In vitro differentiation of human pluripotent stem cells (hPSCs) into definitive endoderm (DE) represents a key step towards somatic cells of lung, liver and pancreas. For future clinical applications, mass production of differentiated cells at chemically defined conditions and free of xenogeneic substances is envisioned. In this study we adapted our previously published two-dimensional (2D) DE induction protocol to three-dimensional (3D) static suspension culture in the absence of the xenogeneic extracellular matrix Matrigel. Next, fetal calf serum and bovine serum albumin present in the standard medium were replaced by a custom-made and xeno-free B-27. This yielded in a chemically defined and xenogeneic-free 3D culture protocol for differentiation of hPSCs into DE at efficiencies similar to standard 2D conditions. This novel protocol successfully worked with different hPSC lines including hESCs and hiPSCs maintained in two different stem cell media prior to differentiation. DE cells obtained by our novel BSA-free 3D protocol could be further differentiated into PDX1- or NKX6.1-expressing pancreatic progenitor cells. Notably, upon DE differentiation, we also identified a CXCR4+/NCAM+/EpCAMlow cell population with reduced DE marker gene expression. These CXCR4+/NCAM+/EpCAMlow cells emerge as a result of Wnt/beta-catenin hyperactivation via elevated CHIR-99021 concentrations and likely represent misspecified DE.
Human pluripotent stem cells (hPSCs) possess an unlimited proliferative potential and can be differentiated into all somatic cell types. Owing to these properties they represent an attractive cell source for cell replacement therapies, pharmacological studies on defined somatic cell types and basic research such as the study of human development1.
In vitro, hPSCs can be specifically differentiated towards the definitive endoderm (DE) in a process recapitulating gastrulation2 providing the basis for further specification towards endoderm-derived cell types3. Numerous protocols have been published to differentiate hPSCs into DE cells that differ in composition, concentration and timed application of growth factors (mostly activin A, BMP4, Wnt3A or bFGF) and/or small molecules (mostly glycogen synthase kinase 3 [GSK3] inhibitors [CHIR or BIO] and phosphatidyl-inositol-3-kinase [PI3K] inhibitors4,5,6,7,8,9,10,11,12,13. Commonly, DE differentiation of hPSCs is induced by contemporaneous activation of Wnt/beta-catenin and activin A signaling for one day followed by continuous activation of activin A signaling alone4,8,14. Alternative to Wnt pathway activation, induction of BMP signaling by BMP4 was found to synergistically act with activin A to induce DE formation9,10,15. The efficiency of DE formation in the presence of activin A is higher at lower levels of serum supplementation8. Serum contains insulin-like growth factor (IGF) which inhibits DE differentiation of hPSCs by elevated PI3K signaling12. However, PI3K signaling is required for self-renewal of hPSCs and the removal of serum at the beginning of DE differentiation in combination with activin A is associated with massive cell death13,16,17. Thus, to improve cell survival, DE differentiation media commonly contain the xenogeneic supplements fetal calf serum (FCS), bovine serum albumin (BSA) or B-27TM 16,18,19,20. B-27TM is a serum-free media supplement composed of vitamins, antioxidants, lipids, steroids and trace elements but it also contains BSA21. DE differentiation is commonly initiated from two-dimensional (2D) cultures of adherent cellular monolayers on xenogeneic matrices like Matrigel4,14 or on murine embryonic fibroblasts8. Alternatively, hPSCs can be differentiated towards the DE in three-dimensional (3D) culture as cellular aggregates embedded in extracellular scaffolds, which, however, are often based on Matrigel15,22,23. In a different approach efficient DE differentiation was achieved from singularized hPSCs that initially formed spheroids in suspension culture without addition of exogenous extracellular matrices but the differentiation was performed in the presence of xenogeneic BSA24. A further advantage of culturing hPSCs in 3D is the possibility for scalable expansion in stirred bioreactors enabling the mass production of differentiated cells as desired for medical applications25,26.
