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The formation of epithelial tissues requires both the generation of apical-basal polarity and the co-ordination of this polarity between neighboring cells to form a central lumen. During de novo lumen formation, vectorial membrane transport contributes to formation of a singular apical membrane, resulting in contribution of each cell to only a single lumen. Here, from a functional screen for genes required for 3D epithelial architecture we identify key roles for Synaptotagmin-like proteins 2-a and 4-a (Slp2-a/4-a) in generation of a single apical surface per cell. Slp2-a localizes to the luminal membrane in a PI(4,5)P2-dependent manner, where it targets Rab27-loaded vesicles to initiate a single lumen. Vesicle tethering and fusion is controlled by Slp4-a, in conjunction with Rab27/Rab3/Rab8 and the SNARE Syntaxin-3. Together, Slp2-a/4-a co-ordinate the spatiotemporal organization of vectorial apical transport to ensure only a single apical surface, and thus formation of a single lumen, occurs per cell.
Epithelia represent the most fundamental tissue in metazoa, forming complex layers of cells such as the skin, or kidney tubules. The epithelial plasma membrane is divided into two domains: apical and basolateral, separated by cellular junctions, dependent on the asymmetric delivery and segregation of membrane proteins and lipids1,2. Such plasma membrane asymmetry allows the formation of a central lumen, and hence the evolution of specialized functions for different metazoan tissues3. Epithelial cells create lumens via an array of morphogenetic mechanisms. Despite this diversity, a series of common molecular events create biological tubes: vectorial transport to a nascent apical domain, de novo apical plasma membrane biogenesis, and secretion and expansion of the luminal space4,5. Transport of apical proteins to the initial site for apical-membrane formation, at which the Par3–aPKC–Cdc42 polarity complex is established, is controlled by a Rab11a/8a GTPase cascade and its effectors, the exocyst and Myo5B6,7. At the lumen, phosphoinositide asymmetry is concomitantly established with PI(4,5)P2 and PI(3,4,5)P3 localizing to, and specifying, the apical and basolateral domains, respectively8,9. How vectorial exocytic transport is coordinated and directed so that each cell has a single apical initiation site, and thus the tube has a single lumen, however, is largely unclear. Similarly, how such machineries are controlled at the transcriptional level during morphogenesis of epithelial tissues is poorly understood3.
Here, we report a functional screen for regulators of 3-dimensional (3D) epithelial polarity using MDCK cyst cultures, based on transcriptional, RNAi, and morphogenetic analysis.
Synaptotagmin-like proteins (Slp1–5) are a family of Rab effectors involved in regulated exocytosis10. Slps harbour a N-terminal Rab-binding domain (also called Slp-homology-domain SHD), and tandem C-terminal C2 domains involved in Ca2+ and phospholipid binding, and function in tethering secretory vesicles to the plasma membrane11. In D. melanogaster, a single divergent Slp paralogue, Bitesize (Btsz), functions in epithelial polarization12, though whether mammalian Slps function in polarity generation is unknown.
We demonstrate that Slp2-a and related family member Slp4-a function in distinct, but complimentary, steps of apical transport to form a lumen de novo. Slp2-a controls positioning of Slp4-a/Rab27-positive vesicles to target exocytosis to a single PI(4,5)P2-enriched lumen. Slp4-a regulates the tethering of these vesicles, through the association with the apical SNARE Syntaxin-3, to mediate vesicle delivery to the lumen. Thus, through a functional, multi-step screen we have identified a previously uncharacterized mechanism for co-ordianated vectorial transport, crucial to form a single apical domain.
We performed a multi-step, functional screen for regulators specifically of 3D epithelial architecture and morphogenesis. We first conducted a microarray-based differential expression analysis comparing the transcriptome of MDCK cells undergoing apical-basolateral polarization either in traditional monolayer culture (‘2D’), or as 3D cysts grown in basement membrane extract (‘3D’), wherein MDCK self-assemble to form a 3D monolayer (Figure 1A). Notable transcriptional differences were observed during 3D morphogenesis with 1597 upregulated, and 1304 downregulated probes detected (Figure S1). To prioritize functional analyses, upregulated genes were subjected to bioinformatic analysis to reconstruct potential molecular pathways and known components of epithelial polarization. Using this approach, a set of 99 upregulated genes was selected for secondary validation by qPCR (Figure S2, Table S1). Finally, 47 candidate genes were targeted via siRNA, including the known polarity regulators Claudin-2 (CLDN2) and Wrch-1 (RHOU) as internal controls13,14(Figure 1B; Table S2). We found a set of 14 genes previously uncharacterized to be required for this process (Figure 1B–C, green stars; Table S3). These included tight and adherens junctions, Rho GTPases, lipid signaling, and membrane trafficking proteins.
