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Many cellular responses during development are regulated by interactions between integrin receptors and extracellular matrix proteins (ECMPs). Although the majority of recent studies in human embryonic stem cell (hESC) differentiation have focused on the role of growth factors, such as FGF, TGFβ, and WNT, relatively little is known about the role of ECMP-integrin signaling in this process. Moreover, current strategies to direct hESC differentiation into various lineages are inefficient and have yet to produce functionally mature cells in vitro. This suggests that additional factors, such as ECMPs, are required for the efficient differentiation of hESCs. Using a high-throughput multifactorial cellular array technology, we investigated the effect of hundreds of ECMP combinations and concentrations on differentiation of several hPSC lines to definitive endoderm (DE), an early embryonic cell population fated to give rise to internal organs such as the lung, liver, pancreas, stomach, and intestine. From this screen we identified fibronectin (FN) and vitronectin (VTN) as ECMP components that promoted DE differentiation. Analysis of integrin expression revealed that differentiation toward DE led to an increase in FN-binding integrin α5 (ITGA5) and VTN-binding integrin αV (ITGAV). Conditional short hairpin RNA-mediated knockdown of ITGA5 and ITGAV disrupted hESC differentiation toward DE. Finally, fluorescence-based cell sorting for ITGA5 and ITGAV significantly enriched cells with gene expression signatures associated with DE, demonstrating that these cell surface proteins permit isolation and enrichment of DE from hESCs. These data provide evidence that FN and VTN promote endoderm differentiation of hESCs through interaction with ITGA5 and ITGAV, and that ECMP-integrin interactions are required for hESC differentiation into functionally mature cells.
Human embryonic stem cells (hESCs), with their ability to differentiate into mature cell types, represent a novel system to study human development and disease, and assess safety and efficacy of drugs before clinical trials. In addition, these cells provide an unlimited source of ‘raw material' for regenerative medicine therapies of many incurable diseases, including diabetes and heart disease. However, applications of hESCs in basic research, pharmaceutical, and regenerative medicine are hampered by the lack of well-defined conditions for their directed differentiation and insufficient methods for the purification of lineage-specific cell types from heterogeneous cell populations. Cells derived from definitive endoderm (DE), including those comprising the gut, lung, and pancreas, are of significant interest for many regenerative medicine purposes. Previous studies have identified conditions to generate DE from hESCs through growth factor or small molecule modulation of various soluble signaling pathways including TGFβ, Wnt and AKT/PI3K.1, 2, 3, 4 However, most DE differentiation protocols yield heterogeneous cell populations,4 suggesting that additional factors, such as extracellular matrix proteins (ECMPs), are required for the specification of hESCs to specific fates.
While many studies have focused on the roles of signaling molecules in the differentiation of hESCs, relatively little is known about the role of ECMPs and their interactions with integrins in controlling hESC fate. In mammals, 24 heterodimeric integrin receptors consisting of one of 18 α-subunits and one of 8 β-subunits have been identified. In addition to mediating binding to specific ECMPs, which provide a scaffold for cell growth,5, 6 activation of integrins through interactions with local ECMPs influence cellular processes during embryonic development, including cell survival, proliferation, motility and differentiation. Furthermore, the bidirectional (i.e. inside-out and outside-in) nature of integrin signaling serves as a link between the extracellular and intracellular environments and in turn modulates various downstream signaling pathways and components, such as MEK–ERK, PI3-kinase, and SRC.7 Moreover, many of these downstream pathways have previously been implicated in regulating hESC self-renewal, proliferation, and differentiation.7 Therefore, the study of ECMP-integrin signaling is important in understanding the mechanisms that control hESC differentiation.
Current endodermal differentiation strategies involve guiding hESCs through sequential, staged protocols that mimic early embryonic signaling events known to control primitive streak formation and gastrulation. However, these protocols are often variable and inefficient, yielding only 30–40% cells expressing endodermal markers, such as SOX17. A potential strategy for improving hESC differentiation efficiency involves a two-pronged approach in which hESCs are differentiated to DE and then isolated and enriched using cell surface markers. This strategy not only relies on developing methods for improving the efficiency of DE differentiation from hESCs but also on methods for isolating endodermal cells from heterogeneous differentiating hESC cultures.
