-like protein that functions to tether mitochondria during homotypic membrane fusion, similar to its paralog Mfn1 (14). Recently, an ER membrane protein, PDZD8, was also implicated in ER-dependent mitochondrial Ca2+ homeostasis (15). PDZD8 has notable similarities to the yeast protein Mmm1, a subunit of the ER-mitochondria encounter structure (ERMES) complex (see below). PDZD8 concentrates at ER-mitochondria MCSs, although mechanistically it is still unclear how PDZD8 localization and its role in Ca2+ homeostasis are achieved.

Both the ER and mitochondria are required for lipid biosynthesis, and various intermediate molecules must travel between these organelles, a shuttling likely to occur at MCSs. So far, the best candidate for this function is the ERMES complex in yeast (16). ERMES has four subunits: Mmm1, Mdm10, Mdm12, and Mdm34. These subunits form a complex to bridge the ER and mitochondria. Three out of four ERMES subunits (Mmm1, Mdm12, and Mdm34) contain synaptotagmin-like mitochondrial lipid-binding protein (SMP) domains, which form a long hydrophobic cavity to transfer lipids between membranes (17). ERMES is proposed to transfer phosphatidylserine (PS) and phosphatidylcholine to the mitochondrial membrane (16, 18, 19). Although some crystal structures are available (19, 20), a structure of the whole ERMES complex is needed to mechanistically elucidate how exactly the ERMES complex is involved in lipid transfer.

Genetic studies indicate that lipid transfer is quite pliable and may follow diverse routes. For example, only a marginal defect in cellular lipid composition is detected in ERMES mutants (16, 21). Under these conditions, distinct MCSs between mitochondria and the vacuole—the vacuole and mitochondria patch (vCLAMP)—become essential for lipid homeostasis. Highlighting the interdependence of these MCSs, ERMES becomes essential in cells lacking vCLAMP (2224). vCLAMP MCSs involve the OMM protein Mcp1 and soluble proteins Vps13 and vacuolar Vps39; however, it is not clear how they cooperate in lipid transfer (22, 23, 25, 26).

Similarly, ERMES is also essential in cells lacking Lam6/Ltc1, a member of a recently identified family of steroidogenic acute regulatory transfer (StART)–like proteins (27). Lam6/Ltc1 is an ER membrane protein that localizes to ER-mitochondria MCSs through interaction with OMM proteins Tom70 and Tom71 (27, 28). Like other members of the LAM (lipid transfer proteins anchored at a membrane contact site)/Ltc (lipid transfer at contact site) family, Lam6/Ltc1 is capable of sterol transfer in vitro through the StART-like domain (2729). However, further studies are required to test whether Lam6/Ltc1 lipid transfer activity is necessary at ER-mitochondria MCSs. So far, no lipid trafficking machinery in animal cells at ER-mitochondria MCSs has been described.

Mitochondria are dynamic organelles that remodel their network to maintain the integrity of their genome and metabolic state through a balance of fission and fusion. Mitochondrial fission and fusion are elaborate processes tightly regulated by conserved molecular machineries. A surprising function for ER-mitochondria MCSs is that they define the sites of mitochondrial division in yeast and animal cells (2) (Fig. 2, A and B). This process has been described in detail and occurs sequentially (Fig. 2A). First, ER tubules wrap around mitochondria to form MCSs defining the fission position; subsequently, mitochondrial constriction and division machineries are recruited to execute fission (2). Surprisingly, ER-associated IMM constriction occurs before OMM constriction (30). These data suggest that signals coming from the mitochondrial matrix initiate ER recruitment to the OMM to position the division machinery. That signal could be coming from the mitochondrial DNA (mtDNA), as actively replicating mtDNA nucleoids are present at sites of ER-associated mitochondrial constriction and division (Fig. 2A) (31, 32). In animal cells, mitochondria have wide diameters, and multiple machineries function in sequence to drive the process of ER-associated OMM constriction and division. First, mitochondria are constricted by actin-myosin assemblies recruited to the MCSs by an ER-localized inverted formin (INF2) and a mitochondrial actin nucleator (Spire 1c) (33, 34). Next, the mitochondrial division dynamin Drp1 is recruited to ER-marked mitochondrial constrictions. Drp1 (Dnm1 in yeast) is a cytosolic guanosine triphosphatase (GTPase) and dynamin family member that oligomerizes around the OMM to drive mitochondrial constriction in a GTPase-dependent manner (Fig. 2B) (3537). Drp1 is recruited from the cytoplasm to the mitochondria at ER MCSs by adaptor proteins such as Mff, MiD49, and Mid51 in animal cells (3842). Both Drp1 and the adaptors localize to ER-marked mitochondrial constrictions before division (2, 43). Drp1 can drive constriction of mitochondria down to <50 nm, at which point another dynamin family member, Dnm2, is recruited to complete fission at ER MCSs (Fig. 2A) (43).