To analyze a possible relevance of these genes in vivo, we analyzed whether this gene set was downregulated in human cancers, suggesting an importance in the maintenance of a differentiated epithelial phenotype in vivo (Figure 1D). Notably, renal, breast, and skin cancers presented with the strongest downregulation of this gene set. We selected one of these genes, SYTL2 (Slp2-a), which was significantly downregulated in several epithelial cancer datasets (Figure 1E), to characterize its role in lumen formation.
The mammalian Slp family has been shown to regulate primarily Rab27-dependent membrane trafficking and secretion15–17, but their function in mammalian epithelial morphogenesis is unknown. We confirmed that Slp2-a protein levels were upregulated in 3D compared to 2D cultures (14-fold enrichment at 72h; Figure 2A), and qPCR data (Figure S2). Next, we characterized Slp2-a localization in MDCK cysts. Upon plating MDCK into 3D, the apical Podocalyxin (Podxl) localized to the peripheral surface of early aggregates, before it is internalized into vesicles and delivered to the contact between two cells, where lumen is formed de novo7,9,18. In early aggregates, Slp2-a localized to the plasma membrane, enriched at cellular junctions (Figure 2B, Table 1). A pool of Slp2-a became apparent on internalized Podxl-positive transcytosing vesicles near the cell-cell contact (Figure 2B, 16–20h). Upon lumen formation (24–48h), Slp2-a localized to the apical membrane (Figure 2B, 48h).
Slp2-a depletion perturbed 3D lumen formation in a dose-dependent manner (Figure 2C–E), without affecting cell polarity in cells growing in monolayers (Figure S3A). Slp2-a depletion results in abnormal morphology with multiple small lumens (Figure 2D), and the accumulation of Podxl (Figure 2D), that we identify as transcytotic vesicles (Figure S5C). Notably, stable expression of RNAi-resistant human Slp2-a (Slp2-aGFP; Figure 2F) completely rescued lumen formation and morphogenesis of cysts with endogenous Slp2-a KD (Figure 2G,H). Moreover, these results indicate that Slp2-a is the predominant variant required for epithelial morphogenesis in 3D-MDCK19.
Slp-family proteins share an amino-terminal Rab27-binding domain (the ‘Slp-homology domain’, SHD), a linker region, and two c-terminal tandem C2-domains (phospholipid and/or protein interaction sites)20,21. Slp2-a could potentially therefore connect Rab-GTPases and phosphoinositides during lumen formation9,22,23. To elucidate the control of Slp2-a localization, we analyzed Slp2-a domains during cyst formation. In early aggregates, the C2-domains localized to the plasma membrane and to cell-cell junctions, but not to Podxl-vesicles (Figure 3A, S4B, 12–20h). Once lumens formed, C2A/B fragment localized exclusively to the apical membrane (Figure 3A, S4B, 24–48h). In contrast, the SHD fragment was predominantly cytoplasmic, and partially localized to Podxl-vesicles in early aggregates and subapically in mature cysts (Figure 3A, bottom panels). Deletion of the C2 domains (GFP–ΔC2A/B) resulted in a similar localization to the SHD, while linker region was cytoplasmic (Figure S4). These results suggest that while the SHD binds to apical vesicles, the C2-domains target Slp2-a to membranes.
Notably, the distribution of the C2-domains resembles PI(4,5)P2 localization during cyst formation9. Furthermore, Slp2-a, and paralogues, bind selectively to PI(4,5)P212,17, although it could bind also to phosphatidyl-serine (PS)16. We found that C2-domains bound specifically to PIP2 species, but not to PS (Figure 3C). Furthermore, Lact-C2-GFP, a probe for PS, presents non-polarized membrane localization in cysts (Figure S4E). Given the established role of PI(4,5)P2 in apical membrane specification9, and higher cellular abundance24, we reasoned that PI(4,5)P2 may target Slp2-a to plasma membranes. During cyst formation Slp2-a and PI(4,5)P2 co-localized at the plasma membrane, becoming progressively enriched to the lumen in morphogenesis (Figure 3D). Furthermore, both PI(4,5)P2 and Cherry-Slp2-a disappeared rapidly from the apical membranes upon Ionomycin treatment, which causes membrane PIP-depletion25 (Figure 3E, Video S1). Taken together, these results confirm that Slp2-a requires the C2 domains for PI(4,5)P2 binding and apical membrane localization, whereas the SHD region targets Slp2-a to apically destined vesicles (Figure 3F).