To the best of our knowledge, no chemically defined and xenogeneic-free approach for DE differentiation of hPSCs as free-floating suspension culture spheroids in 3D culture has been published until today. Thus, we established static 3D conditions for DE differentiation of hPSCs in the absence of xenogeneic scaffolds and media supplements based on our previously published protocol4. All xenogeneic components were successively replaced or removed without negative effects compared to the original protocol. 3D conditions also supported further differentiation of DE cells towards PDX1-positive pancreatic progenitors (PPs)27 using an adapted, chemically defined and BSA-free media formulation. Additionally, we noticed that DE differentiation conditions gave rise to a subpopulation of CXCR4+ that was also positive for NCAM. These cells could be associated with a decreased expression of important DE marker genes suggesting that DE differentiation protocols should be optimized towards low NCAM-positivity.
hPSCs can be efficiently differentiated into the DE under 3D culture conditions
An overview of the tested culture conditions and their abbreviations is presented in Fig. 1. Our previously published adherent DE differentiation protocol relies on media supplementation with CHIR-99021 (CHIR) and activin A for one day and with activin A on the consecutive days (CA-A protocol4), which will be herein referred to as standard (STD)-2D. This protocol was adapted to a small-scale static suspension culture (STD-3D) to exclude Matrigel (Fig. 2A). Dissociated human embryonic stem cells (hESCs) of the cell line HES3 were cultured in suspension for 24 h until they formed small clusters. Subsequently, randomized differentiation (w/o) or DE differentiation according to the STD-3D approach was induced. The STD-3D protocol resulted in larger and more densely packed clusters compared to the randomized condition (Fig. 2B). Different cell densities (0.25–1.0 × 106 hPSCs inoculated per six well) were tested for the STD-3D culture condition and yielded similar percentages of CXCR4+ cells and rates of proliferation comparable with the STD-2D condition (Fig. 2C,D). Thus, by increasing the inoculum, higher numbers of cells committed to the DE are yielded. As expected, randomized differentiation (w/o) in 2D or 3D culture did not induce significant numbers of CXCR4+ cells (Fig. 2C). Expression analysis of DE marker genes (SOX17, FOXA2) revealed strong inductions only after STD differentiation at all tested cell densities in 3D culture, which were similar to the STD-2D condition. SOX7 gene expression was also comparable between STD-3D and STD-2D conditions, which excluded an extensive differentiation into extra-embryonic endoderm in 3D culture. Pluripotency markers (POU5F1, SOX2, NANOG) showed similar expression levels after four days of differentiation comparing 3D with 2D STD conditions (Fig. 2E). HES3 differentiated in STD-3D showed a distinct co-localization of SOX17 and FOXA2 proteins as a hallmark of proper DE development and FOXA2-positive cells were negative for SOX2 (Fig. 2F). Taken together, the STD-2D protocol for DE differentiation4 of hPSCs could be adapted to static suspension culture (STD-3D) enabling the exclusion of xenogeneic Matrigel without negatively affecting the efficiency or proliferation.
Chemically defined conditions are compatible with DE differentiation in 2D and 3D culture
Differentiation according to the STD protocol was performed in the presence of FCS. In order to establish a chemically defined (CD, Fig. 1) condition, FCS was replaced by our custom made serum-free media supplement called modified (m)B-27 (Table 1)28. This mB-27 is related to the commercially available B-27TM but lacks insulin and BSA. The CD condition was tested in 2D (CD-2D) and 3D (CD-3D) culture for its capability to support DE differentiation of hPSCs. The proportion of CXCR4+ cells and proliferation under CD-2D and STD-2D conditions were comparable for HES3 and HUES8 cells (Figs 3A,B and S1A,B). As shown for HES3, this was independent of the hPSC maintenance medium (Figs 3A and S1A). Similar, during small scale 3D culture, the CD condition supported DE differentiation of HES3 comparable to the STD condition (Figs 3C and S1C). Gene expression of typical endodermal and pluripotency marker genes during CD-3D and STD-3D conditions were comparable (Fig. 3D). Similar results in 3D culture were also obtained for the human induced pluripotent stem cell (hiPSC) line hCBiPSC2 (Fig. 3E,F). Taken together, replacement of FCS by mB-27 enabled chemically defined differentiation of hPSCs in 2D and 3D culture without negative effects on the DE induction.
Establishment of albumin-free DE differentiation in 2D culture
The CD protocol was based on advanced RPMI 1640 (adRPMI) already supplemented with BSA (AlbuMAX™ II). To establish a BSA-free condition (BF), the adRPMI was replaced by RPMI 1640 (RPMI) or MCDB131 (MCDB) supplemented with BSA-free mB-27.
