Efficient generation of cardiomyocytes from human pluripotent stem cells is critical for their regenerative applications. Microgravity and 3D culture can profoundly modulate cell proliferation and survival. Here, we engineered microscale progenitor cardiac spheres from human pluripotent stem cells and exposed the spheres to simulated microgravity using a random positioning machine for 3 days during their differentiation to cardiomyocytes. This process resulted in the production of highly enriched cardiomyocytes (99% purity) with high viability (90%) and expected functional properties, with a 1.5 to 4-fold higher yield of cardiomyocytes from each undifferentiated stem cell as compared with 3D-standard gravity culture. Increased induction, proliferation and viability of cardiac progenitors as well as up-regulation of genes associated with proliferation and survival at the early stage of differentiation were observed in the 3D culture under simulated microgravity. Therefore, a combination of 3D culture and simulated microgravity can be used to efficiently generate highly enriched cardiomyocytes.
Heart disease is a major health concern, claiming more lives each year than any other diseases1. Cardiomyocytes (CMs) derived from human pluripotent stem cells (hPSCs) could provide an unlimited supply of cells to replenish the lost cardiac muscle. In preclinical studies, hPSC-CMs and hPSC-cardiac progenitors have been found to prevent progression of heart failure in animal models2,3,4,5,6,7,8,9. It is estimated that ~109 CMs are needed to repair a failing human heart, and graft survival is challenging—for example, in over 90% of transplanted hPSC-CMs die even with pro-survival pretreatment in a nonhuman primate model10. Therefore, to fully realize the potentials of hPSCs, efficient and robust generation of large quantities of CMs is critical. CM differentiation requires specific induction of the transition from stem cells to cardiac progenitors with growth factors2,11, small molecules12,13, signals from endodermal environment14,15 and matrix proteins16. It is also conceivable that promoting proliferation of cardiac progenitors and increasing cell viability during in vitro differentiation could increase the CM yield and improve graft survival.
3D culture and microgravity, a condition in which objects appear to be weightless, can profoundly modulate cell proliferation and survival. 3D culture allows cells to self-organize by aggregation and facilitate spatially unrestricted interactions between cells and their surroundings, circumventing the disadvantages of 2D culture that limit cell-cell signaling and restrict cell growth in an artificial environment17. Consequently, incorporating 3D culture during the transition from cardiac progenitors to CMs may facilitate the proliferation and survival of cardiac progenitors. In addition, 3D culture has advantages for scale up production of hPSCs and their derivatives18,19,20. Microgravity is also known to modulate cell proliferation and survival21. For example, simulated microgravity potentiates the proliferation of bone marrow-derived human mesenchymal stem cells22 and adipose-derived stem cells23. Bioreactors have been designed to simulate aspects of microgravity and weightless environment during spaceflight and have been utilized to culture many cell types including stem cells, osteoblasts and cancer cells24,25,26. In these systems, cells can form complex multicellular aggregates or organoids and can be maintained for days and months in a gentle, low-shear and low-turbulence environment with sufficient oxygenation and effective mass transfer of nutrient and waste.
In this study, we have examined whether 3D tissue engineering of cardiac progenitors in combination with simulated microgravity could improve the efficiency of CM generation from hPSCs. We generated cardiac progenitors from hPSCs, engineered them into multicellular 3D progenitor cardiac spheres through controlled aggregation, and then examined the impact of 3D culture and simulated microgravity on CM purity, viability and yield. In addition, we analyzed CM induction, proliferation, cell survival and molecular changes in early-stage cardiac cells in an effort to gain possible mechanistic insights of the effect of 3D culture and simulated microgravity on differentiation.
Suspension culture of progenitor cardiac spheres and simulated microgravity increase cell viability and CM yield
We initially characterized starting materials of hPSCs and evaluated the efficiency of cardiac induction. At day 0, the culture displayed sheet-like morphology and contained >95% TRA1-60pos stem cells (Fig. S1A). At day 4, cells lost typical stem cell morphology (Fig. S1B) and >90% of them expressed a cardiac mesoderm marker, MESP1, which is typically up-regulated at days 4 to 527.
To generate 3D cell aggregates of cardiac progenitors using a microscale technique, day 4 cells were dissociated and force-aggregated in a microwell plate at three different densities: 500, 1500 and 2500 cells/microwell. After 24 h, sphere-shaped cell aggregates, named progenitor cardiac spheres, were generated from all cultures (Fig. S1C). After culture in suspension, cardiac spheres from cultures seeded at densities of 1500 and 2500 cells/microwell were more compact than those from cultures seeded at densities of 500 cells/microwell (Fig. S1C). Similar results were observed when progenitor cardiac spheres were generated from day 6 cells. At day 20, almost all cardiac spheres showed spontaneous beating, and α-actinin, a CM-associated protein, was detected in ~62%, ~87% and ~82% of the cells in cultures with seeding densities of 500 cells/microwell, 1500 cells/microwell and 2500 cells/microwell, respectively (Fig. S1D). Thus, seeding density of 1500 cells/microwell was selected for subsequent experiments.
