Lung injury and fibrosis represent the most significant outcomes of severe and acute lung disorders, including COVID-19. However, there are still no effective drugs to treat lung injury and fibrosis. In this study, we report the generation of clinical-grade human embryonic stem cells (hESCs)-derived immunity- and matrix-regulatory cells (IMRCs) produced under good manufacturing practice requirements, that can treat lung injury and fibrosis in vivo. We generate IMRCs by sequentially differentiating hESCs with serum-free reagents. IMRCs possess a unique gene expression profile distinct from that of umbilical cord mesenchymal stem cells (UCMSCs), such as higher expression levels of proliferative, immunomodulatory and anti-fibrotic genes. Moreover, intravenous delivery of IMRCs inhibits both pulmonary inflammation and fibrosis in mouse models of lung injury, and significantly improves the survival rate of the recipient mice in a dose-dependent manner, likely through paracrine regulatory mechanisms. IMRCs are superior to both primary UCMSCs and the FDA-approved drug pirfenidone, with an excellent efficacy and safety profile in mice and monkeys. In light of public health crises involving pneumonia, acute lung injury and acute respiratory distress syndrome, our findings suggest that IMRCs are ready for clinical trials on lung disorders.
Lung injury is a serious threat to human health, which is caused by many chemical, physical and biological agents, resulting in pneumonia, lung inflammation, and fibrosis. In a comprehensive analysis, the World Health Organization ranks lung diseases as the second largest category, and predicts that by 2020, about one fifth of human deaths will be attributed to lung diseases.1 Acute lung injury (ALI) is the injury of alveolar epithelial cells and capillary endothelial cells caused by various direct and indirect injury factors, resulting in diffuse pulmonary interstitial and alveolar edema, and acute hypoxic respiratory insufficiency. Pathophysiologically, its characteristics include decreased lung volume, decreased lung extensibility and imbalance of the ventilation/blood flow ratio. When ALI develops into the severe stage (oxygenation index < 200), it is called acute respiratory distress syndrome (ARDS). Globally, there are more than 3 million patients with ARDS annually, accounting for 10% of intensive care unit (ICU) admissions.2 ALI/ARDS patients have an average mortality rate of 35%–46%.3,4 In late ARDS, pulmonary fibrosis (PF) develops due to persistent alveolar injury, repeated destruction, repair, reconstruction and over-deposition of extracellular matrix (ECM),5 leading to progressive lung scars and common interstitial pneumonia. In general, idiopathic pulmonary fibrosis (IPF) patients show very poor prognosis, with a median survival time of 3–5 years after diagnosis.6 It has also been reported that the degree of pulmonary fibrosis is closely related to the mortality of ARDS.7,8 Importantly, there are still no effective FDA-approved drugs to treat ALI, ARDS or IPF hitherto, and most experimental drugs are still in the midst of Phase II or Phase III clinical studies.2,9,10
Stem cell therapy is an emerging treatment modality being used to cure various inflammatory and/or degenerative diseases, including ALI and PF. In particular, mesenchymal stem cells (MSCs) have been tested as an intravenous infusion therapy for ALI and PF.11,12 Preclinical and clinical studies of pulmonary fibrosis have shown that, after infusion, MSCs could migrate to the sites of lung injury, inhibit inflammation and improve recovery.13,14,15 However, clinical studies with primary MSCs derived from the umbilical cord, bone marrow or adipose tissue have been hampered by the lack of available donors, limited cell numbers from each donor, donor and tissue heterogeneity, inconsistent cell quality and the lack of standardized cell preparations. Moreover, primary MSCs show limited self-renewal capacities and finite lifespans. MSC-like cells derived from human embryonic stem cells (hESCs)16 could solve these problems,17,18,19 but the use of ill-defined and variable components of animal origin, such as fetal bovine serum (FBS) or OP9 feeder cells, may greatly compromise their consistency, safety and clinical applicability. Furthermore, these hESC-derived MSC-like cells have not been deeply characterized for their immunomodulatory functions in disease models.
In this study, we demonstrate that our hESC-derived MSC-like cell population has unique abilities in modulating the immunity and regulating extracellular matrix production, compared to regular MSC populations. Therefore, we named it as immunity- and matrix-regulatory cells (IMRCs). On the one hand, IMRCs resemble MSCs in their capacity for self-renewal and tri-lineage differentiation. On the other, compared to primary umbilical cord mesenchymal stem cells (UCMSCs), IMRCs also displayed a higher consistency in quality, stronger immunomodulatory and anti-fibrotic functions, and a robust ability to treat lung injury and fibrosis in vivo.