The majority of hESC differentiation protocols utilize poorly defined matrices, such as Matrigel (MGEL, BD Biosciences, San Jose, CA, USA), which is a protein mixture produced by EHS mouse sarcoma cells. While such protein extracts provide extracellular components necessary to support cell adhesion, they fail to mimic the specialized microenvironments to which cells are exposed in vivo. In this study, we employed a high-throughput combinatorial ECMP array platform to identify fibronectin (FN) and vitronectin (VTN) as components that improve differentiation of hESCs to DE. Furthermore, we show that the integrin receptors that engage FN and VTN are required for hESC differentiation to DE. Finally, we identified a novel DE integrin ‘signature' that allows for fluorescence-based cell sorting methods to purify endodermal progeny from differentiating hESC cultures. Thus, our studies demonstrate the utility of investigating ECMP-integrin interactions to improve of hESC differentiation.
In an effort to further define and optimize current differentiation protocols of hESCs, we chose to examine the staged differentiation protocol toward pancreatic endoderm (PE, Figure 1a), the first stage of which involves Wnt3a and Activin A treatment to differentiate hESCs to DE,2, 8, 9 as assessed by expression of SOX17, FOXA2, and CXCR4. Although certain hESC lines, such as CyT49, efficiently differentiate into DE,2, 8, 9 other cell lines yield variable amounts of cells expressing DE marker genes, ranging from 32–65% (Supplementary Figure 1), suggesting that additional factors are required for DE differentiation. We sought to investigate to what extent the extracellular milieu, specifically ECMPs, affects endodermal differentiation of three hESC lines, H9, HUES1, and HUES9. We employed a cellular microarray screening platform previously developed in our laboratory.10, 11, 12, 13 All possible combinations of seven ECMPs, collagen I (COL I), collagen III (COL III), collagen IV (COL IV), collagen V (COL V), FN, laminin (LN) and VTN were printed on arrays as described (see Materials and Methods). For comparison we included MGEL (BD Biosciences), which is commonly employed in differentiation protocols of adherent hESC cultures. These arrays were seeded with hESCs, the medium was supplemented with Wnt3a and Activin A to promote endodermal differentiation, and cells were fixed, stained, and imaged for the DE marker SOX17 and DNA (Hoechst Stain 33342) (Figure 1b).
Hierarchical clustering of data sets revealed eight well-defined clusters (Figure 1c; for raw data see Supplementary Table 1), representing ECMP combinations that either promoted high normalized SOX17 expression in all three hESC lines tested (Cluster I), two out of three hESC lines tested (clusters II, III, and IV), one out of the three hESC lines tested (cluster V, VI, VII), or in none of the hESC lines tested (cluster VIII). Analysis of the Pearson correlation coefficient between independent array experiments demonstrated the consistent effects of ECMP combinations within each hESC line but also revealed that the efficiency of some ECMP conditions in promoting DE differentiation was cell line-specific (Supplementary Figures 2a and b). To identify the ECMPs that most effectively promoted DE formation, we performed a full factorial analysis,14 which revealed FN and VTN as the most common DE promoting ECMPs (Figure 1d). Other ECMPs had either no effect (e.g. LN) or negative effects (e.g. COL V) on DE differentiation (Figure 1d).
To confirm that FN and VTN promoted DE differentiation of hESCs we compared their effects to that of MGEL in conventional cell culture formats. HUES9 hESCs were plated on MGEL and the combination of FN and VTN (FN+VTN) and differentiated to DE. Immunofluorescent (IF) staining demonstrated that FN+VTN caused a statistically significant increase in the percentage of cells expressing the DE marker SOX17 (Figure 2a). Moreover, culture on FN+VTN increased the total number of SOX17+ cells, as well as the total cell number (Figure 2b). Flow cytometry revealed that culture on FN+VTN produced an increase in the percentage of cells expressing the DE marker CXCR4 (Figure 2c). Finally, quantitative PCR (qPCR; Figure 2d) of DE markers SOX17, FOXA2, and CXCR4 showed that FN+VTN increased the efficiency of DE differentiation relative to MGEL. We also observed that FN+VTN resulted in increased DE differentiation in two additional hESC lines, HUES1 and H9 (Supplementary Figures 3a and b). Finally, our analysis revealed that FN+VTN increased the efficiency of DE differentiation over that observed when hESCs were differentiated on either ECMP alone (FN, VTN) or on MGEL (Supplementary Figures 3c and d).
To address whether culture on FN+VTN improved differentiation of hESC to more mature endodermal lineages, HUES9 were cultured on FN+VTN and MGEL and differentiated to primitive gut tube (PGT), posterior foregut (PF), and pancreatic endoderm (PE) using previously published protocols (Figure 1a).9 Expression of HNF1β and HNF4α, markers of both pancreas and liver development, was higher in cells differentiated on FN+VTN compared with those differentiated on MGEL (Figure 2e). Expression of the PF marker HNF6 (Figure 2f) and the PE marker PDX1 (Figure 2g) was higher in FN+VTN versus MGEL cultures. These results demonstrate that culture on FN+VTN increases differentiation efficiency toward endodermal lineages.