Nearly all described functions of mammalian Slps required the SHD domain21. In contrast, bitesize, the sole Slp paralogue in Drosophila does not require a Rab-binding domain for epithelial morphogenesis12 (Figure S5B), suggesting Rab-Slp interactions may be dispensable for epithelial polarity. To address this possibility, we expressed the epithelial bitesize protein (Btsz2-GFP) and an SHD-deleted Slp2-a mutant (GFP-Slp2-a-ΔSHD). Importantly, neither GFP-Slp2-a-ΔSHD nor Btsz2-GFP was able to rescue the defects caused by endogenous Slp2-a KD (Figure 4A–C, Figure S4B). These results reveal that the SHD region is required for epithelial morphogenesis in MDCK cysts.
To determine which Rab-GTPase interactions are required for Slp2-a function we analyzed Rabs that interact with other Slps10. Slp2-a bound to Rab3b, Rab8a, Rab27a, and to a lower extent Rab3a (Figure S5A). While Rab8a/b are required for cyst formation7,18, only KD of both Rab27a/b strongly perturbed lumen formation (Figure 4D–G), confirming partial isoform redundancy noted from knockout mice26. In contrast, while Rab3a-d isoforms are expressed in MDCK (data not shown), silencing of Rab3b was sufficient to disrupt cyst formation (Figure 4D–G), suggesting Rab3b may have subtle non-redundant roles in apical transport27,28, and epithelial polarity. These results suggested that Slp2-a could mediate the targeting of apical vesicles loaded with Rab27a/b, Rab3b and/or Rab8a/b.
Next, we generated Slp2-a-SHD mutants to disrupt interaction with specific Rabs based on structure of the Slp2-a/Rab27 interaction20. Introduction of a V18A mutation in Slp2-a completely abolished interaction with Rab3b and Rab8a, while preserving Rab27a binding; E11A/R32A mutations also disrupted the binding to Rab27 (Figure 4G). Although both mutants retain apical localization (Figure 4I, Table 1), GFP-Slp2-a-V18A, but not E11A/R32A, completely rescued the Slp2-a KD phenotype (Figure 4H–I, Figure S5F). Together, these data indicate that although Slp2-a can bind multiple Rabs, Rab27a/b is necessary and sufficient for Slp2-a function in lumen morphogenesis.
Next, we analyzed Rab27 localization. Before lumen formation, GFP-Rab27a colocalized with Podxl and Slp2-a in vesicles transcytosing to the lumen (Figure 4J, top and middle panels; Figure S5C). Once lumen initiation was completed, Rab27a localized to a subapical compartment, while Slp2-a localized apically (Figure 4J, bottom panels; Figure S5C–E). Finally, Slp2-a KD caused the scattering of Rab27a vesicles close to the plasma membrane (Figure 4K, bottom panels). Thus, Slp2-a is required to localize Rab27a. Taken together, these results indicate that Slp2-a binds to Rab27a-loaded apical vesicles and targets them to initiate the lumen.
In addition to Slp2-a, mammalian cells express four additional Slp-family proteins (Slp1–5), and 4 closely related Slac2s (Slp homologue lacking C2 domains)10. To determine whether additional Slps proteins function in epithelial polarization, we analyzed their expression during lumen formation. Notably, while Slp2-a was the sole Slp upregulated in 3D at early times (Figure 5A, 3D-14h), Slp1 and Slp4-a were upregulated at later times (Figure 5A, 3D-36h).
In contrast to Slp1, Slp4-a silenced cysts presented acute defects with formation of multiple lumens and internal vesicles (Figure 5B–C). In addition, Slp4-a KD did not affect polarity or ciliogenesis in monolayers (Figure S3A–B). Moreover, we observed Slp2-a is specifically induced before Slp4-a in 3D cultures (Figure 5D), suggesting Slp2-a is required earlier than Slp4 in lumenogenesis.
We next examined the localization of Slp4-a. Endogenous Slp4a/b and GFP-Slp4-a associated with apical membranes at all stages of polarization (Figure 5E, S6D), thus presenting a different localization pattern than Slp2-a (see Figure 3, Table 1). Next, we examined Slp4-a domains in cysts. The C2 domains (C2A/B), either alone or in tandem, localized to apical and basolateral plasma membranes (Figure 5F, left panels; Figure S6E, Table 1), suggesting they confer non-specific plasma membrane localization. In support of this, GST-Slp4-a C2 domains bound promiscuously to PI(4,5)P2 and PI(3,4,5)P3 (Figure 5G–H, S6C). In contrast, the C2A domain of Slp2-a bound specifically to PI(4,5)P2 and localized apically (Figure S4D), suggesting that only Slp2-a is able to tether Rab27 vesicles to apical PI(4,5)P2-enriched plasma membrane. Together, these data highlight a requisite of the SHD-linker region for apical targeting of Slp4-a, representing a major difference with Slp2-a, and suggesting non-redundant roles for Slp2-a and Slp4-a in lumen formation.