Generation of hESC-derived IMRCs
In this study, hESC-derived IMRCs were generated by passaging cells that are migrating from human embryoid bodies (hEBs), using serum-free reagents (Fig. 1a, b). The clinical hESC line (Q-CTS-hESC-2) was prepared as described previously.20 Clinical hESCs were maintained in Essential 8TM basal medium (E8) on vitronectin-coated plates, before dissociation into small clumps to form hEBs for 5 days. Subsequently, hEBs were transferred onto vitronectin-coated plates and cultured for 14 additional days. The hEBs outgrowth cells were dissociated and passaged continuously in IMRCs Medium. After 5 passages, IMRCs were harvested for characterization. IMRCs possessed fibroblast-like morphology (Fig. 1b) and maintained diploid karyotypes at passage 5 (Fig. 1c). Moreover, copy-number variation analysis by whole-genome sequencing data also showed that no chromosomal aneuploidies, large deletions nor duplication fragments were detected (Fig. 1d). Next, we analyzed the expression profile of MSC-specific genes (Fig. 1e). IMRCs showed a pattern that greatly differed from hESCs, and closely resembled primary umbilical cord-derived MSCs (UCMSCs). All pluripotency genes (POU5F1, SOX2, NANOG, ZFP42, SALL4), mesendoderm genes (MIXL1), and ectoderm genes (GAD1) were extinguished in both IMRCs and UCMSCs (Fig. 1e). IMRCs expressed MSC-specific genes, including PDGFRA and SPARC, and the MSC-specific surface markers NT5E (CD73), ENG (CD90), THY1 (CD105) and ITGB1 (CD29). Flow cytometry analysis further confirmed this surface marker profile (Fig. 1f; Supplementary information, Fig. S1a, b). By contrast, IMRCs were negative for the hematopoietic surface markers PTPRC (CD45) and CD34. IMRCs displayed the ability to undergo tri-lineage differentiation into mesenchymal tissues, such as adipocytes, chondroblasts and osteoblasts (Fig. 1g; Supplementary information, Fig. S1c). The proliferation rate of IMRCs was higher than that of UCMSCs at passage 15, suggesting that IMRCs have a stronger capacity for long-term self-renewal than primary MSCs (Fig. 1h). Interestingly, IMRCs were generally smaller than UCMSCs (Fig. 1i), suggesting that IMRCs can pass through small blood vessels and capillaries more easily, and are thus perhaps less likely to cause pulmonary embolism. To evaluate the clinical potential of the IMRCs, we measured the viability of IMRCs suspended in a published clinical injection buffer at 4 °C. We found that the viability of IMRCs remained higher (93%) than UCMSCs (73%) after 48 h (Fig. 1j).
IMRCs possess unique gene expression characteristics
To clarify the degree of similarity between hESCs, IMRCs and primary UCMSCs at the whole transcriptome level, we performed genome-wide profiling of IMRCs and UCMSCs and compared their gene expression with hESCs.21 Whole-transcriptome analysis confirmed that IMRCs clustered together with UCMSCs in an unsupervised hierarchical clustering (Fig. 2a). The global differentially expressed gene analysis showed that highly expressed genes in IMRCs and UCMSCs compared with hESCs, were enriched with angiogenesis, inflammatory response and extracellular matrix disassembly related processes (Supplementary information, Fig. S2). Accordingly, MSC-specific genes such as NT5E, ENG, PDGFRA, SPARC and ITGB1 were up-regulated, whereas pluripotency genes such as POU5F1, SOX2, SALL4 and ZFP42 were extinguished in IMRCs relative to hESCs, and the overall correlation with hESCs was weak (R2 = 0.66; Fig. 2b). Next, we analyzed the expression of genes specific to IMRCs, compared to UCMSCs (Fig. 2c). While the overall correlation with UCMSCs was stronger (R2 = 0.87), we also found that many genes were differentially expressed in IMRCs compared to primary UCMSCs. The up-regulated genes promote immunomodulation (LIF), tissue repair (VEGFA, GREM1), cell division (CDC20) and anti-fibrosis (MMP1). By contrast, the down-regulated genes predominantly promote inflammation (IL-1B, CXCL8, CCL2 and CXCL1; Fig. 2c). Gene set enrichment analysis (GSEA) of the differentially expressed genes confirmed that IMRCs manifest reduced inflammation and stronger proliferative capacity as their top gene signatures, compared to primary UCMSCs (Fig. 2d, e; Supplementary information, Fig. S3).