Having established that FN and VTN were critical ECMP components to promote DE differentiation, we studied the role of integrin receptors in hESC differentiation. HESCs were differentiated to the three germ layers—endoderm, mesoderm, and ectoderm—using previously established protocols2, 15, 16 and analyzed for integrin gene expression. Hierarchical clustering of integrin gene expression revealed specific integrin ‘signatures' that defined each differentiated cell population, with a set of integrin genes (ITGA4, ITGA5 (integrin α5), ITGA7, ITGAV (integrin αV), ITGB2, ITGB5) being upregulated in cells expressing endodermal markers (SOX17, FOXA2, CXCR4) relative to cells expressing either mesodermal (SMA, ACTC1) or ectodermal (SOX1, SOX2) marker genes (Figure 3a). Importantly, among these integrins, ITGA4, ITGA5, ITGAV, and ITGB5 encode subunits of heterodimeric integrin receptors that bind FN and VTN.17, 18, 19, 20, 21
As ITGA5 is required for hESC binding to FN and ITGAV, and ITGB5 are required for binding to VTN,22 we investigated the expression levels of these integrin subunits as hESCs differentiate to DE. A time course of hESCs differentiating to DE revealed that ITGA5 and ITGAV expression is upregulated in a dynamically similar manner to that of SOX17 (Figure 3b). Furthermore, expression of ITGB5 is also upregulated as cells differentiate to DE (Figure 3c), suggesting that hESCs display functional FN and VTN receptors as they differentiate to DE. By contrast, expression of the gene encoding subunits of the LN receptor, ITGA6, is significantly downregulated during endoderm differentiation of (Supplementary Figure 4a).
Using flow cytometry, we confirmed that expression of these three integrin receptors, detected by antibodies that bind ITGA5 (CD49e), ITGAV (CD51), and ITGB5, is increased in DE versus undifferentiated hESCs (Figures 3c and d). In comparison, flow cytometry of ITGA6 and ITGB1, integrin subunits that comprise the LN receptor, were either downregulated or unchanged as hESCs differentiated to DE (Supplementary Figures 4b and c). Taken together, these results suggest that hESCs differentiating to DE significantly upregulate cell surface expression of the subunits that comprise the integrin receptors that bind FN and VTN, the two ECMP components that we identified in our cellular microarray screen to promote DE differentiation.
To determine to what extent expression of the FN and VTN integrin receptors is functionally important during endodermal differentiation, we used a short hairpin RNA (shRNA) approach to knockdown expression of either ITGA5 or ITGAV. HESCs stably harboring doxycycline (DOX) inducible shRNAs (Figure 4a) to either gene—referred to as ITGA5shRNA or ITGAVshRNA hESCs—were treated for 3 days with DOX (1μg/ml) before induction of endodermal differentiation (see flowchart in Figure 4b). DOX treatment of either ITGA5shRNA or ITGAVshRNA hESCs and DE led to a significant increase in expression of red fluorescent protein (Supplementary Figure 5a), the expression of which was driven from the same DOX-inducible promoter as the shRNAs. QPCR analysis confirmed that expression of ITGA5 and ITGAV was significantly decreased in DOX-treated undifferentiated hESC and DE cell populations (Figures 4c and d). Flow cytometry revealed that cell surface protein expression of ITGA5 and ITGAV was decreased in DOX-treated DE cell populations (Figures 4e and f). We confirmed that DOX treatment of ITGA5shRNA hESCs had no effect on ITGAV gene (Supplementary Figure 5b) or cell surface protein expression (Figure 4e). Similarly, DOX treatment of ITGAVshRNA hESCs had no effect on ITGA5 gene (Supplementary Figure 5c) or cell surface protein expression (Figure 4f). Additionally, DOX treatment alone was not responsible for decreases in integrin expression as DOX treatment of wild-type hESCs had no effect on ITGA5 or ITGAV expression (Supplementary Figure 5d). Importantly, expression of the endodermal marker genes, SOX17, FOXA2, and CXCR4, was significantly decreased in hESC-derived DE in which ITGA5 or ITGAV expression was knocked-down by the shRNAs (Figures 4c and d). Furthermore, flow cytometry revealed that CXCR4 cell surface expression was almost absent in DOX-treated DE cells (Figures 4e and f). IF analysis demonstrated that knockdown of either ITGA5 or ITGAV resulted in a significant reduction in SOX17 or FOXA2 staining at DE (Figures 4g and h). These results suggest that expression of FN and VN integrin receptors ITGA5 and ITGAV is necessary for differentiation of hESCs to DE.