To examine the effect of simulated microgravity and 3D culture on CM differentiation (Fig. 1A), progenitor cardiac spheres were generated from day 4 IMR-90 iPSCs induced by activin A and BMP4 (Fig. S1 and S3A), transferred to OptiCell disks and maintained under simulated microgravity using a random positioning machine (RPM) (Fig. S2B and S2C). After the exposure to simulated microgravity for 3 days (the duration was optimized – Fig. S2), the culture, designated as 3D-MG, was transferred to standard gravity at day 8. Parallel cultures of 3D spheres in suspension under standard gravity (3D-SG) and 2D cultures under standard gravity (2D-SG) were also maintained for comparison. Overall cell morphology of 3D-MG was similar to that of 3D-SG; the spheres were similar in size 24 h after aggregation and became irregular in shape at later time points, possibly due to random budding of cell growth (Fig. S3B, S3C and S3D). Typically, contracting cells were observed by differentiation days 8–10 in both 2D and 3D cultures. At day 20, almost all spheres in 3D-SG and 3D-MG showed spontaneous beating, while only some beating areas were observed in 2D-SG (Movies S1,2 to S3). The 3D-SG and 3D-MG cultures at day 20 contained up to 99% α-actininpos cells, which was higher than observed in 2D-SG (Fig. 1B–D, P < 0.001 to 0.05).
Cell viability assayed by ethidium monoazide (EMA) staining in a representative experiment showed that ~90% and 78% of the cells from 3D-MG and 3D-SG, respectively, were viable (EMA negative) whereas only ~56% of the cells from 2D-SG were viable (Fig. 1B). Analysis of 5 to 6 cultures per condition indicated that 3D-SG and 3D-MG contained a higher percentage of viable cells than 2D-SG (Fig. 1D, P < 0.01 and <0.001, respectively). To exclude the possibility that these differences might be caused by cell dissociation of tightly packed 2D or 3D culture, we also performed Live/Dead staining of intact cultures. As shown in Fig. S3D, 3D-MG and 3D-SG had fewer dead cells than did 2D-SG, which was consistent with the observation by flow cytometry assay of post-dissociated cells (Fig. 1).
The CM yield was 1.5-fold and 5-fold higher in 3D-MG than the 3D-SG and 2D-SG, respectively (Fig. 1D and Fig. S4, P < 0.01 and <0.0001, respectively). Cell density was also higher in 3D-MG (6.3 ± 1.0 × 105 cells/ml) than 3D-SG (4.5 ± 1.2 × 105 cells/ml and P < 0.05).
We also examined the effect of simulated microgravity and 3D culture on CM differentiation from H7 and H9 human embryonic stem cells (hESCs) (Fig. 1E,F). Cells were induced for CM differentiation by small molecules targeting the Wnt signaling13 and exposed to simulated microgravity from days 6 to 9. At day 20, the proportions of viable cells were higher in 3D-MG than 3D-SG and 2D-SG (P < 0.05 and<0.01, respectively). CM purity of H7-derived cells as detected by α-actininpos cells was ~97% in 3D-MG while only ~62% and ~41% CMs were detected in 3D-SG and 2D-MG, respectively. CM purity of H9-derived cells was ~85% in 3D-MG while only ~71% and ~48% CMs in 3D-SG and 2D-MG, respectively. The CM yield was 3 to 4-fold and 7 to 8-fold higher in 3D-MG than 3D-SG and 2D-SG, respectively (Fig. 1E,F and Fig. S4). Cell density was also higher in 3D-MG than 3D-SG (P < 0.05). These results indicated that simulated microgravity and 3D culture significantly improved cell viability, CM purity and yield in H7 and H9 cells.
We then examined the effect of simulated microgravity and 3D culture on endothelial cell differentiation since mesoderm stage MESP1pos cells could give rise to endothelial cells. However, at differentiation day 20, very few cells (<2%) were positive for endothelial cell makers, CD31, vascular endothelial cadherin (VE-cadherin) in 3 culture conditions (2D-SG, 3D-SG and 3D-MG) examined (Fig. S6).
To examine if improved CM differentiation in 3D culture was due to dissociation of cardiac progenitor cells and if low cell yield in 2D culture was due to the limitation in space for cell expansion, day 4 cells were dissociated and re-seeded at 3 densities (undiluted, diluted 2 times and 4 times) in 2D culture and CM differentiation efficiency was compared at day 20 with parallel intact cultures. As shown in Fig. S5, the levels in cell viability, CM purity and yield from the dissociated 2D cultures were similar to the intact 2D cultures, suggesting that cell dissociation and providing additional space to cells in 2D culture were not sufficient to improve CM yield.
These observations showed that 3D cultures produced CMs with greater purity and higher yield than 2D culture and that exposure of 3D progenitor cardiac spheres to simulated microgravity improved CM yield even further.