To elucidate the heterogeneity of gene expression amongst IMRCs, single-cell RNA sequencing (scRNA-seq) was performed for both IMRCs and primary UCMSCs. A total of 16,000 single-cell transcriptomes were obtained from two samples. Approximately 100,000 reads were obtained per cell, which generated a median of 31,000 unique molecular identifiers per cell, ~4800 expressed genes per cell and more than 22,000 total genes detected in the population. Our scRNA-seq data also showed that IMRCs were relatively homogenous in expression for the MSC-specific markers PDGFRA, SPARC, NT5E, ITGB1 and ENG (Fig. 2f; Supplementary information, Fig. S4). IMRCs were also relatively homogenous in their suppression of pluripotency and non-mesenchymal markers, relative to hESCs and UCMSCs, suggesting they are likely to be similar in biological activity to primary MSCs after transplantation (Fig. 2g; Supplementary information, Fig. S4). These results provided insight into the clinical applicability of IMRCs, especially with regards to their complete loss of pluripotency and their gain in hyper-immunomodulatory potential.
IMRCs treated with IFN-γ show hyper-immunomodulatory potency
To test the immunomodulatory capacity of IMRCs, we exposed them to the pro-inflammatory cytokine IFN-γ. We found that after stimulation with IFN-γ, both primary UCMSCs and IMRCs displayed similar characteristic morphological changes (Fig. 3a). IFN-γ stimulation also potently up-regulated IDO1 (indoleamine 2, 3-dioxygenase 1) expression in both primary UCMSCs and IMRCs, but much more significantly so in IMRCs (Fig. 3b). This is important because IDO1 has been shown to mediate immunosuppression in T cell-inflamed microenvironments through its catabolism of tryptophan and thus suppression of the tryptophan-kynurenine-aryl hydrocarbon receptor (Trp-Kyn-AhR) pathway in T cells. To further characterize IMRCs at a molecular level, we conducted genome-wide RNA profiling to compare IMRCs with UCMSCs, after IFN-γ stimulation (Fig. 3c). Hierarchical clustering revealed that IMRCs clustered separately from UCMSCs, although they appeared more similar after IFN-γ stimulation (Fig. 3d). To analyze IMRCs after IFN-γ stimulation in greater detail, we separated their differentially expressed genes into different categories and tested their overlap using Venn diagram analysis (Fig. 3e). The global differentially expressed gene analysis showed that highly expressed genes in IMRCs and UCMSCs after IFN-γ stimulation, compared with IMRCs and UCMSCs before IFN-γ stimulation, were enriched with immune response and interferon-gamma-mediated signaling pathway (Supplementary information, Fig. S5). Accordingly, we found that some pro-inflammatory genes showed lower expression while some pro-regenerative genes showed higher expression levels in IMRCs, compared to primary UCMSCs (Fig. 3f).
To confirm these findings, we performed a focused Enzyme-linked immunosorbent assay (ELISA) analysis of 48 biologically relevant chemokines and cytokines in the secretomes of both stimulated IMRCs and UCMSCs. We found that at least nine pro-inflammatory cytokines were lower in IMRCs than UCMSCs, including interleukin-6 (IL-6), IL-1β, tumor necrosis factor alpha (TNF-α), GRO-α, IFN-α2, IL-1α, IL-3, and IL-8 (Fig. 3g; Supplementary information, Fig. S6a). Furthermore, while the anti-inflammatory IL-4 was lower, the immunomodulatory cytokines IL-1RA, LIF, and RANTES were higher in IMRCs than UCMSCs (Fig. 3h). Amongst the pro-regenerative cytokines, we found that GM-CSF was similar while VEGFA, MIG and SDF-1α were higher in IMRCs than UCMSCs (Fig. 3i). To determine the immunomodulatory properties of IMRCs, we examined the effects of IMRCs on PBMCs’ proliferation and found that IMRCs significantly inhibited PHA-stimulated PBMCs’ proliferation when cocultured together at a ratio of 1:1 (Supplementary information, Fig. S6b). These results indicate that IMRCs manifest much stronger immunomodulatory and pro-regenerative functions than UCMSCs.