In line with earlier results4,5, the BF-2D condition required a threshold concentration of the Wnt-signaling activator CHIR of at least 2.5 µM during the first 24 h to induce a substantial number of DE cells (Fig. 4A). For all media 5 µM CHIR yielded similar numbers of more than 70% DE committed cells. Interestingly, 2.5 µM CHIR in RPMI (BF-2D) was sufficient to obtain nearly identical numbers of CXCR4+ cells compared to the adRPMI-containing controls (STD-2D and CD-2D), while 2.5 µM CHIR in MCDB131 resulted in higher variations (Fig. 4A). Proliferation rates in RPMI (BF-2D) were similar to the adRPMI-containing controls irrespectively of the CHIR concentration, whereas they were significantly reduced with MCDB supplemented with 5 µM CHIR (Fig. 4B).
We also determined the numbers of CXCR4+/NCAM+ cells (Fig. 4C), which are potentially falsely committed because NCAM is linked to early mesodermal/neuroectodermal differentiation and reorganization of cell assembly29,30,31,32. Under BSA-free conditions with MCDB medium in 2D, all CHIR concentrations induced a prominent CXCR4+/NCAM+ population of 10–20% within the CXCR4+ cells. BSA-free conditions with RPMI and 1 µM or 2.5 µM CHIR led to significantly lower levels of CXCR4+/NCAM+ cells compared with adRPMI-containing controls, while 5 µM CHIR considerably increased the percentage of CXCR4+/NCAM+ cells. Of note, STD-2D and CD-2D conditions with adRPMI and 5 µM CHIR yielded in high levels of CXCR4+/NCAM+ cells (Fig. 4C). Thus, CHIR appears to induce the appearance of CXCR4+/NCAM+ cells in a dose-dependent manner.
To characterize this effect, HES3 cells were differentiated using STD-2D conditions with 5 µM CHIR and then stained for CXCR4, NCAM and EpCAM. CXCR4+/NCAM+/EpCAMlow and CXCR4+/EpCAM+ cells were sorted (Fig. 4D). Remarkably, the CXCR4+/EpCAM+ population expressed higher levels of SOX17 and FOXA2 compared with the pre-sort sample and the CXCR4+/NCAM+/EpCAMlow population (Fig. 4E). Both populations were almost negative for pluripotency genes and expressed the extraembryonic endoderm marker SOX7 at similar levels (Figs 4E and S2). Interestingly, the CXCR4+/NCAM+/EpCAMlow population exhibited a significant expression of the early primitive streak marker MIXL1 but a slightly reduced expression of the anterior primitive streak marker GSC compared with unsorted cells (pre-sort) and CXCR4+/EpCAM+ cells (Fig. S2). CXCR4+/EpCAM+ cells co-expressed SOX17 and FOXA2 on the protein level, while SOX2 was not detectable (Fig. 4F). In contrast, CXCR4− cells expressed similar levels of POU5F1, SOX2 and NANOG as undifferentiated hESCs without significant inductions of differentiation markers (Figs 4E and S2). In line with our recent publication30, this indicates that the CXCR4− population comprised cells that resisted differentiation.
Taken together, the CXCR4+/EpCAM+ population represents the favored DE population due to its higher expression of DE marker genes compared with CXCR4+/NCAM+/EpCAMlow cells. Also RPMI as basal medium prevented the formation of NCAM+ cells more efficiently than MCDB.
Establishment of BSA-free DE differentiation in 3D culture
Based on our previous observations (Figs 4 and S2) RPMI was chosen as basal medium to establish a BSA-free 3D culture (BF-3D). Next, the effect of either 2.5 µM or 5 µM CHIR during the first 24 h on the frequency of CXCR4+/NCAM+ cells was determined. Comparable numbers of CXCR4+ cells (~70–80%) were obtained upon 3D differentiation using BF or STD conditions, independent from the hPSC medium (Fig. 5A). As observed in 2D, also under 3D culture, 2.5 µM CHIR resulted in significantly lower CXCR4+/NCAM+ cells compared to 5 µM CHIR (Fig. 5A). Proliferation rates at BF-3D conditions in the iPS-Brew group were slightly but not significantly lower compared to the STD-3D condition (~4-fold vs. ~4.5-fold, Fig. S3A). However, no significantly different expression levels of SOX17, FOXA2, POU5F1, SOX2, GSC, SOX7 and NANOG were detectable (Figs 5B and S3B). DE specification was additionally verified by immunofluorescence of SOX17 and FOXA2, which was equally distributed within the cell clusters (Fig. 5C). Similar results were also obtained with the cell lines hCBiPSC2 and HUES8 (Figs 5D,E and S3C,D). In summary, BSA-free 3D differentiation conditions with RPMI as basal medium (BF-3D) induces DE differentiation from hPSCs comparable to the STD-3D condition.