Characterization of CMs derived from progenitor cardiac spheres expanded under standard gravity and simulated microgravity
We next examined cellular and molecular features of the CMs from 3D-SG and 3D-MG. As shown in Fig. 2A, all cultures contained cells that were positive for CM-associated markers, including structural proteins, α-actinin and cardiac troponin I (cTnI), and cell-cell adhesion molecule, cadherin. Overall, 3D-SG and 3D-MG showed more cells positive for these CM-associated markers than did 2D-SG, which is consistent with increased CM purity in 3D-SG and 3D-MG than 2D-SG.
We also examined the expression of genes encoding CM structural proteins (Fig. 2B) and calcium handling proteins (Fig. 2C). Of the 12 genes examined, 11 (MYH6, MYH7, MYL2, MYL7, TNNI1, TNNI3, TNN, ATP2A2, CASQ2, RYR2 and SLC8A1) were detected at higher levels in 3D-MG than 2D-SG (P < 0.0001 to 0.05). In addition, 8 (MYH6, MYL2, MYL7, TNNI1, ATP2A2, CASQ2, RYR2 and SLC8A1) were detected at higher levels in 3D-MG than 3D-SG (P < 0.001 to 0.05), and none was lower in 3D-MG than 3D-SD.
Under higher magnification, sarcomeric structures were observed in a subset of CMs in all cultures stained with α-actinin, confirming the characteristics of CMs. To examine the effect of simulated microgravity on sarcomeric organization, we carried out immunostaining of α-actinin, a marker for myofibrillar Z-discs. Typically hPSC-CM cultures contain CMs with different levels of sarcomeric maturation. We evaluated these cells for their overall appearance of myofibrillar structure and categorize them into 3 different levels as we and others described previously28,29: Score 1 cells are α-actininpos but without clear sarcomeric striations; Score 2 cells have diffuse punctate staining pattern and some patterned striations in partial cell area; and Score 3 cells have highly organized and well-defined myofibrillar structure with distinct paralleled bands of z-discs distributed throughout the cell area. Compared with 3D cardiac spheres expanded under standard gravity, 3D cardiac spheres exposed to simulated microgravity produced CMs with higher levels of structural maturation based on the levels of sarcomeric striations (Fig. 3A), although T tubules were not detectable in cells from any conditions.
We next investigated the effect of simulated microgravity on Ca2+ transients by confocal line-scan recordings of live 3D-SG and 3D-MG cells (Fig. 3B). There were no significant differences in fluorescent amplitude (F/F0) between the two groups. However, the maximal upstroke and decay velocities were ~38% (P < 0.01) and ~44% (P < 0.0001) faster in 3D-MG CMs compared to 3D-SG CMs, respectively. Furthermore, the time from the peak to 50% decay was ~38% shorter (P < 0.0001) in 3D-MG CMs compared to 3D-SG CMs, demonstrating an enhanced rate of Ca2+ reuptake, a feature associated with more mature CMs30. The calcium imaging data is consistent with the increased expression of ATP2A2 (SERCA2a) and SLC8A1 (NCX) in 3D-MG compared with 3D-SG (Fig. 2C) which suggested that 3D-MG had improved calcium handling gene expression because CM purity of 3D-MG was similar to that of 3D-SG.
Action potential parameters including depolarization velocity (dV/dtmax), resting membrane potential (MDP), action potential amplitude (APA) and action potential duration (APD) of CMs from 3D-MG detected by patch-clamp were not significantly different from those from 3D-SG (Fig. 3C; P > 0.05 for all parameters except that the dV/dtmax of 3D-SG CMs was faster than that of 3D-MG CMs.)
Using microelectrode array (MEA) recordings, we investigated pharmacological responses of CMs from the three cultures (Fig. 4A). When the cells were treated with β-adrenergic agonist isoproterenol, all cultures showed an increase in spontaneous beating rate (Fig. 4B,C, P < 0.001); the increased beating was attenuated when cells were further treated with carbamylcholine, a cholinergic agonist, (Fig. 4B,C, P < 0.001 to 0.01). When the cells were treated with phenylephrine, an α1-adrenergic receptor agonist, beating rates in all cultures increased (Fig. 4D, P < 0.01). In addition, when cells were treated with nifedipine, a calcium channel blocker, normalized mean corrected field potential durations (cFPD) of the cells in all 3 cultures decreased (Fig. 4E,F; P < 0.01 to 0.05).
These data suggest that CMs generated from 3D-SG and 3D-MG have similar electrophysiological properties and pharmacological responses.
Simulated microgravity and 3D culture promote the induction of cardiac progenitors and CM differentiation
To examine the effect of simulated microgravity and 3D culture on the induction of cardiac progenitors and CM differentiation, we analyzed the expression of markers associated with cardiac progenitors and CMs at various time points from differentiation days 4 to 12. At day 4, ~61% of the population were positive for KDR and PDGFRα, markers associated with cardiac mesoderm induction11. At day 6, KDRpos/PDGFRαpos cells increased to ~76% in 3D-MG, but decreased to ~16% and ~41% in 2D-SG and 3D-SG, respectively (Fig. 5A). At day 8, 3D-MG cells retained the expression of CD13, a cardiac mesoderm marker31,32 at higher levels compared with cells under standard gravity (Fig. 5B). The expression of ISL1, a marker for cardiac progenitors33, increased overtime with a peak at day 8 to ~75% in 3D-MG as compared with ~61% and ~68% in 2D-SG and 3D-SG, respectively (Fig. 5C). These results suggest that simulated microgravity and 3D culture increase the induction of cardiac progenitors.