Fig. 2 Organelle division by ER MCSs.

(A) Model of factors involved in ER-associated mitochondrial constriction and division in animal cells. ER MCSs and actively replicating nucleoids define where IMM constriction, followed by OMM constriction, occurs. The activities of INF2, Spire1c, and polymerized actin, followed by the sequential activities of Drp1 and Dnm2, are required to drive OMM constriction and division. (B) ER tubules define the position of mitochondrial constriction and division. Time-lapse live-cell imaging of the ER (green) and mitochondria (red) in a COS-7 cell shows that the division machinery Drp1 (cyan) is localized to the position where an ER tubule crosses over a mitochondrial constriction (first two time frames). As the mitochondria divide, the Drp1 punctum splits and the ER tubules bridge the gap to maintain contact with both Drp1-labeled ends on daughter mitochondria (arrows). Images were provided by J. Lee. (C) Dynamic ER tubules are recruited and rearrange around endosome cargo-sorting domains to promote endosome fission. Time-lapse live-cell imaging of the ER (green), LEs (red), and epidermal growth factor (EGF) cargo (blue) shows an endosome bud growing through an ER ring (arrows). As the ring closes, the bud undergoes fission (compare the third and fourth time frames). Reproduced from (61).

Factors and functions of ER-Golgi MCSs

Between the ER and the Golgi, cargo traffics by both vesicular and nonvesicular routes. Whereas proteins must be sorted into coated vesicles to traffic between these two organelles, lipids can take a more direct route. In fact, the general principle that lipids can be transferred at MCSs between the ER and other organelles was first demonstrated for the Golgi (44, 45). So far, vesicle-associated membrane protein–associated proteins (VAPs) are the only ER proteins known to regulate nonvesicular lipid trafficking at ER-Golgi MCSs. VAPs (VAPA and VAPB in animals, Scs2 and Scs22 in yeast) are highly conserved integral ER membrane proteins. VAPs localize throughout the ER, and they bridge contacts with various proteins to perform functions at multiple MCSs (Fig. 3). VAPs contain a major sperm protein (MSP) domain that interacts with the FFAT [two phenylalanines (FF) in an acidic tract] motif of protein partners located on the opposing membrane (46). At the ER–trans-Golgi network (TGN) MCSs, VAPs bridge contact with the FFAT motifs of three different lipid transfer proteins: Nir2 (45), ceramide transferase 1 (CERT) (44), and oxysterol-binding protein (OSBP) (Fig. 3, A and B) (47).

Fig. 3 The conserved ER proteins VAPA and VAPB establish MCSs with multiple organelles.

(A) Domain organization of ER-localized VAP and its binding partners. Some VAP binding partners have more than one location. VAPs are tail-anchored membrane proteins that contain an MSP domain, which interacts with the FFAT motif found on the other proteins listed. Orp5 is included as an exception because it is an ER-anchored lipid transfer protein that can regulate phospholipid trafficking at MCSs independently of VAPs. Other relevant domains are indicated, including PI transfer protein (PITP); DDHD, LNS2 (lipin/Nde1/Smp2), and PH domains; ORD; StART, MLN64 NH2-terminal (MENTAL), TM, and FYVE domains; the KIF5 binding domain (KIF5BD); the low-complexity region (LCR); and ACBD. Numbers indicate amino acid positions. (B) Diagram of VAP binding partners at ER-Golgi MCSs. Nir2 binds VAP, contains an LNS2 domain to bind to phosphatidic acid (PA) on the Golgi, and contains a PITP domain that may transfer PIs from the ER to the Golgi. OSBP binds VAP and contains a PH domain to bind PI4P at the Golgi and an ORD to transfer PI4P from the Golgi to the ER, where it can be processed by Sac1 in exchange for cholesterol. CERT binds VAP and contains a PH domain to bind PI4P at the Golgi and a StART domain to transfer ceramide from the ER to the Golgi. (C) Diagram of VAP binding partners at ER-endosome MCSs. OSBP binds VAP. OSBP contains a PH domain that binds PI4P on endosomes, and its ORD transfers PI4P to the ER membrane to be processed by Sac1. STARD3 binds VAP and contains a StART domain to bind cholesterol. ORP1L binds VAP when endosomal cholesterol is low, and it contains a PH domain to bind PI4P on endosomes and an ORD to transfer cholesterol from the ER to endosomes. At high endosomal cholesterol levels, ORP1L dissociates from VAP and can be found instead in complex with dynein, resulting in retrograde trafficking of endosomes. Protrudin is an ER protein that binds VAP and Rab7 and contains a FYVE domain to bind to endosomal PI3P. The protrudin-VAP-Rab7-PI3P complex associates with kinesin and promotes anterograde trafficking of LEs on MTs. (D) Diagram of VAP binding partners at ER-peroxisome MCSs. ACBD5 is a tail-anchored peroxisomal protein that binds to VAP and may transfer lipids at these MCSs. (E) Diagram of VAP binding partners at ER-PM MCSs. Nir2 binds VAP and functions as depicted in (B) to transfer PI from the ER to the PM. Yeast Osh3 binds Scs2 and Scs22 (VAP orthologs) and contains a PH domain to bind PI4P on the PM and an ORD to transfer PI4P from the PM to the ER, where it can also be processed by Sac1. ORP5 is an example that does not bind VAP. It is a tail-anchored ER membrane protein that contains a PH domain to bind PI4P on the PM and an ORD to exchange PI4P on the PM with PS on the ER.