BSA-free 3D differentiation can give rise to pancreatic progenitor cells
Next, we determined whether BF-2D/3D culture permits differentiation into PDX1+ pancreatic progenitor (PP) cells using our previously published protocol27 adapted to BSA-free differentiation (Fig. 6A). HCBiPSC2 cells were differentiated under BF-2D into DE resulting in >80% CXCR4+ cells. Subsequent differentiation for four days yielded ~60% PDX1+ PP cells (Fig. S4A). PDX1 expression became strongly detectable and FOXA2 remained strongly expressed throughout the protocol (Fig. S4B). Contemporaneously, expression of POU5F1 decreased, while expression of SOX2 continuously increased during differentiation of DE into PP cells (Fig. S4B).
Next, these conditions were tested in 3D with a different cell line (HES3). From ~70% CXCR4+ cells >50% PDX1+ PP cells were generated after four days of PP induction (Fig. 6B). PDX1, FOXA2, MNX1, SOX2, HNF1B, and HNF6 gene expression was strongly increased or maintained during PP induction (Fig. 6C,D). Similar to 2D culture conditions, POU5F1 expression was very low, (Fig. 6D). Furthermore, co-expression of PDX1 and FOXA2 demonstrated the endodermal origin of the PDX1+ cells, whereas the co-expression of PDX1 with HNF1B revealed foregut identity (Fig. 6E). Finally we tested differentiation of DE cells generated at XF-3D conditions into multipotent pancreatic progenitor cells positive for NKX6.1. Therefore, the resulting clusters were allowed to settle down and treated for the next seven days of differentiation according to the Kieffer-protocol33. Typical pancreatic marker genes including NKX6.1 were strongly expressed upon differentiation (Fig. 6F). Furthermore PDX1- (S3) and NKX6.1-positive cells (S4) were readily detected by immunofluorescence (Fig. 6G). Thus, 3D BSA-free generated DE is capable of pancreatic differentiation.
hPSCs can be differentiated into DE under xenogeneic-free conditions
Our custom-made mB-27 still contained bovine superoxide dismutase and catalase. In order to exclude any xenogeneic compound from the medium, these two enzymes were removed from mB-27 resulting in a xenogeneic-free formulation designated as mB-27XF (Table 1). In addition, activin A was dissolved in pure water without BSA for protein stabilization. This resulted in a 100% chemically defined and xenogeneic-free media formulation for hPSCs differentiation into DE designated XF. XF was compared to STD and BF for HES3 and HUES8 under 2D culture (XF-2D, Fig. S5) and for HES3 under 3D culture (XF-3D, Fig. 7). Under 2D and 3D culture the percentages of CXCR4+ cells and the proportion of unwanted CXCR4+/NCAM+ cells were similar for all tested conditions (Figs 7A,B and S5A,B). We also tested the effects of 1, 2.5, and 5 µM CHIR on the distribution of EpCAM+, NCAM+ and CXCR4+ cells under XF conditions during differentiation and verified CXCR4 gene and protein expression by RT-qPCR and Western Blot (Fig. S6A–C). As described above, higher CHIR concentrations (>2.5 µM) yielded in a NCAM+ cell population slightly expressing EpCAM (EpCAMlow) at the expense of EpCAM+ cells. Analysis of CXCR4 expression in EpCAM+ and NCAM+/EpCAMlow cells revealed that CXCR4 is upregulated in both populations dependent on the CHIR concentration. In NCAM+/EpCAMlow cells, however, CXCR4 is weakly expressed along with lower gene expression of FOXA2 and SOX17 (Fig. 4). Thus, these NCAM+/EpCAMlow/CXCR4low cells likely represent misspecified endoderm cells as a result of Wnt/beta-catenin hyperactivation (Fig. S6A). Further representative flow cytometry dot plots are presented in Supplementary Figs S7 and S8.
The proliferation rates in the 3D culture were unaltered comparing the tested conditions (Fig. 7C). The XF condition did not influence expression levels of SOX17, FOXA2, SOX7, MIXL1 and GSC under 3D or 2D culture compared to the BF and STD conditions. However, expression of pluripotency markers (POU5F1, SOX2, NANOG) appeared to be slightly reduced after four days of DE differentiation with the XF condition (Figs 7D and S5C,D).