IMRCs suppress the pro-fibrotic effects of TGF-β1
Our scRNA-seq results also indicated that more than 99% of IMRCs expressed MMP1 compared with primary UCMSCs (< 1%) (Fig. 4a; Supplementary information, Fig. S4). Similarly, gene expression analysis by qPCR showed that IMRCs express much higher levels of MMP1 than hESCs, UCMSCs or human foreskin fibroblasts (HFF; Fig. 4b). MMP1 could be detected as a highly secreted protein in the conditioned media of IMRCs by ELISA (Fig. 4c). In addition, the secreted MMP1 was an enzymatically active and correctly processed isoform (Fig. 4d, e). To investigate the role of the IMRCs on fibrosis, the human epithelial cell line A549 was used to establish an in vitro fibrosis model. The morphology of A549 cells became myofibroblast-like after 48 h treatment with 10 ng/mL TGF-β1 (Fig. 4f). Consistent with the morphological changes, the expression of myofibroblast markers such as ACTA2, Collagen I, Collagen II, Fibronectin and TGFB1 increased, while the expression of the epithelial identity marker CDH1 was extinguished, suggesting that the A549 cells had undergone TGF-β1-induced myofibroblast transdifferentiation (Fig. 4g). Immunofluorescence and western blot analyses confirmed that TGF-β1 induced the up-regulation of collagen I and the down-regulation of E-cadherin (Fig. 4h, i). These results indicated that the A549 alveolar epithelial cells could simulate lung fibrosis in vitro. Thereafter, A549 cells were cultured with or without the conditioned media of IMRCs, along with TGF-β1 treatment. Our results showed that the IMRC conditioned media significantly ameliorated the induction of Collagen I, ACTA2 and TGFB1 expression (Fig. 4j; Supplementary information, Fig. S7a). Immunofluorescence and western blot analyses further confirmed that IMRC conditioned media could extinguish Collagen I protein expression and inhibit α-SMA protein expression during the A549-to-myofibroblast transdifferentiation (Fig. 4k–m; Supplementary information, Fig. S7b, c). These results suggested that IMRCs might be able to inhibit lung fibrosis.
Safety evaluation of IMRC transfusion into mice and monkeys
Tumorigenicity has long been an obstacle to the clinical application of cells derived from hESCs, due to the contamination of residual hESCs that could form teratomas. Our scRNA-seq showed that no residual OCT4+/SOX2+/NANOG+/TERT+/DPPA5+ hESCs remained amongst the IMRCs, and that all pluripotency gene expression had been extinguished (Fig. 5a). To ensure their short-term and long-term safety, a series of biosafety-related experiments were performed according to the “Guidelines for Human Somatic Cell Therapies and Quality Control of Cell-based Products” of China Food and Drug Administration (CFDA) (http://samr.cfda.gov.cn/WS01/CL0237/15709.html), whereupon the IMRCs were verified as suitable for use in human therapy (Supplementary information, Table S1). These biosafety-related experiments included testing for bacteria, fungi, mycoplasma, virus (by in vivo and in vitro methods), pluripotent cell residuals, tumorigenicity and biopreparation safety (endotoxin and bovine serum albumin residuals). According to these tests, the safety of the IMRCs has been verified as required by the National Institutes for Food and Drug Control (NIFDC) in China.
To track the biodistribution and long-term engraftment of IMRCs in vivo, whole-animal imaging of wild-type mice was performed at designated time points (day 0, 1, 3, 5, 7, 9, 15, 21, 27, 32, 37 and 46) after injection with DiR-labeled IMRCs (Supplementary information, Fig. S8a). Our data showed that DiR fluorescence intensity declined by half on day 5, and dropped steadily over at least 15 days, disappearing around day 46 (Fig. 5b, c; Supplementary information, Fig. S8c). No DiR fluorescence signals were observed in the control mouse. These results indicate that IMRCs never show long-term engraftment in vivo. However, IMRCs were predominantly distributed to the lung, with small amounts in the liver and spleen (Supplementary information, Fig. S8b). To assess the recruitment of IMRCs to the lung in greater detail, GFP-labeled IMRCs were used to track the distribution of IMRCs. A number of GFP-labeled IMRCs were observed in the interstitial spaces in the lung, but not in the lung capillaries (Fig. 5d). Immunofluorescence analysis of the expression of the alveolar type II epithelial cell marker SPC and the endothelial cell marker CD31 showed that neither marker was co-expressed with GFP-labeled IMRCs in the lungs of mice by day 21 (Fig. 5d). These data suggested that IMRCs are unlikely to engraft nor transdifferentiate into endothelial or epithelial cells, after homing to the interstitium of lung tissues in vivo.