Slp4-a functions in docking of secretory granules with the plasma membrane, a function modulated by the SHD region, which interacts with Rab3, Rab8, and Rab27 family members10. Therefore, we examined Rab binding contribution to Slp4-a function.
To elucidate the role of Rab binding we examined the ability of SHD mutations to bind to Rab27/3/8 and to rescue the phenotype of endogenous Slp4-a KD (Figure 6A–B)29. In contrast to apical WT-Slp4-a, removal of the Rab-interacting region of Slp4-a (ΔSHD) resulted in both cytoplasmic and non-polarized membrane localization of Slp4-a (Figure 6C, Figure S6E, Table 1), similar to W118S-Slp4-a (no-Rab-binding) expression (Figure 6A–C, Figure S6F, Table 1). Uncoupling of Slp4-a from Rab3b (V21A) resulted in subapical localization (Figure 6C, Figure S6F). In contrast, co-uncoupling of Rab8 and Rab3b (I18A) resulted in the targeting of a pool of Slp4-a to the basolateral membrane, in addition to subapical vesicles (Figure 6A–C, Figure S6F, Table 1). While WT-Slp4-a was able to rescue endogenous Slp4-a KD, none of the Rab-binding mutants were able to restore lumen formation (Figure 6B–C, Table 1). These results indicate that Rab27, Rab8 and Rab3 binding are required for Slp4-a localization and function. The different localization of the mutants also suggests that Rab27 is required for Slp4-a targeting to vesicles, Rab8 would be necessary to exclude Slp4-a from the basolateral membrane, and Rab3 may be important for subsequent Slp4-a transport to the lumen initiation membrane.
Next we analyzed the role of phospholipid binding for Slp4-a, using a phospholipid-uncoupled mutant (K>Q16). Slp4a-K>Q localized to subapical puncta of apical membranes (Figure S6G, Table 1), and conferred a partial rescue to morphogenesis (Figure 6B), suggesting that while the C2 domains can confer membrane localization, interaction of Slp4-a with additional factors (Rabs and SNARE complexes) may partially compensate for the lack of C2 domain function.
Slp4, in contrast to others Slps, binds to SNARE proteins by its linker domain30,31. To analyze SNARE-binding, we generated a chimeric construct of Slp4-a bearing Slp5 linker domain (Slp4-5-4) that was unable to bind Syntaxin3 (Stx3) (Figure 6D). Slp4-5-4 showed a subapical and basolateral localization, and failed to rescue lumen formation upon endogenous Slp4-a KD (Figure 6E–F, S6I, Table 1), suggesting an important role for Stx3 binding to Slp4-a. Next, we mapped the Stx3 binding domain of Slp4-a, and identified aa 305–354 to be essential for Stx3 binding (Figure S6H). Consistently, expression of a construct lacking aa 305–354 of Slp4-a (GFP-Slp4-Δ305–354) also failed to localize to the apical plasma membrane and to rescue lumen formation upon endogenous Slp4-a KD (Figure 6E, S6J, Table 1).
Stx3 functions as a critical apical SNARE32. In cysts, GFP-Stx3a colocalized with Slp4-a at the nascent luminal membrane (Figure 6G). Notably, Stx3 KD resulted in disruption of lumen formation and the redistribution of a pool of GFP-Slp4 to the basolateral membrane (Figure 6I–K), a similar localization observed upon removal of Stx-binding region of Slp4-a (Figure S6I–J). In contrast, Slp4-a KD did not disrupt the apical localization of Stx3 (Figure 6H). These data suggest that Stx3 association with Slp4-a, by interaction with the linker domain, directs recruitment of Slp4-a to apically destined vesicles, and initiation of de novo lumen formation.
Our data thus far indicate that Slp2-a and Slp4-a function in distinct, non-redundant steps in Rab-dependent transport to form the lumen. We thus examined their localization during lumen formation. In early aggregates, Slp2-a localized mainly to cell-cell junctions, while Slp4-a colocalized with Podxl at the cell-ECM interface (Figure 7A, 16h, top panels, Figure S7C). As internalized Podxl transcytosed to the cell-cell contact, Slp4-a co-localized to these vesicles, whereas Slp2-a was mainly at the cell-cell junctions (Figure 7A, 20h, Figure S7C). Finally, Slp2-a/4-a co-localization was evident once lumens formed (Figure 7A, 24h, Figure S7C).