Differentiation media for hPSCs are typically not defined and contain xenogeneic components that harbor risks of transmitting pathogenic agents such as zoonotic viruses or mycoplasma to human recipients34,35. Additionally, the incorporation of foreign proteins or glycans36,37 into hPSC-derived lineages may possibly activate the recipient’s immune system and cause graft inflammation or rejection. Removal of xenogeneic compounds from differentiation media would also simplify the governmental registration of stem cell-derived medical products and disburden animals from pain as requested by the 3 R principle38. Furthermore, chemically defined media compositions, in which all ingredients are precisely known, allow standardization with reduced variabilities during cultivation and differentiation. Consequently, the development of chemically defined and xenogeneic-free differentiation protocols for hPSCs is an important step for future clinical application of hPSC-derived somatic cells. To achieve this aim, chemically undefined and xenogeneic components including Matrigel, FCS and BSA were removed step-by-step from our previously published DE and PDX1+ PP differentiation protocols4,27.
In order to eliminate Matrigel, hPSCs were cultured in 3D as free floating spheroids in the absence of exogenous extracellular matrices or scaffolds as described before39 and were then differentiated into DE cells with similar efficiencies as reported for standard 2D culture conditions4. In line with our observations, efficient DE induction in 3D suspension culture of hPSC spheroids has been already described by Pagliuca et al.24, which demonstrates that self-assembled suspension culture spheroids of hPSCs provide an efficient 3D environment without the need for exogenous matrices. The possibility to scale up 3D cultures to controlled, stirred bioreactors25,26 enables the mass expansion and differentiation of hPSCs under defined conditions to obtain abundant cell quantities needed for (pre)clinical applications. Our standard medium for DE differentiation4 contained FCS and BSA. Both are xenogeneic components and can be found in various DE differentiation media8,14,40. Also the recently published 3D differentiation conditions by Pagliuca et al. contained BSA24. It has been earlier shown that replacement of serum by the chemically defined and serum-free supplement B-27TM was compatible with efficient DE differentiation of hPSCs9,10,16. To obtain chemically defined conditions for 2D differentiation into DE, Teo et al. further replaced the Matrigel by fibronectin9,10. However, commercial B-27TM present in these differentiation media contains high concentrations of BSA that is commonly derived by fractionation of serum proteins and it is neither pure nor defined. With the aim to omit BSA and because the commercial B-27TM components’ concentrations are still confidential, we generated a custom-made modified B-27 (mB-27, Table 1)28. This mB-27 is based, with minor modifications, on the formulation of B-27 and its ancestor B-1821,41,42 but lacks BSA and insulin. A further source of BSA in our standard DE differentiation medium (STD) was the adRPMI, which was in a subsequent step replaced by standard, BSA-free RPMI. Both, replacement of B-27TM and adRPMI by mB-27 and RPMI, respectively, in combination with a Matrigel-free 3D culture condition yielded in a chemically defined (CD) and BSA-free (BF) differentiation medium that supported DE differentiation comparable to the standard condition. These findings appear contrary to Wang et al., who could substitute B-27TM with BSA although they found that BSA alone “was not as good as complete B-27”16. Different to Wang et al., our BSA-free mB-27 contained the other ingredients of B-27, including vitamins, antioxidants, lipids, steroids and trace elements. ITS-X (insulin, transferrin, selenite and ethanolamine) was separately supplemented to our differentiation media, which might compensate for the loss of BSA and insulin. Especially insulin is generally considered as a potent mitogen43,44 that might in our approach support cell survival. Accordingly, BSA-free differentiation of hPSCs towards DE has been recently described by Qu and co-workers17 in the absence of cell viability supporting supplements like serum, BSA, B-27TM or insulin by using a cocktail of activin A, WNT3A, BMP4 and bFGF that prevented activin A induced cell death. However, in their chemically defined (CD) 2D culture system it was not clear whether fibronectin/vitronectin was of xenogeneic origin.