OSBP is the prototype member of the OSBP/OSBP-related protein (ORP)/oxysterol-binding homology (Osh) family. OSBP contains a pleckstrin homology (PH) domain that binds phosphatidylinositol 4-phosphate (PI4P) at the TGN and an FFAT motif to bind to ER-localized VAPs. This protein bridge stabilizes ER-TGN MCSs when TGN PI4P levels are high. Under these conditions, the OSBP-related domain (ORD) of OSBP facilitates the exchange of cholesterol with PI4P between the ER and the TGN. At ER-Golgi MCSs, PI4P levels are kept low by the ER phosphatase Sac1, which can convert PI4P into phosphatidylinositol (PI) (Fig. 3B) (47). The transfer of PI4P down its concentration gradient drives cholesterol transport against its concentration gradient (47, 48). This process may be facilitated by Nir2, which also binds VAPs through an MSP-FFAT interaction (49) and is proposed to supply PI from the ER to the Golgi at MCSs through its PI transfer domain (Fig. 3, A and B) (45).

In animal cells, CERT transfers ceramide from the ER to the Golgi at ER-Golgi MCSs through its StART domain (44, 45). CERT also contains a PH domain to target it to the Golgi (44) and an FFAT motif to interact with ER-localized VAPs (Fig. 3, A and B) (50). In yeast, the ER membrane protein Nvj2 promotes ceramide transport to the Golgi. Nvj2-dependent ceramide transport strongly increases during ER stress, preventing toxic ceramide accumulation in the ER (51). This conditional transport system involves Nvj2 relocalization and requires its PH and SMP-like domains, implicated in lipid transfer at other MCSs. Nvj2 mutant phenotypes are partially suppressed by expression of mammalian homologs of Nvj2, suggesting that a similar CERT-independent ceramide transfer mechanism also operates in higher eukaryotes.

Factors and functions of ER-endosome MCSs

Cargo from the PM is internalized into vesicles destined for the endocytic pathway. Endosomes sort cargo as they mature and traffic. Very early in their maturation, endosomes acquire ER MCSs so that most early endosomes and all late endosomes (LEs) are bound to the tubular ER network (52, 53). Endosomes are so tightly tethered to the ER that they will pull ER tubules with them as they traffic with molecular motors along microtubules (MTs), as visualized by live-cell imaging (Fig. 1C). An individual endosome can form several ER MCSs, and cumulatively these contacts cover ~2 to 5% of the cytoplasmic surface (52, 54). The past decade has revealed several functions for ER MCSs with endosomes, including lipid trafficking, cargo sorting, endosome trafficking, and fission (55).

VAPs regulate multiple functions at ER-endosome MCSs. In animal cells, VAPs interact with at least three endosome-localized FFAT-containing partners: OSBP, STARD3, and ORP1L (Fig. 3, A and C). The VAP-ORP1L interaction is important to determine the direction of LE trafficking on MTs. ORP1L is an endosomal ORP that is implicated in lipid homeostasis at ER MCSs (Fig. 3). Consistently, ORP1L contains a hydrophobic pocket that may be involved in cholesterol transport at ER-endosome MCSs (Fig. 3C) (56, 57). ORP1L is considered a sterol sensor because its binding to VAPs on the ER depends on endosomal cholesterol levels (56, 57). When the level is high, ORP1L binds to cholesterol and the interaction with VAPs is precluded. Conversely, depletion of endosomal cholesterol frees ORP1L to interact with VAPs, which establishes an MCS between endosomes and the ER. This MCS influences the direction of LE trafficking on MTs. Rab7 GTPase also assembles into VAP-ORP1L complexes, resulting in the displacement of the dynein from the LE surface and halting the retrograde trafficking of LEs to the cell center (57). VAPs can also promote kinesin loading onto LEs when in complex with the ER membrane protein protrudin. The VAP-protrudin complex binds to Rab7 to recruit kinesin-1 to promote anterograde trafficking of LEs to the PM (Fig. 3, A and C) (58). Perhaps protrudin and VAPs work together with ORP1L and Rab7 to coordinate dynein dissociation and kinesin loading, resulting in anterograde trafficking of LEs in response to cholesterol levels.