We next examined if these cardiac progenitors led to robust CM differentiation (Fig. 5D,E). At day 12, the proportions of cells that were positive for SIRPA, a surface CM marker, increased to ~74% in 3D-MG compared with ~52% and ~65% in 2D-SG and 3D-SG, respectively. Similarly, the proportions of cTnTpos/α-actininpos cells were the highest in 3D-MG at day 12. These result suggest that simulated microgravity and 3D culture promote CM differentiation.
Simulated microgravity and 3D culture promote the proliferation of cardiac progenitors
To determine if there was increased proliferation of cardiac progenitors in 3D-SG and 3D-MG at the early stage (which may contribute to the higher cell yield and viability in the 3D cultures at late stages), we examined the ability of the cells to incorporate EdU as an indicator of proliferation. Among the NKX2-5pos progenitors at day 10, a subset of them was EdUpos (Fig. S7A). By flow cytometry, 24.4%, 32.3% and 44.0% were identified as EdUpos/NKX2-5pos cells in 2D-SG, 3D-SG and 3D-MG, respectively (Fig. 6A). The number of EdUpos/NKX2-5pos cells was higher in 3D-MG than 3D-SG and 2D-SG (P < 0.05 and <0.01 respectively).
We also found that a subset of the NKX2-5pos cells at day 10 expressed Ki-67, a marker for cells at active phases of the cell cycle (Fig. S7B). By flow cytometry analysis, ~31%, ~40% and ~55% of the cells were NKX2-5pos/Ki-67pos in 2D-SG, 3D-SG and 3D-MG, respectively (Fig. 6B). The proportions of NKX2-5pos/Ki-67pos cells were higher in 3D-SG and 3D-MG than 2D-SG (P < 0.05 and <0.001, respectively), and also higher in 3D-MG than 3D-SG (P < 0.01). Similarly, a subset of the NKX2-5pos cells at day 8 expressed IAK1 (aurora-A kinase), a key regulator in the control of cell proliferation (Fig. 6C). The proportions of NKX2-5pos/IAK1pos cells were higher in 3D-MG than 2D-SG and 3D-SG (P < 0.001 and <0.05, respectively).
To further investigate the effect of 3D culture and simulated microgravity on cell proliferation, we also examined the expression of genes associated with proliferation and cell cycle at day 8 by qRT-PCR. Higher expression levels of genes related to cell proliferation (MKI67 and PCNA) and cell cycle (ANLN, AURKA, AURKB, CCNB1 and PLK1) were detected in 3D-SG and 3D-MG than 2D-SG (P < 0.0001, Fig. 6C). Furthermore, expression levels of genes associated with cell cycle and proliferation (ANLN, AURKA, AURKB, CCNB1, MKI67, and PLK1; 6 out of 7 examined) were higher in 3D-MG than 3D-SG (P < 0.0001 to 0.001).
Simulated microgravity and 3D culture increase cell survival of cardiac progenitors
To examine if suspension culture and exposure to simulated microgravity could improve cell survival, we assessed cell survival at day 8 before and after dissociation of cultures. Live/Dead staining of intact cultures showed that 3D-MG contained less dead cells than 3D-SG and 2D-SG (Fig. S3C). To quantify the difference, we stained the dissociated cells using propidium iodide (PI), which stains dead cells, and FITC-labeled Annexin V, which stains apoptotic cells. In 3D-MG, ~90% of the cells were viable, whereas in 2D-SG and 3D-SG, ~70% and ~74% of the cells were viable, respectively (Fig. 7A,B); the proportions of live cells in 3D-MG were higher than 3D-SG and 2D-SG (P < 0.0001) while the proportions of apoptotic or dead cells were significantly lower in 3D-MG than 3D-SG and 2D-SG (P < 0.0001 to 0.05).
In addition, the cell yield at day 8 generated from each input hPSC was higher in 3D-MG than 3D-SG and 2D-SG (P < 0.05 and <0.01, respectively, Fig. 7C). Cell density was also higher in 3D-MG than 3D-SG (Fig. 7C).
We next examined the expression of prosurvival genes in day 8 cells (Fig. 7D). Expression of BIRC5, which encodes an anti-apoptotic protein34, was detected at higher level in 3D cultures than 2D culture (P < 0.0001) and in 3D-MG than 3D-SG (P < 0.001). Similarly, expression of genes encoding heat shock proteins HSP60, HSP70 and HSP90 was detected at higher level in 3D cultures than 2D culture (P < 0.0001), and the level of HSP60 expression was higher in 3D-MG than 3D-SG (P < 0.001).