Interestingly, we observed in BF and XF conditions less NCAM+ cells within the CXCR4+ population in RPMI medium at lower CHIR concentrations. Typical DE genes were significantly reduced in CXCR4+/NCAM+/EpCAMlow compared with CXCR4+/EpCAM+ cells. Thus, these cells might represent a falsely specified endoderm subpopulation. CXCR4+/NCAM+/EpCAMlow cells strongly expressed MIXL1, whereas GSC was reduced. This indicates that this population could be stuck in a primitive streak pattern or was partially committed towards a mesodermal cell fate. Accordingly, Kempf et al. recently proposed a model, in which the concentration of CHIR and its duration affects primitive streak-like patterning along the anterior-posterior axis influencing cell fate decisions towards DE, cardiac mesoderm or presomitic mesoderm45. Along with Lian et al., who reported that BSA reduces the activity of CHIR during mesodermal differentiation46 and the issue that NCAM-positivity in the CXCR4+ population increased in a CHIR concentration-dependent manner, the CHIR concentration should be carefully determined for BSA-free differentiation conditions. Furthermore, our data suggests NCAM-positivity as a negative marker for DE quality.
DE cells obtained by the newly established BF condition for DE formation in 2D and 3D culture could be further differentiated into PDX1+ pancreatic progenitor (PP) under BSA-free conditions adapted from our recently published protocol27 and into multipotent pancreatic NKX6.1+ progenitor cells according to the Kieffer-protocol33. Actually, 3D culture was shown to be superior to 2D culture for further maturation of DE cells into PDX1+ PP cells and subsequently into insulin producing cells24,47,48, which underlines the importance of scalable 3D cultures. It can be expected that the microenvironment within these 3D aggregates mimics the in vivo distribution and accessibility of morphogens and nutrients and thus may enhance maturation of differentiated progeny49,50. In line with our findings, Pagliuca et al. reported the efficient differentiation of 3D suspension culture spheroids of hPSCs into PDX1+ PP cells and into functional pancreatic beta cells24. In the future fully defined and xenogeneic-free differentiation protocols for the generation of pancreatic beta cells will be required.
As our mB-27 still contained a small amount of bovine-derived proteins (superoxide dismutase and catalase), we also omitted these proteins to obtain a 100% xenogeneic-free formulation designated mB-27XF. This mB-27XF supported DE differentiation to a similar extent as the CD, BF or STD condition, which is in concordance with Wang et al., who reported that antioxidants in B-27TM were redundant during DE differentiation of hPSCs16.
In summary, we describe here the first fully chemically defined and xenogeneic-free differentiation protocol in 3D for various hPSC lines permitting efficient DE differentiation.
Human PSC culture
HESC lines HES3 and HUES8 and the hiPSC line hCBiPSC251 were cultivated as described earlier4,27,30. Briefly, all hPSCs were cultured as colonies on cell culture plastic coated with hESC-qualified Matrigel (Corning, Amsterdam, Netherlands). As cultivation medium mTeSR1 (Stem Cell Technologies, Cologne, Germany) or StemMACS™ iPS-Brew XF (Miltenyi Biotec, Bergisch Gladbach, Germany) was used. Passaging was performed every 5–7 days using a non-enzymatic solution52 or Dispase (5 U/mL) in a ratio of 1:6 up to 1:40 onto Matrigel-coated 6-well plates.
Formulation of modified B-27 (mB-27) and xenogeneic-free modified B-27 (mB-27XF)
Our custom made modified B-27 (mB-27)28 is based on a publication by Roth et al.42. with modifications. Substances are specified in Table 1. 50x stock solutions of modified B-27 (mB-27) or the xenogeneic-free modified B-27 (mB-27XF) were assembled, sterile-filtered and stored at −20 °C in aliquots. After thawing mB-27 or mB-27XF aliquots were diluted to a final concentration of 0.5x in the culture media.
Differentiation of hPSCs as adherent monolayer (2D) was performed as described earlier4 and the media composition will be herein referred to as standard (STD) condition. Briefly, hPSC colonies were dissociated into single cells by Trypsin/EDTA (Biochrom) and centrifuged for 3 min at 300 × g. The pellet was re-suspended in mTeSR1 or iPS-Brew XF containing 10 µM Y-27632 (Selleck Chemicals, Munich, Germany) and a defined number (50,000–70,000 cells/cm2 for HES3 and hCBiPSC2; 70,000–90,000 cells/cm2 for HUES8) was seeded on cell culture dishes coated with used or fresh Matrigel. Cells were allowed to re-attach overnight and differentiation was initiated the following day.