Next we tested if their activities were mutually dependent. KD of Slp2-a caused the scattered distribution of small Podxl-vesicles near the plasma membrane, with the latter pool only colocalizing with Slp4-a-GFP (Figure 7B), which had also been redistributed to the plasma membrane. In contrast, Slp4-a KD cysts presented with clusters of Podxl-vesicles (Figure 7C), but GFP-Slp2-a localized normally to cell-cell contacts, suggesting that Slp2-a localization and function is independent of, or upstream to, Slp4-a. Furthermore, overexpression of GFP-Slp2-a forced endogenous Rab27a and Slp4a mis-recruitment to cell-cell contacts at early time points (Figure 7D), while the converse effect of GFP-Rab27a on Slp2-a was not observed (not shown). These results suggest that Slp2-a functions to regulate the positioning of Rab27 vesicles upstream of Slp4-a-mediated vesicle docking, thus controlling the position of the apical membrane and subsequent lumen.
To test this hypothesis, we silenced Slp2-a and Slp4-a alone or together (Figure 7E–G). Strikingly, we observed that while Slp4-a KD induced accumulation of Podxl vesicles close to the membrane (Figure 7E, middle panels), Slp2-a KD cysts possessed some cells simultaneously developing more than one apical membrane (Figure 7E, top panels, quantification 7G). And while dual KD cysts presented a mixture of both phenotypes (Figure 7E, bottom panels), they perturbed single lumen formation to a level resembling that of Slp4-a KD alone, supporting the notion that Slp4-a functions downstream of Slp2-a (Figure 7F). Although cysts with multiple lumens have been observed previously upon KD of trafficking proteins, the KD of Slp2-a is unique in that this is the first time, to our knowledge, that a cell can participate simultaneously in the generation of multiple luminal surfaces.
In summary, these results indicate that Slp2-a and Slp4-a form part of a core apical transport pathway that controls the positioning of Rab27a/b vesicles, and their subsequent Rab8/Rab3b/Stx3-dependent fusion with the apical plasma membrane, respectively, to form a single PI(4,5)P2–enriched apical membrane and lumen during de novo apical domain biogenesis (Figure 7H).
One of the central, unsolved questions in epithelial biology concerns how apical-basolateral polarity is coordinated between neighboring cells to form a common, single luminal region. Making use of the fact that MDCK can undergo polarization into either in 2D or 3D, we have uncovered a gene set that specifically facilitates transition to 3D architecture. Interestingly, most of this gene set is downregulated in some glandular epithelial cancers, indicating potential clinical relevance in maintaining a polarized phenotype (Figure 1).
During the development of 3D polarity, apical membrane components are delivered to the site for lumen initiation, between neighboring cells to initiate a luminal space de novo7,33. What had remained unclear, though, was how this trafficking pathway was organized to direct vectorial transport to a singular position, thus allowing formation of a single apical membrane per cell. Here, we have identified a molecular pathway specifically upregulated during 3D morphogenesis that controls the formation and positioning of a single apical membrane per cell, through the complementary functions of Slp2-a and Slp4-a (Figure 7H). We demonstrate that Slp2-a controls the clustering of apically destined vesicles through the interaction with Rab27a/b and the association with PI(4,5)P2 at the nascent apical membrane. Subsequently, Slp4-a acts as an effector of Rab27a/b, Rab8a/b and Rab3b on vesicles, to couple the vesicles to Stx3-mediated fusion events at the plasma membrane to create the lumen. Inhibition of this Slp2-a/4-a pathway perturbs this transport and ultimately causes formation of multiple apical membranes. These data support our model that Slp2-a and Slp4-a function in a spatiotemporal cascade to control vectorial apical transport (Figure 7H), a fact supported by their sequential transcriptional upregulation during cyst formation.
How may Slp2-a/4-a coordinate vectorial transport to a single lumen? In non-polarized cells, both Slp2-a and Slp4-a are considered as negative regulators of secretion, based on the fact that their overexpression attenuates secretory granule release15–17,29,34. Indeed, Slp4-a can interact with the closed (non-fusion-forming) confirmation of SNARE complexes31. To this end, transient overexpression of Slp2-a or Slp4-a in the presence of endogenous protein consistently reduced single-lumen-formation rates (Figure S7A–B), a trend which could be strongly reversed by expression of SHD-deleted Slp2-a/4-a, suggesting they may act as negative regulators of vesicle trafficking. However, Slp2-a/4-a are also clearly required for single lumen formation, thus suggesting a scenario where, rather than being considered as ‘negative’ or ‘positive’ regulators of exocytosis, Slp2-a/4-a act as molecular traffic wardens34, controlling vectorial exocytosis through ensuring vesicles dock and fuse only at singular membrane domains to form a single, co-ordinated luminal space between neighboring cells.