We then examined day 8 cardiac progenitor cells for their expression of p-AKT (phosphorylated AKT-pS473), which plays a critical role in regulating cell survival35,36 (Fig. 7E and 7F). By flow cytometry, ~10%, ~27% and ~39% of NKX2-5pos/p-AKT pos cells were detected in 2D-SG, 3D-SD and 3D-MG, respectively; the proportions of NKX2-5pos/p-AKT pos cells in 3D-MG were higher than 3D-SG and 2D-SG (P < 0.05 and <0.001, respectively), and also higher in 3D-MG than 3D-SG (P < 0.05) (Fig. 7E).
To further understand how simulated microgravity affects cardiac progenitors during early stage of cardiac differentiation, RNA-sequencing analysis was performed to compare global gene expression profiles of day 8 cells in 3D-MG vs. 3D-SG. Among differentially expressed genes, 53 of them were up-regulated and 75 were down-regulated. The top 30 up-regulated genes (Table S1) include LEPR, liptin receptor, which is involved in fatty acid metabolism required for mature CMs; HCN4, which is a marker for the first heart field cardiac progenitors and conduction systems37; HAND2 which is essential for cardiac ventricle formation38; and LIFR, leukemia inhibitory factor receptor, which is involved in AKT signaling that is important for CM growth, survival and function39.
Together, these data demonstrate increased cell viability and increased expression of genes associated with growth, development, and pro-survival in 3D-MG than 3D-SG at the progenitor cell stage.
The effect of simulated microgravity on cells is known to vary depending on factors including cell type, specific bioreactor used and duration of exposure to simulated microgravity40,41,42. Our study suggests that a short-term exposure of cardiac progenitors to simulated microgravity in an RPM may be leveraged to improve the expansion and viability of cardiac progenitors and subsequent generation of CMs. In combination with the engineering of microscale 3D cardiac progenitors, the exposure of the cells to simulated microgravity significantly increased cell viability (up to 90%), purity (up to 99%) and yield (up to 8-fold higher) of hPSC-CMs compared with the conventional 2D culture under standard gravity. In addition, CM yield was 1.5 to 4-fold higher in 3D-MG than 3D-SG.
Although 2D cardiac differentiation protocols using monolayer methods are available to produce CMs at high purity2,13, differentiation efficiency among different cell lines or batches varies. Methods such as depletion of glucose from medium43 have been developed to enrich CMs at late stages of differentiation when the differentiation efficiency is low. The culture system we have established using simulated microgravity and 3D culture provides a novel way to increase the induction, proliferation and survival of cardiac progenitors, thus further improving CM cell numbers (yield) and purity, an outcome that is desirable for the application of hPSC-CMs in regenerative medicine. Furthermore, this culture system could help identify molecular mechanisms associated with improved the induction of cardiac progenitors and develop alternative strategies under standard gravity to improve CM differentiation.
The high purity, viability and yield of hPSC-CMs at the late stage of differentiation are also likely contributed by the increased proliferation and viability of cardiac progenitors at the early stage of differentiation. Compared with the 2D culture, the early stage 3D cultures contained more cells with features of proliferation (measured by the incorporation of EdU and expression of Ki-67) and higher expression levels of genes related to cell proliferation and cell cycle. Furthermore, the 3D culture and simulated microgravity improved the viability of cardiac progenitors and up-regulated pro-survival genes that encode heat shock proteins and anti-apoptotic protein BIRC5 (also known as survivin). The HSP70/90 heat shock proteins are known to be involved in the regulation of cell cycle progression and cell proliferation44, and increased expression of BIRC5 should result in less apoptosis that might be induced by microgravity stress. In other studies, up-regulation of heat shock proteins was also observed in rat hypothalamus tissues45, the Jurkat cells46 and myelomonocytic U937 cells47 as a result of exposure to microgravity, and BIRC5 was up-regulated in thymus after mice returned from a spaceflight48. In addition, a study on neonatal and adult cardiovascular progenitors reported that simulated microgravity could affect cell differently depending on age42. Among many differential responses, final number of cells and expression of DNA repair genes were increased in neonatal but not adult cardiac progenitors upon exposure to simulated microgravity42. These studies suggest that simulated microgravity can improve cell proliferation and survival in a cell type dependent manner.
Given the high viability of CMs and higher expression levels of genes associated with proliferation and pro-survival including HSPs and BIRC5, the cardiac sphere preparation generated under simulated microgravity may be desirable for regenerative medicine over CMs generated from the 2D culture. Up-regulation of heat shock proteins through a brief treatment of heat shock has been shown to increase cell survival in both in vitro and in vivo studies with hPSC-CMs49. The transcriptional mechanisms and the biological meaning of the higher expression of HSPs and BIRC5 in 3D-MG hPSC-CMs remain to be elucidated. These 3D-MG cells with high levels of HSPs and BIRC5 might be more resistant to cell death and improve graft survival in vivo. Further understanding the mechanisms and pathways involved in the regulation of cell survival by simulated microgravity could facilitate the identification of alternative methods under standard gravity for efficient production of cardiac progenitors and CMs with enhanced potential for graft survival. Further understanding the mechanisms and pathways involved in the regulation of cell survival by simulated microgravity could facilitate the identification of alternative methods under standard gravity for efficient production of cardiac progenitors and CMs with enhanced potential for graft survival.