As increases in ITGA5 (CD49e) and ITGAV (CD51) expression correlate with endodermal differentiation, we tested whether cell separation by flow cytometry for these integrin receptors could be employed to isolate cells with endodermal gene expression signatures (Figure 5a). HESC-derived DE was sorted for ITGA5 (CD49e) and ITGAV (CD51) (Figure 5b) and analyzed for expression of SOX17 (Figure 5c and Supplementary Figure 6). This analysis revealed that double-positive ITGA5(CD49e)+/ITGAV(CD51)+ cells expressed higher amounts of the DE maker gene SOX17 than single-positive ITGA5(CD49e)+/ITGAV(CD51)− or ITGA5(CD49e)−/ITGAV(CD51)+ cells or double-negative ITGA5(CD49e)−/ITGAV(CD51)− cells (Supplementary Figure 6). Furthermore, expression of additional DE marker genes FOXA2 and CXCR4 was increased in double-positive cells compared with double-negative cells (Figure 5c). We next investigated if double-positive ITGA5(CD49e)+/ITGAV(CD51)+ were capable of differentiating into more mature endodermal progeny. Double-positive ITGA5(CD49e)+/ITGAV(CD51)+ and double-negative ITGA5(CD49e)−/ITGAV(CD51)− cells were replated after cell sorting and differentiated to PGT. Subsequent gene expression analysis revealed that expression of HNF1β and HNF4α, markers of pancreas and liver development, were enriched in the ITGA5(CD49e)+/ITGAV(CD51)+ population relative to the ITGA5(CD49e)−/ITGAV(CD51)- population (Figure 5d). Therefore, cell enrichment strategies for ITGA5 (CD49e) and ITGAV (CD51) significantly increase the yield of cells with DE gene expression patterns from differentiating hESC cultures.
In addition to exploring the effects of exogenous ECMP on DE formation, we wanted to investigate the role of endogenous ECMP production and remodeling during endodermal differentiation. To that end, we measured endogenous ECMP gene expression of hESCs differentiated to DE (Figure 6a). In general, expression of endogenous ECMPs increased as cells differentiated to DE on MGEL and FN+VTN substrates. Specifically, we observed a statistically significant increased expression of several COLs (COL4A2, COL5A1, COL6A1, COL7A1, COL8A1, COL11A1, COL12A1), FN1, VTN, and LN subunits (LAMA3, LAMAB1, LAMAB3) as hESCs differentiated to DE.
Previous studies have shown ECMP degradation and proteolysis have a critical role in endoderm development and cell differentiation.23, 24 Therefore, we wanted to determine if ECM remodeling and degradation through the action of matrix metalloproteinases (MMPs) was required for differentiation of hESCs to DE. While expression of MMP 1, 3, 7, 10, 12, or 13 was not detected in hESCs or DE (data not shown), we observed a statistically significant increased expression of MMP 2, 8, 9, 14, and 15 during DE differentiation (Figure 6b). To test whether MMP activity was required for DE differentiation, we treated cells with broad-spectrum small molecule inhibitors of MMP (Baritasmat, Marimastat, CP471474) and the glycoprotein tissue inhibitor of metalloproteinases (TIMP1) during DE differentiation. Gene expression analysis of DE markers SOX17, FOXA2, and CXCR4 revealed that MMP inhibition does not inhibit formation of DE (Figure 6c). Therefore, even though we observe changes in the composition of the extracellular environment during DE differentiation, including endogenous deposition of ECMPs and secretion of MMPs, pharmacological inhibition of MMPs does not appear to disrupt endodermal differentiation of hESCs.
The selection of the appropriate extracellular matrix is critical for hESC self-renewal and proliferation,13, 22 and here we show that the ECMP composition also potently influences hESC differentiation to DE. By systematically screening hundreds of ECMP combinations, we identified two ECMPs, FN, and VTN, which significantly improve the efficiency of hESC differentiation to DE, thereby overcoming the need for poorly defined and non-human biological components, such as MGEL, in the manipulation of hESCs.
While certain studies have explored the role of physical properties of the microenvironment, including three-dimensional culture25 and substrate rigidity,26 we focused our analysis on the role of the ECM in differentiation and found that changes in the composition of the ECM profoundly affected the differentiation of hESCs to endoderm. It is particularly important to note that the effects of the growth factors inducing DE (Wnt3a and Activin A) are significantly influenced by ECMP composition. Our results suggest that appropriately defining the ECMP substrate in addition to the soluble signaling molecule environment is critical for improving the differentiation of hESCs to specific lineages.