In summary, we identified, for the first time, a transcriptionally regulated molecular pathway that controls the formation of a single apical surface per cell, addressing a major, long-term unanswered question in cell biology. Study of the responsible transcriptional machinery for lumenogenesis in vivo presents as a major future challenge to both cell and developmental biology.
A microarray-based differential expression analysis was conducted using the Affymetrix Canine Genome 2.0 platform. MDCK type II cells were grown in P100 dishes to form 2D monolayers or 3D cysts in Matrigel (at 105 cells/ml). Total RNA was isolated at 36h and purified using RNeasy (Qiagen) and 5 µg of RNA were submitted for microarray analysis (n=3) using Affymetryx platform at Parque Científico de Madrid (Cantoblanco, Madrid). The raw microarray data is deposited in NCBI GEO (Gene Expression Omnibus), accessible online by this number GSE32495. A LiMMA (FDR<0.05) analysis revealed a set of 1597 upregulated genes. The resulting data set was analyzed to select a maximum of 100 upregulated genes for qPCR validation. To further examine this selection, we used bioinformatic/bibliographic searches to analyze all 1597 upregulated genes for previously published references into function (RIFs), and Gene Ontology (GO) terms from human or mouse orthologues in NCBI databases. We selected genes with GO terms, or RIFs related to processes or mechanisms involved in changes in cell signaling, cell architecture and organ morphogenesis.
The list included a comprehensive list of GO terms related to cell polarity, membrane trafficking, cell-to-cell junction assembly and remodeling, cell cycle regulation, cytoskeleton regulation, and cell division, among others (complete list on demand). The second selection approach used STRING software (http://string-db.org/) to select genes interacting with pathways previously known to have a role in epithelial architecture or morphogenesis. From the resulting list, we selected 99 genes based on bibliographic research and designed specific primers to perform qPCR analysis validation of their overexpression pattern in 3D cyst formation.
After qPCR validation, a stealth®-siRNA library was custom designed to target 47 validated candidate genes (Invitrogen, USA). To perform the siRNA screening, MDCK cells were transfected with siRNA using Nucleofector-II (Lonza). Transfected cells were cultured for 2 days in 3D conditions and RNA extracts were analyzed by RT-PCR to check silencing efficiency (Table S2). Gene expression silencing was verified by RT-qPCR procedures (SYBR RT-PCR premix, Applied Biosystems), normalizing to GAPDH or HPRT expression. For functional analyses, transfected MDCK cells were grown for 3 days in Matrigel to form cysts, and lumen formation efficiency was quantified by confocal microscopy using the following markers to assess lumen formation: localization of the apical protein podocalyxin (Podxl), integrity of the actin cytoskeleton (F-actin; Phalloidin), adherens junctions (β-catenin), tight junctions (ZO-1), nuclei (DNA; DAPI).
Antibodies against α-tubulin (1:5000; T9026, Sigma-Aldrich), Rab27a (1:200; R4655, Sigma-Aldrich), GFP (1:500; a5455, Invitrogen), Rab8a (1:1000, 610845, BD Biosciences), mRFP/Cherry (1:250; PM005, MBL), Syntaxin-3 (1:200; Ab4113, Abcam), GST (1:5000; sc138), β-catenin (1:1000, sc7199), and Slp4-a (1:100; 34448) from Santa Cruz Biotechnology were commercial primary antibodies. The Slp2-a antibody was raised as a polyclonal serum against the Slp2-a SHD region and used as previously described35. Podxl antibody was a gift from the Ojakian laboratory (State University of New York Downstate Medical Center, Brooklyn, NY). ZO-1 (1:500; R4076) from DSHB. Peroxidase-conjugated donkey anti–mouse IgG and anti– rabbit IgG were used as secondary antibodies for Western blots (Jackson ImmunoResearch Laboratories, Inc.). Alexa Fluor–conjugated secondary antibodies (Alexa Fluor 405, 488, 555, or 647; Invitrogen) and TOPRO-3 or DAPI (for nuclear/DNA staining) were used in microscopy protocols.