VAPs also contribute to phospholipid homeostasis at ER-endosome MCSs. This is achieved through coordination with OSBP and the endosome-localized protein sorting nexin 2 (Snx2) to allow the ER-localized phosphatase Sac1 to process PI4P (Fig. 3C) (59). VAP depletion causes an increase in PI4P on early and late endosomal membranes and a ripple of downstream effects. The increase in endosomal PI4P boosts the levels of endosomal actin, which nucleates actin comets and alters endosomal motility, and this also reduces cargo trafficking from the endosome to the TGN (59).

ER-endosome MCSs can regulate cargo sorting directly. At least one key growth factor receptor, epidermal growth factor receptor (EGFR), is dephosphorylated by an ER-localized phosphatase, Ptp1B, and this leads to its internalization and subsequent degradation. EGFR and Ptp1B can be colocalized by immuno-EM at MCSs, and Ptp1b depletion by small interfering RNA decreases the number of ER-endosome MCSs and reduces the number of intraluminal vesicles per multivesicular body (60). Lastly, ER MCSs regulate cargo sorting by defining the position of endosome bud fission in a manner similar to their role on mitochondria. Both early endosomes and LEs sort out cargo to be degraded and material to be recycled into vacuolar and budding domains, respectively. ER tubules are recruited to the saddle between these domains, and fission follows MCS formation (Fig. 2C) (61). It is not known what machinery tethers this interaction. However, an ER-localized isoform of the MT-severing protein spastin may drive the final step of bud fission at the MCSs. When spastin is depleted, ER MCSs with endosome buds still form and accumulate but the efficiency of ER-associated bud fission is reduced (62).

Factors and functions of ER-peroxisome MCSs

The ER makes contact with most cellular organelles, and peroxisomes are no exception (Fig. 1C). Peroxisomes are ubiquitous organelles with essential roles in lipid synthesis, fatty acid turnover, and detoxification of reactive oxygen species. Many of these metabolic functions of peroxisomes are carried out in partnership with the ER. For example, the synthesis of ether-linked phospholipids in mammalian cells is initiated in peroxisomes but completed in the ER (63). This process requires lipid intermediates to traffic between the two organelles. Similarly, the phospholipids essential for peroxisome growth and division originate in the ER. ER-peroxisome MCSs, likely facilitating this active trading of metabolites, were described in a variety of cell types long ago. However, the identification of the machineries involved has only recently begun.

Acyl–coenzyme A (CoA) binding domain protein 5 (ACBD5), a tail-anchored peroxisomal membrane protein, establishes ER-peroxisome MCSs by binding through its FFAT motif to VAPs in the ER (Fig. 3, A and D) (64, 65). Supporting a function of this interaction in ER-peroxisomal tethering, overexpression of either ACBD5 or VAPA/VAPB increases the number and surface of MCSs between the ER and peroxisomes, with maximal effect observed when both proteins are overexpressed (64, 65). Conversely, depletion of either ACBD5 or VAPA/VAPB reduces ER-peroxisome MCSs. Depletion of ACBD5 and/or VAPA/VAPB also prevents membrane expansion under conditions that favor peroxisome elongation and a reduction in total ether lipids and cholesterol (65, 66). These observations support the anticipated role of ER-peroxisome MCSs in lipid transfer, even though direct transfer activity by VAP-ACBD5 has not yet been demonstrated.

Disruption of ER-peroxisome MCSs increases peroxisomal motility (64). Though not much is known about how peroxisomal function depends on the spatial distribution of peroxisomes, recent work has uncovered a link between peroxisome positioning and cell fate decisions in skin epithelia (67). Thus, MCSs may also affect cellular homeostasis by controlling organelle positioning. The regulation of peroxisome positioning by MCSs has been investigated in greater detail in Saccharomyces cerevisiae, where MCSs are essential for the proper partitioning of peroxisomes between mother and daughter cells in mitosis. In that case, the MCS is composed of distinct Pex3 molecules in the ER and peroxisomal membranes, bridged by the soluble Inp1 (inheritance of peroxisomes) protein (Fig. 4) (68). Besides VAP-ACBD5 and Pex3-Inp1, other proteins likely contribute to the tethering of the ER and peroxisomes in mammalian and yeast cells. A peroxisomal ACBD4 isoform, which has strong sequence similarity to ACBD5, interacts with VAPs and was suggested to also participate in ER-peroxisome MCSs (69).