We have not examined the effect of longer exposure to simulated microgravity as we intended to target cardiac progenitors at the early stage of the differentiation rather than CMs at the late stage. Our study was designed to expand cardiac progenitors at differentiation days 5 or 6 under a brief exposure to simulated microgravity (3 days) and then transfer them to standard gravity for further differentiation into CMs, because a long-term exposure of microgravity could have a negative effect on stem cell differentiation. In fact, a long-term exposure of undifferentiated mouse ESCs to space microgravity for 15 days inhibited their differentiation50. Thus, the duration of microgravity treatment is an important factor to be considered, although the discrepancy in experimental outcomes between this mouse ESC study50 and our study may also be due to differences in cell types used (mouse ESCs vs. hPSCs), stages of the cells exposed to microgravity (undifferentiated cells vs. cardiac progenitors), types of microgravity (space microgravity vs. simulated microgravity) and/or environmental factors (with and without radiation and other factors in space and during transportation). In addition, longer exposure to simulated microgravity could also adversely affect the properties of CMs. Prolonged space flight can induce health problems including muscle atrophy and cardiovascular disorders51. CMs produced in our study, however, had expected molecular and functional features. 3D-MG increased the number of cells with the well-organized sarcomeric structure and increased the expression of genes encoding cardiac contractile proteins and calcium handing proteins. 3D-MG CMs also had appropriate pharmacological responses and improved Ca2+ handling properties. The action potential profiles of 3D-MG CMs were similar to those of 3D-SG CMs for all parameters except faster dV/dtmax in 3D-SG CMs. The underlying mechanisms of these observations still require to be further investigated.
In conclusion, we demonstrate that suspension culture and expansion of 3D engineered progenitor cardiac spheres under simulated microgravity result in efficient generation of highly enriched hPSC-CMs. This culture system increases proliferation and viability of cardiac progenitors, which could improve the application of these cells in regenerative medicine.
Detailed methods are available in the Online Supplementary Information. In brief, IMR90 iPSCs52 and hESCs (H7 and H9)53 were used to generate cardiac progenitors by growth factors2,54 or small molecules13. Progenitor cardiac spheres were generated by forced aggregation in AggreWells28 and subjected to simulated microgravity using an RPM55,56. Characterization was performed to compare cells under standard gravity and simulated microgravity using various methods28,57,58 including microscopy, immuonocytochemical analysis, flow cytometry, qRT-PCR, RNA-seq, MEA recordings, calcium imaging, and patch-clamp.
Accession code: The RNA-seq data reported in this paper are available on the GEO database with accession number GSE84582.
How to cite this article: Jha, R. et al. Simulated Microgravity and 3D Culture Enhance Induction, Viability, Proliferation and Differentiation of Cardiac Progenitors from Human Pluripotent Stem Cells. Sci. Rep. 6, 30956; doi: 10.1038/srep30956 (2016).
Kung, H. C., Hoyert, D. L., Xu, J. & Murphy, S. L. Deaths: final data for 2005. Natl Vital Stat Rep 56, 1–120 (2008).
Laflamme, M. A. et al. Cardiomyocytes derived from human embryonic stem cells in pro-survival factors enhance function of infarcted rat hearts. Nat Biotechnol 25, 1015–1024 (2007).
Caspi, O. et al. Transplantation of human embryonic stem cell-derived cardiomyocytes improves myocardial performance in infarcted rat hearts. J Am Coll Cardiol 50, 1884–1893 (2007).
Leor, J. et al. Human embryonic stem cell transplantation to repair the infarcted myocardium. Heart 93, 1278–1284 (2007).
Nelson, T. J. et al. Repair of acute myocardial infarction by human stemness factors induced pluripotent stem cells. Circulation 120, 408–416 (2009).
van Laake, L. W., Passier, R., Doevendans, P. A. & Mummery, C. L. Human embryonic stem cell-derived cardiomyocytes and cardiac repair in rodents. Circ Res 102, 1008–1010 (2008).
Shiba, Y. et al. Human ES-cell-derived cardiomyocytes electrically couple and suppress arrhythmias in injured hearts. Nature (2012).
Blin, G. et al. A purified population of multipotent cardiovascular progenitors derived from primate pluripotent stem cells engrafts in postmyocardial infarcted nonhuman primates. J Clin Invest 120, 1125–1139 (2010).
Masumoto, H. et al. Human iPS cell-engineered cardiac tissue sheets with cardiomyocytes and vascular cells for cardiac regeneration. Sci Rep 4, 6716 (2014).
Chong, J. J. & Murry, C. E. Cardiac regeneration using pluripotent stem cells-Progression to large animal models. Stem Cell Res 13, 654–665 (2014).