Slp2-a and Slp4-a (full length and mutants) were cloned into either pEGFP-C1/C2 or pmCherry-C1 vector (Takara Bio Inc.). Human Slp4-a cDNA template was from Open Biosystems (Thermo Fisher). Plasmids kindly provided were: pEGFP-Slp1 (J. Peränen, U. Helsinki, Finland), pEGFP-STX3a (M. ter Beest, U. Chicago, IL), pENTR-Rab3a/b/c/d (Bruno Goud, Institut Curie, Paris, France), pEGFP-Rab8a (María Montoya, CNIC, Madrid, Spain) and pEGFP-Rab27a/b (WT and DN) (John Hammer, NIH, USA). For bacterial expression of GST-tagged full length and mutant proteins, Slp2-a and Slp4-a were cloned into pGEX-4T1 vector (Promega) or pDEST15 (Invitrogen). Slp2-a (V18A, E11A/R32A16), and Slp4-a (V21A, W118S, I18A, K>Q17,29) mutants were generated using Quickchange XL (Stratagene). To disrupt C2 domain-lipid interactions in Slp4-a (C2AB K>Q; K410Q, K412Q, K416Q, K564Q, K566Q, K571Q), three of four Lysine residues of the PIP-binding consensus motifs present in Synaptotagmin and Synaptotagmin-like familiy C2 domains [K(K/R)KTXXK(K/R)] were mutated to Glutamine in both C2 domains, as reported for Slp2-a16. To disrupt Stx interactions in Slp4-a, the linker domain of Slp4-a was substituted for the linker domain of Slp5 (GFP-Slp4-5-4a) by subcloning the chimeric SHDSlp4-linkerSlp5 fragment from a previously reported Slp4-5-4b construct30 into a GFP-Slp4-C2AB plasmid. T7-tagged Slp4-a, Slp4-5-4a, and Slp4-a linker were used for in vitro syntaxin-3 binding experiments as previously reported31,30. The Slp4-a construct lacking the Stx3-interacting aminoacids of the linker domain (Δ305–354) was cloned into pEGFP-C1. All constructs were verified by sequencing.
T23-MDCKII and MDCKII cells were grown as described previously9. MDCK cells stably expressing GFP-Slp2-a (Full-length and mutants), Cherry-Slp2-a, GFP-Rab27a, GFP-Rab8a, and PLCδ-PH-GFP were made by cotransfection with the blasticidin-resistant gene and selected for 10 days with 0.5 µg/ml blasticidin. MDCK cells stably expressing GFP-Slp1, Stx3-GFP or GFP-Slp4-a (Full-length and mutants) were selected for 10 days using G418 (0.5 mg/ml). Cysts and transwells cultures were prepared as described before36
Immunofluorescence of cysts was as previously described9, 36. Per condition, >100 cysts/experiment were analyzed. For early time points, cysts were grown up to 24h and two/three-cell stage cysts were clasified based on Podxl and β-catenin localization either as “formed preapical-patch” or “presence of internal vesicles”.
RNAi sequences and qPCR primers are listed in Supplementary Table 3. Briefly, 25 nucleotide stealth siRNA duplexes targeting mRNA sequences of canine Slp2-a were purchased from Invitrogen. Sequences were submitted to BLAST search to ensure targeting specificity. For siRNA transfection, MDCK cells were trypsinized and then nucleofected (Lonza) with siRNA duplexes or scrambled siRNA. After 24-h incubation, cells were resuspended and plated in 12-well plates and in coverglass chambers coated with matrigel to grow cysts. Total cell lysates from 3D cultures were analyzed by Western blotting or quantitative real-time PCR (Q-PCR) to confirm siRNA efficiency.
Stable RNAi was achieved by viral shRNA, essentially as previously described7. In all instances KD was verified by western blot or qRT-PCR procedures (Brilliant-II SYBR Green Kit, Agilent, Santa Clara, CA), normalizing to GAPDH expression. RNAi and qRT-PCR primers are presented in Supplementary Table 3. STX3 shRNA is as described37. SLP1 and SLP4-a shRNA lentiviruses were constructed in pLKO.1-puro according to the Addgene pLKO.1 protocol (www.addgene.org) using iRNAi (www.mekentosj.com), and target sequences were based on an (AA)N19 algorithm. RNAi sequences were submitted to BLAST (NCBI) to verify target specificity, with SLP4-a sequences targeting common regions to Slp4a and Slp4b transcripts. GFP-tagged human SLP4, which is not targeted by anti-canine shRNA, was used for Slp4-a KD and rescue experiments.
Lentivirus production was performed essentially as previously described7. For lentivirus transductions, subconfluent MDCK cultures, 1–4 h after plating, were infected with virus-containing supernatants for 12–16 h at 37°C. Viral supernatants were then diluted 1:1 with growth medium, cultured for a further 48 h. Transduced cells were selected by passage into appropriate antibiotic-containing medium. Puromycin (5 µg/ml), and blasticidin (12.5 µg/ml) were used.