The differentiation of hESCs to DE resembles that of primitive streak formation and gastrulation where cells invaginate and generate mesendodermal cell populations. These movements of epiblast cells require several growth factor signaling pathways, as well as an ECM. In this process the ECM does not merely function as a scaffold through which cells migrate. Rather, as determined by computational and optical methods, migrating cells move in concert with the ECM with little cellular movement relative to the ECM.27 This study supports the notion that the ECM has a more active role in development than previously appreciated and further underscores the importance of performing screens to identify optimal ECM compositions that promote specific developmental processes.
Consistent with our identification of FN and VTN as critical components that promote endodermal differentiation in cell culture, several studies in model organisms have provided compelling evidence that these ECM components are critical constituents of the microenvironment guiding the processes of primitive streak formation and gastrulation. For example, injection of agents that disrupt integrin-FN interactions, such as RGDS peptides or antibodies and Fab' fragments directed against FN, into chick embryos perturb gastrulation movements.28 Such microinjection experiments in frog embryos have led to similar observations.29 Mice lacking FN-binding integrins die early in development and fail to extend the anterior–posterior axis.30, 31, 32 Earlier defects, such as during gastrulation, are likely not uncovered due to rescue by maternally contributed FN message and protein. Together, countless studies in a variety of model organisms support the concept that the ECM, and specifically FN, has an important and instructive function in early embryogenesis. However, it should be stressed that in our studies only the initial matrix compositions are specified. Cells exposed to these ECMPs remodel the underlying matrix and begin secreting their own ECMPs. Even so, the observed cellular responses are a result of their exposure to the initial composition of the ECM.
Previous studies demonstrated that undifferentiated hESCs express a variety of integrins, including integrins α1, 2, 3, 5, 6, 7, 11, E, and V, and β1, 2, 3, and 5.33, 34, 35 We extended these studies by examining integrin gene expression in undifferentiated hESCs and hESC differentiated to each of the three primitive germ layers—endoderm, mesoderm, and ectoderm. This analysis revealed a specific integrin ‘signature' that was unique to each of these cell populations. Specifically, we found that ITGA5 and ITGAV gene expression was highly upregulated and ITGA6 expression was significantly downregulated in the endodermal lineage. Treatment with specific integrin blocking antibodies revealed that blocking ITGA5 impaired adhesion to FN, blocking ITGAV and ITGB5 reduced the binding to VTN, and blocking ITGA6 inhibited binding to LN.22 Furthermore, ITGA6 binding to LN has been implicated as having a critical role in the self-renewal and maintenance of pluripotent hESCs.36 In this study, we implemented an inducible shRNA system to demonstrate that knockdown of ITGA5 and ITGAV impaired endoderm formation. During development, integrin switching, rapid changes in the proportions of specific integrin subunits expressed at the cell surface, has been implicated as a mechanism that regulates cell differentiation.37, 38 Together our results suggest a possible mechanism in which hESCs differentiating to DE undergo an integrin switch from an ITGA6 signature which favors binding LN, and thereby maintenance of pluripotency, to an ITGA5 and ITGAV signature, which allows for interaction with FN and VTN and subsequent differentiation to DE.
Mouse models have been used extensively to interrogate integrin expression and functionality during embryonic development.37, 39, 40 Interestingly, mouse embryos stained for different integrin subunits at E6.5 revealed that Itga5 expression was mainly restricted to endoderm,41 which is consistent with the ITGA5 expression patterns that we identified in hESC-derived DE. Furthermore, Itga5 and ItgaV are widely expressed during development of many organs of endodermal origin, such as the pancreas, liver, and lungs.42, 43, 44 Knockout of Itga5 or ItgaV resulted in embryonic lethality,32, 45 while tissue specific deletion of Itga5 or ItgaV resulted in vasculature and neuronal defects.18, 32, 45, 46 Therefore, the novel findings presented here, which demonstrate knockdown of ITGA5 and ITGAV in hESCs impaired endoderm formation in hESCs, suggests that similar integrin knockdown strategies in hESCs can be used to interrogate the function of various integrin-ECMP interactions during the earliest stages of human development.