Kattman, S. J. et al. Stage-specific optimization of activin/nodal and BMP signaling promotes cardiac differentiation of mouse and human pluripotent stem cell lines. Cell Stem Cell 8, 228–240 (2011).
Lian, X. et al. Robust cardiomyocyte differentiation from human pluripotent stem cells via temporal modulation of canonical Wnt signaling. Proc Natl Acad Sci USA 109, E1848–1857 (2012).
Burridge, P. W. et al. Chemically defined generation of human cardiomyocytes. Nat Methods 11, 855–860 (2014).
Mummery, C. et al. Differentiation of human embryonic stem cells to cardiomyocytes: role of coculture with visceral endoderm-like cells. Circulation 107, 2733–2740 (2003).
Stefanovic, S. et al. Interplay of Oct4 with Sox2 and Sox17: a molecular switch from stem cell pluripotency to specifying a cardiac fate. J Cell Biol 186, 665–673 (2009).
Zhang, J. et al. Extracellular matrix promotes highly efficient cardiac differentiation of human pluripotent stem cells: the matrix sandwich method. Circ Res 111, 1125–1136 (2012).
Lancaster, M. A. & Knoblich, J. A. Organogenesis in a dish: modeling development and disease using organoid technologies. Science 345, 1247125 (2014).
Kempf, H. et al. Controlling expansion and cardiomyogenic differentiation of human pluripotent stem cells in scalable suspension culture. Stem Cell Reports 3, 1132–1146 (2014).
Otsuji, T. G. et al. A 3D sphere culture system containing functional polymers for large-scale human pluripotent stem cell production. Stem Cell Reports 2, 734–745 (2014).
Chen, A. K., Reuveny, S. & Oh, S. K. Application of human mesenchymal and pluripotent stem cell microcarrier cultures in cellular therapy: achievements and future direction. Biotechnol Adv 31, 1032–1046 (2013).
Unsworth, B. R. & Lelkes, P. I. Growing tissues in microgravity. Nat Med 4, 901–907 (1998).
Yuge, L. et al. Microgravity potentiates stem cell proliferation while sustaining the capability of differentiation. Stem Cells Dev 15, 921–929 (2006).
Zhang, S. et al. The effects of spheroid formation of adipose-derived stem cells in a microgravity bioreactor on stemness properties and therapeutic potential. Biomaterials 41, 15–25 (2015).
Becker, J. L. & Souza, G. R. Using space-based investigations to inform cancer research on Earth. Nat Rev Cancer 13, 315–327 (2013).
Gerecht-Nir, S., Cohen, S. & Itskovitz-Eldor, J. Bioreactor cultivation enhances the efficiency of human embryoid body (hEB) formation and differentiation. Biotechnol Bioeng 86, 493–502 (2004).
Pardo, S. J. et al. Simulated microgravity using the Random Positioning Machine inhibits differentiation and alters gene expression profiles of 2T3 preosteoblasts. Am J Physiol Cell Physiol 288, C1211–1221 (2005).
Jha, R. et al. Molecular beacon-based detection and isolation of working-type cardiomyocytes derived from human pluripotent stem cells. Biomaterials 50, 176–185 (2015).
Nguyen, D. C. et al. Microscale generation of cardiospheres promotes robust enrichment of cardiomyocytes derived from human pluripotent stem cells. Stem Cell Reports 3, 260–268 (2014).
Ribeiro, M. C. et al. Functional maturation of human pluripotent stem cell derived cardiomyocytes in vitro–correlation between contraction force and electrophysiology. Biomaterials 51, 138–150 (2015).
Lundy, S. D., Zhu, W. Z., Regnier, M. & Laflamme, M. A. Structural and functional maturation of cardiomyocytes derived from human pluripotent stem cells. Stem Cells Dev 22, 1991–2002 (2013).
Skelton, R. J. et al. CD13 and ROR2 Permit Isolation of Highly Enriched Cardiac Mesoderm from Differentiating Human Embryonic Stem Cells. Stem Cell Reports 6, 95–108 (2016).
Ardehali, R. et al. Prospective isolation of human embryonic stem cell-derived cardiovascular progenitors that integrate into human fetal heart tissue. Proc Natl Acad Sci USA 110, 3405–3410 (2013).
Lian, X. et al. Directed cardiomyocyte differentiation from human pluripotent stem cells by modulating Wnt/beta-catenin signaling under fully defined conditions. Nat Protoc 8, 162–175 (2013).
Tamm, I. et al. IAP-family protein survivin inhibits caspase activity and apoptosis induced by Fas (CD95), Bax, caspases, and anticancer drugs. Cancer Res 58, 5315–5320 (1998).
Zoncu, R., Efeyan, A. & Sabatini, D. M. mTOR: from growth signal integration to cancer, diabetes and ageing. Nat Rev Mol Cell Biol 12, 21–35 (2011).
Liu, P. et al. Cell-cycle-regulated activation of Akt kinase by phosphorylation at its carboxyl terminus. Nature 508, 541–545 (2014).