Fig. 4 MCSs between the ER and ER-derived organelles.

Peroxisomes form MCSs with the ER. VAP on the ER membrane interacts with ACBD5 on peroxisomes (see Fig. 3). Pex3 molecules on both the ER and peroxisomal membranes are bridged by Inp1. A lens of neutral lipids build up in the ER membrane to form a precursor of LDs. Seipin and DGAT2 play important roles in LD biogenesis. Membrane bridges exist between the continuous ER and LD membranes. After budding off from the ER membrane, LDs and ER form canonical MCSs. FATP1 on the ER membrane binds DGAT2 on LDs. ER-localized SNAREs (Syntaxin18, Use1, and BNIP1) form MCSs with Rab18 on LDs through the NRZ complex (NAG, RINT1, and ZW10).

Factors and functions of ER–lipid droplet MCSs

Lipid droplets (LDs) are storage organelles for neutral lipids such as triglycerides and steryl esters. LDs make frequent and conspicuous contacts with the ER (70). However, ER-LD contacts are one of a kind, often displaying membrane continuity between the two organelles (see Fig. 1B and Fig. 4), a feature that sets them apart from canonical MCSs. These unusual contacts, normally described as membrane bridges, are intimately linked to the unique structure and process of biogenesis of LDs (Fig. 4). Unlike most membrane-bound organelles, which contain a bilayer, LDs contain a phospholipid monolayer surrounding a neutral lipid core. During LD biogenesis, a lens of neutral lipids accumulates in between the leaflets of the ER bilayer. The expansion of the lens, due to neutral lipid synthesis, facilitates the emergence of LDs at the ER surface. Thus, the LD monolayer is literally derived from and continuous with the cytoplasmic leaflet of the ER membrane (Fig. 4). The ER-LD membrane bridge facilitates the incorporation of neutral lipids into LDs, as well as hairpin-containing membrane proteins (70). Many aspects of LD biogenesis remain enigmatic, but seipin, an ER membrane protein sitting right at the ER-LD interface, clearly plays a central role in the process (7173). LDs still form after seipin depletion; however, ER-LD contacts are aberrant, resulting in defective incorporation of both neutral lipids and proteins and, ultimately, abnormal LD morphology (7277). Though diverse, non–mutually exclusive functions have been proposed for seipin, the mechanisms by which it affects ER-LD contacts remain unresolved. In humans, seipin is encoded by the Berardinelli-Seip congenital lipodystrophy 2 (BSCL2) gene, which is frequently mutated in patients with severe lipodystrophy. Lipodystrophy is a metabolic syndrome that is associated with a complete loss of adipose tissue. Whether and how the function of seipin at ER-LD contacts leads to such a devastating pathology is a topic of very active research.

Membrane bridges, essential during biogenesis, often persist throughout the lifetime of LDs (78). However, in a population of LDs, the bridges dissolve and LDs completely detach from the ER. This appears to be a reversible process, as bridges may be reestablished through a process involving components of the coat protein complex I (COPI) coat, which is normally involved in trafficking between the Golgi apparatus and the ER (79).

Besides membrane bridges, other ER-LD tethers have been identified. These appear to be the canonical MCSs and act in parallel with membrane bridges to control different aspects of LD dynamics. Two protein complexes have been implicated in canonical MCSs between the ER and LDs. One of these consists of the ER-localized acyl-CoA synthetase FATP1 and DGAT2, a diacylglycerol acyltransferase. Whereas DGAT2 localizes both to the ER and to LDs, the LD pool specifically interacts with FATP1. Fatty acid activation by FATP1 coupled to DGAT2 acyltransferase activity results in local triglyceride synthesis and LD expansion (Fig. 4) (80).