For DE differentiation in static suspension (3D) culture, HES3 or hCBiPSC2 were dissociated into single cells either using 0.5 µM EDTA (in PBS) or gentle cell dissociation reagent (Stem Cell Technologies). A defined cell number was inoculated in Costar® Ultra-Low Attachment 6-well plates (Corning) using mTeSR1 or iPS-Brew XF supplemented with 10 µM Y-27632. Initially tested cell seeding densities ranged from 0.25 to 1 × 106 cells per well. For subsequent experiments 1–2 × 106 cells per well were used as inoculum. HUES8 cells were seeded as small clusters in a similar size as obtained during normal passaging. One full well of a 6-well plate (~2–3 million cells) was re-seeded into 2–3 wells of a Costar® Ultra-Low Attachment 6-well plate. All hPSC lines were cultured o/n or for 24–48 h in maintenance medium to permit aggregate formation before differentiation.
DE differentiation was performed by medium supplemented with 1, 2.5 and 5 µM CHIR-99021 (CHIR) (Biozol, Eching, Germany) and 50 ng/ml activin A (Peprotech, Hamburg, Germany) for 24 h followed by 48–72 h with 50 ng/ml activin A only. Media were changed daily. Randomized differentiation was performed without adding CHIR and activin A. DE differentiation of hPSCs was performed in different basal media. All basal media were supplemented with 1x GlutaMAXTM or 2 mM glutamine plus penicillin/streptomycin (P/S, 10 IU/ml and 70 IU/ml). Instead of advanced RPMI 1640 (adRPMI, Thermo Fisher Scientific) RPMI 1640 (RPMI, Biochrom, Berlin, Germany) was used and supplemented with 0.11 mg/ml sodium pyruvate (Sigma Aldrich, Munich, Germany), 1x ITS-X (Thermo Fisher Scientific) and 1x non-essential amino acids (NEAA, Thermo Fisher Scientific), while MCDB131 additionally contained 1x NEAA, 1x ITS-X and 5.5 mM glucose. Basal media were further supplemented with 0.2% FCS (PAA, Vienna, Austria), mB-27 or mB-27XF and designated according to Fig. 1.
After DE induction pancreatic differentiation for 6 days was performed with minor modifications as earlier described27. The basal medium was changed to DMEM (Biochrom) supplemented with P/S, glutamine, 0.5x mB-27, 1 µM all-trans retinoic acid (Sigma-Aldrich), 0.5 µM LDN-193189 (Sigma-Aldrich), 2 µM IWR-1 (Selleck Chemicals) and 5 ng/ml FGF-7 (ReliaTech, Wolfenbüttel, Germany). Differentiation into NKX6.1-expressing cells was done according to Rezania et al.33. Clusters generated in BF- 3D from HES3 cells were allowed to settle down from day 3–4 and then differentiation was continued in S2 (+2d), S3 (+4d) and S4 (+7d) medium with minor modifications (Pdbu was used instead of TPB).
Flow cytometry and cell sorting
Cells in 2D conditions were washed with PBS and dissociated using Trypsin/EDTA or 0.5 µM EDTA. Clusters from 3D suspension culture were collected in a 15 ml conical tube, centrifuged at 300 × g for 3 min and subsequently dissociated by incubation with 0.5–1 ml collagenase B and occasional tapping (1 mg/mL, diluted in low calcium buffer, Table S1) for 7–10 min. Single cells were then centrifuged at 300x g for 3 min and re-suspended in PBS + 2% FCS.
For flow cytometric staining 1–2 × 105 cells were washed, incubated for 20–60 min at 4 °C with primary conjugated antibodies and washed twice prior to analysis. Staining of intracellular PDX1 was performed with the Foxp3 staining buffer set (Thermo Fisher Scientific). Flow cytometric measurement was performed on a CyFlow ML flow cytometer (Partec, Münster, Germany) and at least 2 × 104 events of each sample were analyzed using the FlowJo software (Ashland, OR, USA). Fluorescence activated cell sorting (FACS) was performed at the central facility of the Hannover Medical School.
The following anti-human Fc-conjugated antibodies were used: CXCR4-PE (FC15004, Neuromics, Minneapolis, USA), CXCR4-APC (130-098-357, Miltenyi Biotec), CD56/NCAM-BV510 (318340, BD Biosciences, Heidelberg, Germany), NCAM-FITC (345811, BD Biosciences), CD326/EpCAM-PE (135905, BioLegend, San Diego, CA, USA) and CD56/NCAM-BV510 (318340, BD Bioscience, Heidelberg, Germany). For staining of PDX1 the primary PDX1 antibody (AF2419, R&D Systems, Minneapolis, USA) was visualized with a secondary AlexaFluor-647-conjugated antibody (Dianova, Hamburg Germany).