Liang, X. et al. HCN4 dynamically marks the first heart field and conduction system precursors. Circ Res 113, 399–407 (2013).
Yamagishi, H. et al. The combinatorial activities of Nkx2.5 and dHAND are essential for cardiac ventricle formation. Dev Biol 239, 190–203 (2001).
Matsui, T. & Rosenzweig, A. Convergent signal transduction pathways controlling cardiomyocyte survival and function: the role of PI 3-kinase and Akt. J Mol Cell Cardiol 38, 63–71 (2005).
Blaber, E., Sato, K. & Almeida, E. A. Stem cell health and tissue regeneration in microgravity. Stem Cells Dev 23 Suppl 1, 73–78 (2014).
Grimm, D. et al. Growing tissues in real and simulated microgravity: new methods for tissue engineering. Tissue Eng Part B Rev 20, 555–566 (2014).
Fuentes, T. I. et al. Simulated Microgravity Exerts an Age-Dependent Effect on the Differentiation of Cardiovascular Progenitors Isolated from the Human Heart. PLoS One 10, e0132378 (2015).
Tohyama, S. et al. Distinct metabolic flow enables large-scale purification of mouse and human pluripotent stem cell-derived cardiomyocytes. Cell Stem Cell 12, 127–137 (2013).
Hirono, S. et al. Chlamydia pneumoniae stimulates proliferation of vascular smooth muscle cells through induction of endogenous heat shock protein 60. Circ Res 93, 710–716 (2003).
Iqbal, J. et al. Differential expression of specific cellular defense proteins in rat hypothalamus under simulated microgravity induced conditions: comparative proteomics. Proteomics 14, 1424–1433 (2014).
Cubano, L. A. & Lewis, M. L. Effect of vibrational stress and spaceflight on regulation of heat shock proteins hsp70 and hsp27 in human lymphocytes (Jurkat). J Leukoc Biol 69, 755–761 (2001).
Maier, J. A. Impact of simulated microgravity on cell cycle control and cytokine release by U937 cells. Int J Immunopathol Pharmacol 19, 279–286 (2006).
Gridley, D. S. et al. Spaceflight effects on T lymphocyte distribution, function and gene expression. J Appl Physiol (1985) 106, 194–202 (2009).
Laflamme, M. A. et al. Formation of human myocardium in the rat heart from human embryonic stem cells. Am J Pathol 167, 663–671 (2005).
Blaber, E. A. et al. Microgravity Reduces the Differentiation and Regenerative Potential of Embryonic Stem Cells. Stem Cells Dev 24, 2605–2621 (2015).
White, R. J. & Averner, M. Humans in space. Nature 409, 1115–1118 (2001).
Yu, J. et al. Induced pluripotent stem cell lines derived from human somatic cells. Science 318, 1917–1920 (2007).
Thomson, J. A. et al. Embryonic stem cell lines derived from human blastocysts. Science 282, 1145–1147 (1998).
Jha, R., Xu, R. H. & Xu, C. Efficient differentiation of cardiomyocytes from human pluripotent stem cells with growth factors. Methods Mol Biol 1299, 115–131 (2015).
Patel, M. J. et al. Identification of mechanosensitive genes in osteoblasts by comparative microarray studies using the rotating wall vessel and the random positioning machine. J Cell Biochem 101, 587–599 (2007).
van Loon, J. J. Some history and use of the random positioning machine, RPM, in gravity related research. Adv Space Res 39, 1161–1165 (2007).
Han, J., Wu, Q., Xia, Y., Wagner, M. B. & Xu, C. Cell alignment induced by anisotropic electrospun fibrous scaffolds alone has limited effect on cardiomyocyte maturation. Stem Cell Res 16, 740–750 (2016).
Xu, C. et al. Efficient generation and cryopreservation of cardiomyocytes derived from human embryonic stem cells. Regen Med 6, 53–66 (2011).
This study was supported in part by grants GA-2014-126 from the Center for the Advancement of Science in Space (CASIS) and R21HL118454 from the NIH. Q.W. and M.P.K. were supported by the Center for Pediatric Nanomedicine at Emory/Georgia Tech. We thank Dr. Courtney McCracken at the Emory Children’s Biostatistics Core for advice on statistical analysis, Gregory Tharp and Nirav Patel at the Yerkes Genomics Core for RNA-seq analysis, Aaron Rae and Bridget Neary at the Emory Children’s Flow Cytometry Core for assistance with flow cytometry analysis and Ming Shen and Rong Jiang at the Emory Children’s Animal Physiology Core for assistance with the preparation of mouse embryonic fibroblasts.
The authors declare no competing financial interests.
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Jha, R., Wu, Q., Singh, M. et al. Simulated Microgravity and 3D Culture Enhance Induction, Viability, Proliferation and Differentiation of Cardiac Progenitors from Human Pluripotent Stem Cells. Sci Rep 6, 30956 (2016). https://doi.org/10.1038/srep30956
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