The small GTPase Rab18 has been identified as a key LD regulator. In a guanosine 5′-triphosphate–dependent manner, Rab18 is recruited to the LD surface and specifically to the ER-associated NAG-RINT1-ZW10 (NRZ) complex and SNARE (soluble N-ethylmaleimide–sensitive factor attachment protein receptor) proteins Syntaxin18, Use1, and BNIP1 (Fig. 4) (81). Consistent with the ER-LD linker activity, depletion of Rab18, NRZ complex components, or associated SNAREs results in diminished LD growth and triglyceride storage. The NRZ complex has long been studied for its function in tethering to Golgi-derived COPI vesicles before their fusion with the ER (82). The connection between NRZ complex tethering to COPI vesicles and LDs is not yet clear. Similarly, SNARE proteins, normally involved in membrane fusion, may act differently in this ER-LD tethering complex. Rab18, NRZ, and associated SNAREs function as an ER-LD tether only in a subset of cell types. Curiously, the ability to assemble into a complex does not correlate with the expression of these proteins, suggesting that additional posttranslational regulatory factors are at play (81). These observations also highlight the often dynamic and context-dependent regulation of MCSs.

Factors and functions of ER-PM contact sites

In all eukaryotes, the ER forms extensive contacts with the PM. Though the PM is not an organelle, ER-PM contacts share some functions (such as lipid trafficking and homeostasis) and factors (such as VAP and OSBP) with organellar MCSs. In yeast, ER-PM MCSs are substantial and cover up to 40% of the cytoplasmic surface of the PM (83, 84) (Fig. 1B). By comparison, ER-PM MCSs in animal cells occupy only ~2 to 5% of the cytoplasmic surface area (3, 85, 86) (Fig. 1B). Despite this difference, ER-PM contacts carry out conserved functions in lipid and Ca2+ homeostasis, which are discussed separately below.

Lipid trafficking at ER-PM MCSs

ER-synthesized phospholipids, such as PI and PS, and sterols are transferred to the PM at ER-PM MCSs. ORP/Osh family members regulate phospholipid homeostasis at ER-PM MCSs. Like other family members, ORP5 and ORP8 contain both an ORD and a PH domain (Fig. 3A) (85). In vitro, the purified ORD of ORP8 can bind and transfer PS or PI4P between proteoliposomes, suggesting that it may also countertransport PS and PI4P at MCSs in cells (85). In animal cells, ORP5 and ORP8 are ER-localized lipid sensors that concentrate at ER-PM MCSs when PM PI4P levels are elevated (85). Because these ORPs are tail anchored into the ER, they do not need to bind to VAP to regulate lipid trafficking (Fig. 3, A and E). In yeast, Osh3 regulates PI4P metabolism at ER-PM MCSs. Osh3 similarly contains a PH domain that binds PI4P on the PM but requires an FFAT motif to bind to the ER-localized yeast VAP orthologs Scs2 and Scs22 to bring Osh3 to the ER. The bridge between PI4P in the PM, Osh3, and Scs2 and Scs22 facilitates recruitment of the ER-localized phosphatase Sac1 to process PI4P at the MCSs (Fig. 3E) (87).

The extended synaptotagmin-like proteins (E-Syts) and their yeast homologs the tricalbins (Tcbs) are another conserved family of ER membrane proteins that regulate ER-PM MCS formation and lipid transfer (Fig. 5) (86, 88, 89). There are three E-Syt paralogs (E-Syt1 to -3) in animal cells and three tricalbins (Tcb1 to -3) in yeast (89). Knockdown of E-Syts decreases the level of ER-PM MCSs in animal cells (86). The E-Syts/Tcbs are anchored to the ER membrane by an N-terminal reticulon-like hairpin transmembrane (TM) domain. Their cytoplasmic C terminus contains an SMP domain and multiple (three to five) C2 domains (86, 90). The SMP domain can dimerize to form a long hydrophobic β-barrel cavity, through which phospholipids may move between membranes (Fig. 5B) (17, 91). With a length of 10 nm, this cavity is consistent with the minimum gaps measured between the ER and the PM (83, 9193). Whether E-Syts selectively transfer lipids in a certain direction remains unclear.

Fig. 5 Calcium-regulated ER-PM MCSs.

(A) Domain organization of proteins found at MCSs that are regulated by Ca2+. All examples are found at ER-PM MCSs. Relevant domains are indicated, including TM, EF-hand (binds Ca2+), C2 (binds Ca2+ and/or lipids), and SMP domains. SAM, sterile α motif; CC1 to CC3, coiled-coil domains 1 to 3; S/P, serine- and proline-enriched region; K, lysine-enriched region. (B) Diagram depicting the localization and oligomerization of ER MCS proteins that respond to calcium store depletion (compare top and bottom panels). The EF-hand domain of STIM1 is sensitive to calcium store depletion from the ER lumen, which leads to STIM1 oligomerization and translocation of STIM1 to ER-PM MCSs via its polybasic domain, allowing STIM1 to bind and activate the Orai1 CRAC channel on the PM. Activation opens the Orai1 channel and funnels Ca2+ from the extracellular space back into the ER through the SERCA channel (not depicted). E-Syt1 is another ER membrane protein that translocates to ER-PM MCSs in response to ER calcium store depletion. E-Syt1 contains five C2 domains. ER calcium store depletion causes cytosolic Ca2+ to increase, the C2A and C2C domains bind this cytosolic Ca2+, and then C2E binds to PI(4,5)P2 at the PM, resulting in E-Syt1 translocation to ER-PM MCSs. E-Syt1 transfers phospholipids at ER-PM MCSs through the SMP domain. TMEM24 is an ER membrane protein with a C2 domain and an SMP domain. TMEM24 transfers PI from the ER to the PM through the SMP domain. However, ER calcium store depletion causes TMEM24 to bind Ca2+, become phosphorylated, and then dissociate from ER-PM MCSs.