Single lumen formation was quantified as described7. The percentage of cysts with a single lumen was determined, and normalized to control cysts as 100%. Values are mean ± SD from ≥3 replicate experiments, with n ≥100 cysts/replicate. For qRT-PCR experiments, percentage remaining mRNA in each KD condition was normalized to HPRT level, and represented as a percentage of control (scramble shRNA) mRNA levels. Significance was calculated using a paired, two-tailed Student’s t-test. *p < 0.05, ** < 0.001.
Rab GTPase-Slp protein pulldowns were performed using HEK293T cells overexpressing GFP-tagged Rab proteins, and GST-tagged Slp proteins. HEK293T expressing GFP-tagged Rab proteins were lysed in 0.1% SDS, 1% Triton X-100, 0.5 mM DTT, and 1× TBS buffer with protease inhibitor cocktail and sodium orthovanadate. Cell debris and nuclei were removed by centrifugation at 14,000 × g for 2 min at 4°C, and lysates were precleared and incubated in rotation with 100 ng relevant GST protein–loaded beads (GE Amersham) for 30 min, using GST alone as control, in presence of non-hydrolizable GTP analog (Sigma). Beads were centrifuged and washed five times, dried using aspiration, and resuspended in 40 µl Laemmli buffer before Western blot analysis.
Co-immunoprecipitation assays in COS-7 cells were performed essentially as described previously30,31. In brief, pEF-Flag-Stx3, pEF-Flag-Munc18-2, pEF-T7-Slp454 (a linker domain-swapping construct between Slp4a and Slp530 or pEF-T7-Slp4a linker deletion constructs (i.e., Linker, amino acids (AA) 144–354; F1, AA144–240; F2, AA215–304; and F3, AA272–354) were transfected into COS7 cells by using Lipofectamine 2000 (Invitrogen) according to the manufacturer’s instructions. Cells were harvested 48 h after transfection and homogenized in a homogenization buffer30,31. After removal of insoluble materials by centrifugation, cell lysates were obtained. The associations between T7-tagged proteins and FLAG-tagged Stx3/Munc18-2 in the cell lysates were evaluated by immunoprecipitation using anti-T7 tag antibody-conjugated agarose beads (Merck Biosciences) as described previously38. Immunoreactive bands were visualized with horseradish peroxidase (HRP)-conjugated anti-T7 tag antibody (1:10,000 dilution; Novagen, 69522-4) and HRP-conjugated anti-FLAG tag M2 antibody (1:10,000 dilution; Sigma-Aldrich, A8592) and detected by enhanced chemiluminescence (ECL; GE Healthcare). For Rab-GTPase co-immunoprecipitation assay was performed as previously described22.
A solution of 1 µg/ml of purified protein (GST, GST-Slp2-a, GST-Slp4-a) was incubated with PIP-strip membranes according to the instructions of the manufacturer (Echelon Bioscience). Lipid beads (Echelon) prepared with different phosphoinositides or phosphatidylserine were incubated with 2 µg of purified GST-C2A or GST-C2B from Slp2-a or Slp4-a, washed five times, dried and resuspended in 100 µl sample buffer before Western blot analysis. ECL blotting of membranes was developed by immunostaining with an anti-GST antibody (Sigma-Aldrich) and HRP-conjugated donkey anti-mouse IgG (Jackson Immunoresearch).
We thank Carmen M. Ruiz-Jarabo for comments on the manuscript, and members of Martin-Belmonte lab for discussion. We thank M. ter Beest J. Peränen, and K. Simons for generous gifts of reagents, and the Mostov lab for kind assistance. Work supported by grants from Human Frontiers Science Program (HFSP-CDA 00011/2009), Marie Curie (IRG-209382), MICINN (BFU2008-01916), (BFU2011-22622) and CONSOLIDER (CSD2009-00016) to FM-B; by NIH R01DK074398, R01AI25144 and R01DK91530 to KM, and The March of Dimes Basil O’Connor Starter Research Award to PRB. AER-F is recipient of a JAE fellowship, from CSIC; MG-S is recipient of a FPI fellowship, from MICINN; and IB-R is recipient of an AECC fellowship. An institutional Grant from Fundación Ramón Areces to CBMSO is also acknowledged.
The authors declare that they have no competing financial interests
AUTHOR CONTRIBUTIONSM.G.S, A.E.R.F, D.M.B., S.V. and , F.M.-B. designed the experiments. M.G.S, A.E.R.F, D.M.B., S.V, T.S., I.B.R:, I.B., A.D., N.S., K.Y., and C.L.S. did the experimental work. M.G.S, A.E.R.F, D.M.B. K.E.M., and F.M.-B. analysed the experiments. P.R.B and M.F. provided reagents. F.M.-B., D.M.B. M.G.S, and A.E.R.F wrote the manuscript.