Current hESC differentiation protocols are insufficient in creating pure cell populations, which are required for understanding human development and creating disease relevant models. Therefore, developing sorting strategies for flow cytometry-based isolation of highly pure populations of cells from differentiating hESC cultures is of particular interest.47, 48, 49, 50 By investigating the role of integrin-ECMP interactions in hESC differentiation to DE, we identified a panel of novel surface integrins, ITGA5 (CD49e) and ITGAV (CD51), that allow for the FACS-based isolation of endodermal cells. In the future, similar integrin ‘signatures' could be developed that would permit the isolation of lineage committed cells from mixed differentiated hESC cultures.
Arrayed cellular microenvironment (ACME) slides were fabricated as previously described. Briefly, glass slides were cleaned, silanized, and then functionalized with a polyacrylamide gel layer. Stock solutions of human COL I, COl III, COl IV, COl V, FN, LN (Sigma-Aldrich, St Louis, MO, USA) and VTN (EMD-Millipore, Billerica, MA, USA) were prepared in an ECMP-printing buffer (200mM acetate, 10mM EDTA, 40% (v/v) glycerol, and 0.5% (v/v) triton-X-100 in MQH2O, with pH adjusted to 4.9 using glacial acetic acid). All ECMP combinations were premixed at a constant protein concentration of 250μg/ml in polypropylene 384-well plates. SMP 3.0 spotting pins (Telechem Corp., Atlanta, GA, USA) were washed with 90% ethanol. All printings were performed with a SpotArray 24 (Perkin-Elmer, Waltham, MA, USA) at room temperature (RT) with 65% relative humidity. The printing conditions were a 1000-ms inking time and a 250-ms stamping time. To control for variability, each ECMP combination was printed in replicates of five spots. Each spot had a diameter of 150–200μm, and neighboring microenvironments were separated by a center-to-center distance of 450μm. A single slide carried 6400 spots arranged in sixteen 20 × 20 matrices so that one slide carried 1280 unique ECMP conditions. Slides were inspected manually under a light microscope for consistent and uniform ECMP deposition. ECMP spotting was characterized using general protein stain (SYPRO Ruby gel stain, Life Technologies, Carlsbad, CA, USA) or protein specific antibodies (Sigma-Aldrich) as previously described. A single slide from each batch of printed arrays was seeded with HEK-293 (2.5 × 105 cells per slide) to ensure that each ECMP spot supported cell adhesion.
The following media were used: mouse embryonic fibroblast (MEF) (1 × high glucose DMEM, 10% fetal bovine serum (FBS), 1% (v/v) -glutamine penicillin/streptomycin); H9/WA09 hESCs (1 × DMEM-F12, 20% (v/v) Knockout Serum Replacement, 1% (v/v) non-essential amino acids, 0.5% (v/v) glutamine, 120μM 2-mercaptoethanol (Sigma-Aldrich)); HUES1 and nine hESCs (1 × Knockout DMEM, 10% (v/v) Knockout Serum Replacement, 10% (v/v) human plasmanate (Chapin Healthcare, Anaheim, CA, USA), 1% (v/v) non-essential amino acids, 1% (v/v) penicillin/streptomycin, 1% (v/v) Gluta-MAX, 55μM 2-mercaptoethanol (Sigma-Aldrich)). All media components are from Life Technologies unless indicated otherwise. H9, HUES9, and HUES1 hESC lines were maintained on feeder layers of mitotically inactivated MEFs (2 × 104/cm2; Millipore). All hESC cultures were supplemented with 30ng/ml bFGF (Life Technologies). MEF-CM was produced by culturing the appropriate hESC medium on MEFs for 24h. Cells were routinely passaged with Acutase (Millipore), washed, and replated at a density 4.25 × 104/cm2).
Before their use, slides were soaked in PBS while being exposed to UVC germicidal radiation in a sterile flow hood for 10min. Before seeding onto the ACME slides, hESCs were cultured for two passages on MGEL (BD) with MEF-CM supplemented with 30ng/ml bFGF to remove residual feeder cells. HESCs were then acutase-passaged onto the ACME slides (5.0 × 105 cells per slide) and allowed to settle on the spots for 18h. Array slides were then gently washed twice with RPMI (Life Technologies) to remove cell debris and residual hESC media. The medium was then changed to RPMI supplemented with 1% (v/v) Gluta-MAX and 100ng/ml recombinant human Activin A (R&D Systems, Minneapolis, MN, USA). Cells were cultured for 3 days, with FBS concentrations at 0% for the first day and 0.2% for the second and third days. Cultures were supplemented with 30ng/ml purified mouse Wnt3a for the first day.