Classically, C2 domains are capable of binding lipids and sensing Ca2+. E-Syt1 contains five C2 domains (Fig. 5A), two (C2A and C2C) of which can bind Ca2+ (90). E-Syt1 localization is sensitive to an increase in cytosolic Ca2+, which leads to its accumulation at ER-PM MCSs (86, 94). E-Syt2 and E-Syt3 each contain three C2 domains, of which C2A binds Ca2+ and C2C binds PI(4,5)P2 at the PM (86, 95). When PM PI(4,5)P2 is depleted, E-Syt1 translocates to ER-PM MCSs. Nir2 and VAPs translocate to the same MCSs, presumably to replenish the PI (49, 96). Thus, Nir2 and VAPs appear to function similarly at both ER-PM and at ER-TGN MCSs to regulate PI trafficking (Fig. 3, compare B and E). Depletion of cellular Nir2 decreases PI, PI(4)P, PI(4,5)P2, and PI(3,4,5)P3 levels at the PM (97, 98).

TMEM24 is an ER protein that regulates PI transfer at ER-PM MCSs in response to changes in the cytosolic Ca2+ concentration. This protein’s mechanism of action reveals a link between lipid transfer and insulin secretion. TMEM24 contains an N-terminal TM domain, an SMP domain, a C2 domain, and a PM binding C-terminal domain (Fig. 5A) (99). Overexpression of TMEM24 promotes ER-PM MCS formation, which is dependent on TMEM24’s ability to bind to the PM. TMEM24 preferentially transfers PI from the ER to the PM. TMEM24 knockout cells display decreased insulin secretion upon glucose stimulation. This decrease is directly related to the PI transfer ability of TMEM24 because TMEM24 lacking the SMP domain is unable to rescue insulin secretion deficiency (99). Recruitment of TMEM24 to ER-PM MCSs is regulated by both the Ca2+ concentration and phosphorylation (Fig. 5B). Upon elevation of cytosolic Ca2+, TMEM24 is phosphorylated by protein kinase C and is depleted from the ER-PM MCSs. TMEM24 is recruited back to the PM upon its dephosphorylation by protein serine-threonine phosphatase 2B (PP2B/calcineurin).

Lam1/Ysp1, Lam2/Ltc4/Ysp2, Lam3/Sip3, and Lam4/Ltc3, members of the Lam/Ltc protein family in yeast, were recently shown to localize to ER-PM MCSs (29). Among these, Lam2/Ltc4/Ysp2 and Lam4/Ltc3 directly transfer sterol between proteoliposomes through StART-like domains (29, 100, 101). Lam1/Ysp1, Lam2/Ltc4/Ysp2, and Lam3/Sip3 knockout cells are sensitive to PM sterol depletion, which indicates their involvement in sterol transfer (29). Mutations in Lam/Ltc family members such as Lam1/Ysp1, Lam2/Ltc4/Ysp2, and Lam3/Sip3 result in slowed sterol transfer from the PM to the ER (29). How the directionality of sterol transfer is regulated is not known, but Lam/Ltc proteins appear to play important roles at ER-PM MCSs. In mammalian cells, GRAMD1a and GRAMD2a, Lam/Ltc-related proteins, also localize to ER-PM MCSs (102). However, colocalization experiments showed that GRAMD1a and GRAMD2a label distinct MCSs and are likely to be involved in different functions. Future studies will be required to test whether these proteins are also involved in sterol homeostasis.

Ca2+ regulation at ER-PM MCSs

In animal cells, the ER is a major storage site for Ca2+. When the ER is depleted of Ca2+, it relies on extracellular reservoirs to be replenished. The involvement of ER-PM MCSs in this process was proposed more than 30 years ago (103). The best-studied conduit for the influx of extracellular Ca2+ at ER-PM MCSs is the Orai1 channel (104107). Orai1 is a hexameric Ca2+ release–activated Ca2+ (CRAC) channel on the PM that is required for store-operated Ca2+ entry (108110). Orai1 contains four TM domains with both its N and C termini facing the cytosol. It contains an extracellular glutamate ring to select for Ca2+ and a basic region inside that regulates channel gating (Fig. 5A) (111).