Gene expression analysis
Isolation of total RNA was carried out using the peqGOLD Total RNA Kit (VWR International, Erlangen, Germany). CDNA was synthesized from 500–2000 ng total RNA using RevertAid™ H Minus M-MuLV Reverse Transcriptase (Thermo Fisher Scientific) and random hexamer primers. CDNA samples were then diluted to 5–10 ng/µl and measured in a PCR reaction with the GoTaq® qPCR Master Mix (Promega). All reactions were performed by a 2-step PCR in triplicates followed by melting curve analysis on a ViiA7 real-time PCR cycler (Thermo Fisher Scientific). Primer pairs are specified in Table S2. Data normalization was performed with qBasePlus (Biogazelle, Zwijnaarde, Belgium) against the geometric mean of the three housekeeping genes G6PD, TBP and TUBA1A. Analysis of housekeeping gene stability was performed with the geNorm algorithm.
Sorted or dispersed cells were centrifuged for 3 min at 300x g, re-suspended in differentiation medium supplemented with 10 µM Y-27632 and seeded onto Matrigel-coated glass cover slides (SPL Life Sciences, Pocheon, South Korea). After 24 h the cells were fixated for 10–30 min with 4% (w/v) paraformaldehyde.
Clusters obtained by 3D differentiation were collected with a wide-bore tip and washed once with PBS. Fixation was performed as described above. Embedding of the cluster was done in cryomolds (Sakura, Alphen an den Rijn, Netherlands) with Tissue-Tek® O.C.T.™ Compound (Sakura). Subsequently, 5 µm cryosections were cut with a cryostat CM3050 (Leica Biosystems, Nussloch, Germany) and transferred onto superfrost plus slides at −22 °C (Thermo Fisher Scientific).
For immunocytochemistry, cryosections and glass cover slides were washed once with PBS and then blocking was performed for 20 min in PBS plus 0.2% Triton X-100 and 1 mg/ml NaBH4 with 6% BSA or 5% donkey serum (Dianova). Primary and secondary antibodies were diluted in PBS with 0.1% Triton X-100 plus 0.1% BSA. Primary antibodies were incubated for 1–3 h at room temperature or overnight at 4 °C. Secondary antibodies were diluted 1:250–1:500 and incubated for 1 h at room temperature. The following antibodies were used: anti-SOX17 (AF1924, R&D Systems, Minneapolis, USA), anti-FOXA2 (07–633, MerckMillipore, Schwalbach, Germany), anti-SOX2 (sc-17320, SantaCruz, Dallas, USA), anti-PDX1 (AF2419, R&D Systems), anti NKX6.1 (AF5857, R&D Systems), and anti-HNF1b (sc-22840, Santa Cruz). Secondary antibodies were obtained from Dianova conjugated with AlexaFluor or Cy fluorophores. Finally, the slides were mounted with immunoselect anti-fading mounting medium (Dianova) containing DAPI. Stained cells were examined using an Olympus IX81 microscope (Olympus, Hamburg, Germany) and multiple representative pictures were taken of each sample.
Unless stated otherwise values represent mean ± SEM and the number of independent experiments (n) is stated in the figure legend. Statistical analyses were performed using the GraphPad Prism analysis software (Graphpad, San Diego, CA, USA) using ANOVA followed by Bonferroni’s or Dunnett’s post-hoc-test for multiple comparisons.
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This work has been supported by the Deutsche Forschungsgemeinschaft (DFG, German Research Foundation) for the Cluster of Excellence REBIRTH (From Regenerative Biology to Reconstructive Therapy, EXC 62/2). FFRB was funded by the DFG (FOR2509 BU 2920/2-1 and BU 2920/3-1). ON and UD were funded by the DFG (NA 1285/2-1). UD was funded by the internal program (HiLF) of the Hannover Medical School. The skilful technical assistance of J. Kresse, M. Funck and A. Oberbeck is gratefully acknowledged. We would like to acknowledge the assistance of the Cell Sorting Core Facility of the Hannover Medical School supported by the Braukmann-Wittenberg-Herz-Stiftung and the DFG.