H9, HUES9 and HUES1 were cultured on MGEL (BD) with MEF-CM supplemented with 30ng/ml bFGF for 2 passages to remove residual MEFs. The human ECMP-coated plates were prepared by coating tissue culture plates in the ECMP (diluted in 10mM acetic acid) overnight, followed by air drying. 10μg of total protein was plated per cm2 of culture dish surface. Human ECMP-coated plates were used immediately after air drying. HESCs were passaged at a density of 2.5 × 105cells/ml onto human ECMP or MGEL-coated plates in order to achieve confluency the following day. HESCs were then gently washed twice with RPMI (Life Technologies) to remove cell debris and residual hESC media. The medium was then changed to RPMI supplemented with 1% (v/v) Gluta-MAX and 100ng/ml recombinant human Activin A (R&D Systems). Cells were cultured for 3 days, with FBS concentrations at 0% for the first day and 0.2% for the second and third days. Cultures were supplemented with 30ng/ml purified mouse Wnt3a for the first day. For further differentiation to PGT, the medium was changed to RPMI with 0.2% FBS supplemented with 50ng/ml recombinant human KGF (R&D Systems) for 3 days. For differentiation to PF endoderm, the medium was changed to DMEM with 1 × B27 (Life Technologies), 50ng/ml recombinant human Noggin (R&D Systems), 0.25μM KAAD-cyclopamine (Tocris Biosciences, Bristol, UK), and 2μM retinoic acid (Sigma-Aldrich) for 3 days. Finally, for differentiation to PE the medium was changed to DMEM with 1 × B27 (Invitrogen) supplemented with 50ng/ml recombinant human Noggin, 50ng/ml recombinant human KGF, and 50ng/ml recombinant human EGF (R&D Systems) and for 3 days.
To differentiate hESCs to ectoderm we modified several previously published protocols.9, 15, 51 To initiate ectoderm differentiation, hPSCs were cultured on MGEL in MEF-CM supplemented with 30ng/ml FGF2. Cells were then detached with treatment with acutase (Millipore) for 5min and resuspended in ectoderm embryoid body (EB) media (10% FBS/1% N2/1% B27/DMEM:F12) supplemented with 5μM Y-267632 (Stemgent, Cambridge, MA, USA), 50ng/ml recombinant mouse Noggin (R&D Systems), 0.5μM Dorsomorphin (Tocris Biosciences). Next, 7.5 × 105 cells were pipetted to each well of several 6-well ultra low attachment plates (Corning, Lowell, MA, USA). The plates were then placed on an orbital shaker set at 95r.p.m. in a 37°C/5% CO2 tissue culture incubator. The next day, the cells formed spherical clusters and the media was changed to ectoderm EB media without FBS supplemented with 50ng/ml recombinant mouse Noggin and 0.5μM Dorsomorphin. The media was subsequently changed every other day. After 5 days in suspension culture, the EBs were then transferred to a 10-cm dish coated (3 × 6 wells per 10cm dish) with growth factor reduced MGEL (1:25 in KnockOut DMEM; BD Biosciences) for attachment. The plated EBs were cultured in ectoderm EB media without FBS supplemented with 50ng/ml recombinant mouse Noggin and 0.5μM Dorsomorphin for an additional 3 days. To differentiate hESC to mesoderm, we modified several previously published protocols.16, 52 To initiate mesoderm differentiation, hPSCs were cultured on MGEL in MEF-CM supplemented with 30ng/ml FGF2 until they reached 60% confluency. Cells were then gently washed with RMPI media to remove residual hESC media. The medium was then changed to RPMI supplemented with 0.5% B27 supplement. Cells were cultured for 5 days supplemented with 100ng/ml recombinant human Activin A (R&D systems) for the first day, and 10ng/ml BMP4 for days 2–5.
ACME slides and cultures were gently washed twice with staining buffer (PBS w/ 1% (w/v) BSA) before fixation. Cultures were then fixed for 15min at RT with fresh paraformaldeyde (4% (w/v)). The cultures were washed twice with staining buffer and permeabilized with 0.2% (v/v) triton-X-100 in stain buffer for 20min at 4°C. Cultures were then washed twice with staining buffer. Primary antibodies were incubated overnight at 4°C and then washed twice with stain buffer at RT. Secondary antibodies were incubated at RT for 1h. Antibodies used are listed in Supplementary Table 2. Nucleic acids were stained for DNA with Hoechst 33342 (2μg/ml; Life Technologies) for 5min at RT. Imaging of was performed using an automated confocal microscope (Olympus Fluoview 1000 (Olympus America, Center Valley, PA, USA) with motorized stage and incubation chamber). Images of ACME slides were quantified using GenePix software (MDS Analytical Technologies, Molecular Devices, Sunnyvale, CA, USA). Quantification of additional images was performed by counting a minimum of nine fields at × 20 magnification.