STIM1 is an ER membrane protein that, after ER Ca2+ store depletion, oligomerizes and translocates to the ER-PM MCSs, where it binds and activates Orai1 (Fig. 5) (112114). This interaction guides Ca2+ into the ER lumen through the sarcoplasmic reticulum (SR)–ER Ca2+–adenosine triphosphatase (SERCA) pump. STIM1 has a single TM domain, a cytosolic domain that includes a polybasic region responsible for PM lipid binding, three coiled-coil domains required for Orai1 activation, and a luminal EF-hand domain that senses the ER Ca2+ concentration (107, 113, 115, 116). Upon Ca2+ store depletion from the ER lumen, the EF-hand domain drives a conformational change to initiate STIM1 oligomerization (117).

The STIM1-Orai1 complex can be further regulated by the cytoplasmic EF-hand–containing proteins CRACR2A and CRACR2B. Knockdown of CRACR2A decreases STIM1 recruitment and Orai1 clustering (118). Mutation of the CRACR2A EF-hand domain can lead to constitutive translocation of STIM1 to ER-PM MCSs. Several other regulators of STIM1-Orai1 function have been identified. Junctate is an ER membrane protein that interacts with STIM1 through its C-terminal luminal domain, which also contains a luminal EF-hand domain (119). Junctophilin-4 is a tail-anchored ER membrane protein that interacts with junctate and with the first two coiled-coil domains in the cytoplasmic region of STIM1. These interactions facilitate the translocation of STIM1 to the PM (120). The ER protein TMEM110/STIMATE also binds to STIM1 and promotes STIM1 translocation to ER-PM MCSs, and it is required for Orai1 channel activation (121, 122). There are also negative regulators of STIM1-Orai1 MCS formation and function. SARAF is an ER membrane protein that translocates to STIM1-Orai1 and facilitates STIM1 dissociation from ER-PM MCSs (123). These observations highlight the dynamic nature of MCSs and how they can be finely regulated in response to specific stimuli, such as the Ca2+ concentration.

In skeletal muscle cells, ER-PM MCSs control Ca2+ flux to drive muscle contraction. Specialized membrane structures form in these cells to enhance Ca2+ flux: Transverse tubules are invaginated structures of the PM that are physically opposed to terminal cisternae of the SR (muscle cell ER). These MCSs are composed of RyR1 (ryanodine receptor) on the SR membrane and Cav1.1, a subunit of a voltage-dependent calcium channel, on the PM (124). Upon PM depolarization and action potential generation, Cav1.1 undergoes a conformational change that allows Ca2+ release through RyR1 into the cytoplasm to trigger contraction (125). In cardiac muscle cells, a similar system including RyR2 and Cav1.2 establishes ER-PM MCSs (126). In this case, however, the action potential actually triggers Ca2+ influx into the cytosol from Cav1.2. This Ca2+ influx in turn triggers RyR2-mediated Ca2+ release from the SR. After muscle contractions are terminated, Ca2+ in the cytosol is recycled to the SR through the SERCA pump.


Some of the molecular machineries that regulate membrane tethering have now been identified, and thus MCSs can now be ascribed functions. In recent years, the involvement of MCSs in lipid and ion transport has been confirmed and some of the molecules and mechanisms involved in these processes have been pinpointed. Novel functions for MCSs, such as their crucial role in regulating organelle distribution and division, have also been identified. Moreover, it is becoming apparent that interorganelle communication is highly integrated in and subject to homeostatic regulation. For example, the establishment and regulation of ER-mitochondria and mitochondria-vacuole MCSs are interdependent and appear to respond to nutritional cues (22, 25, 27, 29). Notably, MCSs are linked to human diseases. Among the handful of proteins identified that specifically regulate MCS functions, a high proportion are mutated in a variety of diseases (127129).

References and Notes

Acknowledgments: We thank M. Ladinsky, M. Radulovic, M. West, P. De Camilli, Y. Wu, P. Chitwood, and A. Rowland for images used here. We thank R. Salvador-Gallego for helpful comments on the manuscript. Funding: P.C. was supported by grants from the ERC (starting grant DropFat 309477) and The Wellcome Trust. H.W. was supported by grants from the National Institutes of Health (T32 GM008759 and GM120998). G.K.V. is an HHMI Faculty Scholar. Competing interests: None declared.

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