Cells were dissociated Acutase (Millipore) for 5min at 37°C, triturated, and passed through a 40μm cell strainer. Cells were then washed twice with FACS buffer (PBS, 10mM EDTA, and 2% FBS) and resuspended at a maximum concentration of 5 × 106 cells per 100μl. One test volume of antibody was added for each 100μl cell suspension (Supplementary Table 2). Cells were stained for 30min on ice, washed, and resuspended in stain buffer. Cells were analyzed and sorted with a FACSCanto or FACSAria (BD Biosciences). FACS data was analyzed with FACSDiva software (BD Biosciences). For replating experiments, DE cells were stained with CD49e and CD51 and sorted into FACS buffer with 10nm Y27632 (Stemgent). Sorted cells were replated at a density of 1 × 105cells/cm2 in stage 2 PGT media with 10nM Y27632 and differentiated for 4 days.
Before endoderm differentiation, hESC were treated with 0.5μM Batimastat (Tocris Biosciences), 0.5μM CP471474 (Tocris Biosciences), 0.5μM Marimastat (Tocris Biosciences), or recombinant 130nM human TIMP1 for 48h. The medium was then changed to RPMI supplemented with 1% (v/v) Gluta-MAX and 100ng/ml recombinant human Activin A (R&D Systems). Cells were cultured for 3 days, with FBS concentrations at 0% for the first day and 0.2% for the second and third days. Cultures were supplemented with 30ng/ml purified mouse Wnt3a for the first day. MMP inhibition continued throughout the duration of endoderm differentiation.
RNA was isolated from cells using TRIzol (Life Technologies), and treated with DNase I (Life Technologies) to remove traces of DNA. Reverse transcription was performed by means of qScript cDNA Supermix (Quanta Biosciences, Gaithersburg, MA, USA). QPCR was carried out using TaqMan probes (Life Technologies) and TaqMan Fast Universal PCR Master Mix (Life Technologies) on a 7900HT Real Time PCR machine (Life Technologies), with a 10-min gradient to 95°C followed by 40 cycles at 95°C for 15s and 60°C for 1min. Taqman gene expression assay primers (Life Technologies; Supplementary Table 3) were used. Gene expression was normalized to 18S rRNA levels. Delta Ct values were calculated as Cttarget−Ct18s. All experiments were performed with three technical replicates. Relative fold changes in gene expression were calculated using the 2−ΔΔCt method.53 Data are presented as the average of the biological replicates±S.E.M.
The lenti constructs that were used to generate the inducible shRNA lines were obtained from Open Biosystems (ITGA5:1334333, ITGAV:133468). High titer lenti virus was produced as previously described.54, 55 HUES9 hESCs were infected overnight with lenti virus and treated with puromycin (0.5μg/ml) for 2 weeks.
For statistical analysis, unpaired t-test were used and a P-value <0.05 was considered statistically significant. All values were presented as mean±S.E.M. unless otherwise noted. For each ACME experiment, the ratio (Ri) of the log2 of the SOX17 signal and the DNA signal was calculated for each spot. From this a differentiation z-score was calculated for each spot ZDIF=(Ri−μDIF)/σDIF, where Ri was the ratio for the spot, μDIF was the average of the rations for all spots on each array, and σDIF was the S.D. of the ratios for all spots on each array. Differentiation z-scores from replication spots (n=5 per ECMP condition) were averaged for each ECMP condition on the array. The replicate average z-scores were displayed in a heat map with rows corresponding to individual ECMP conditions and columns representing independent array experiments. For each array experiment, all columns were mean-centered and normalized to one unit S.D. The rows were clustered using Pearson correlations as a metric of similarity.56 All clustering was performed using Gene Cluster.56 The results were displayed using a color code with red and green representing an increase and decrease, respectively, relative to the global mean. All heat maps were created using Tree View.56 Normalized effect magnitudes were calculated as previously described.14
DAB was supported by funding from the UCSD Stem Cell Program and a gift from Michael and Nancy Kaehr. This research was supported in part by the NIDDK Beta Cell Biology Consortium (5U01DK089567-02) and the California Institute for Regenerative Medicine (RB1-01406).
DAB and KW designed the experiments. DAB, CP, and NK performed the experiments. DAB, CP, and KW analyzed the results. DAB and KW wrote the manuscript.
The authors declare no conflict of interest.
Supplementary Information accompanies the paper on Cell Death and Differentiation website (http://www.nature.com/cdd)
Edited by R De Maria