To give some indication of the tumorigenic potential of IMRCs in vitro, a soft agar assay was performed (Fig. 5e). As a positive control, the PANC-1 pancreas tumor cell line showed a colony formation rate of about 30%. A small number of clones were also formed by hESCs, and the colony formation rate was about 0.5%. However, no colonies were formed by IMRCs. These results indicated that IMRCs had no tumorigenic potential as determined by this assay. Somatic mutation analysis by whole-genome sequencing also showed zero mutations in all coding and noncoding exon regions of the IMRCs genome (Fig. 5f). Tumor formation assays also confirmed that IMRCs could not form any tumors in immunodeficient mice after injection in vivo (Supplementary information, Table S1).
We also transfused different doses of IMRCs into cynomolgus monkeys (Macaca fascicularis), to evaluate the short- and long-term toxicity of IMRCs in primates. After 6 months, acute toxicity data showed that all blood biochemistry and urinalysis markers remained in the normal range (Fig. 5g, h; Supplementary information, Fig. S9a), indicating normal liver, kidney, heart, muscular, pancreatic and overall metabolic functions. Moreover, no abnormalities were observed in the long-term toxicity tests either, suggesting minimal xenogeneic rejection responses (Supplementary information, Fig. S9b; n = 18). These results indicated that IMRCs have a robust safety profile in vitro and in vivo, and could potentially provide therapeutic treatments with good safety levels for clinical potential.
IMRC transfusion treats lung injury and fibrosis in a dose-dependent manner
To evaluate the therapeutic effects of IMRCs on lung injury and fibrosis, IMRCs were administered intravenously into a bleomycin-induced model of lung injury (Fig. 6a). IMRCs ameliorated the total body weight reduction in mice exposed to bleomycin (BLM)-induced lung injury, in a dose-dependent manner (Fig. 6b). Kaplan-Meier survival curves indicated that IMRC treatment prolonged the overall survival rates (BLM group 12.5% vs 1 × 106 IMRCs 25%, 3 × 106 IMRCs 50%, 5 × 106 IMRCs 62.5% (P < 0.01)) and the median survival time (BLM group 11.5 d vs 1 × 106 IMRCs 15.5 d, 3 × 106 IMRCs 18.0 d, 5 × 106 IMRCs 21.0 d) in mice exposed to bleomycin-induced lung injury. There was a statistically significant difference between the BLM group and the 5 × 106 IMRCs group, but not the other groups (Fig. 6c). Histological staining of the lung at day 21 after bleomycin injection (inflammation phase) showed diffuse pneumonic lesions with loss of the normal alveolar architecture, septal thickening, enlarged alveoli, and increased infiltration of inflammatory cells in the interstitial and peribronchiolar areas, in the BLM lung compared with normal lung. IMRC treatment reduced alveolar thickening in the lung in a dose-dependent manner (Fig. 6d–f). Moreover, IMRC treatment reduced the number of macrophages in the lung (Fig. 6f). These results indicated that IMRC treatment can reduce inflammation in the lung after acute injury. Moreover, IMRC treatment also improved the Ashcroft score for pulmonary fibrosis in a dose-dependent manner (Fig. 6g). In particularly, IMRC treatment decreased collagen deposition in the BLM lung in a dose-dependent manner (Supplementary information, Fig. S10b, f). The expression levels of COL I, FN and α-SMA were also significant lower after IMRC treatment (Supplementary information, Fig. S10). ELISA showed that IMRC treatment reduced both TNF-α and TGF-β1 levels in the BLM lung in a dose-dependent manner (Fig. 6h, i). These results suggested that IMRCs can significantly reduce inflammation and fibrosis after lung injury, in a dose-dependent manner.
IMRC treatment of lung injury and fibrosis is superior to UCMSCs and pirfenidone injections
Pirfenidone (PFD) is an FDA-approved drug for the treatment of idiopathic pulmonary fibrosis. It works by reducing lung fibrosis through down-regulating the production of growth factors and procollagens I and II. To evaluate the efficacy of IMRC treatment, we compared it side-by-side with UCMSCs and PFD treatments of BLM-injured mice (Fig. 6j). Our results showed that IMRC treatment led to an improved amelioration of the weight reduction after BLM-induced lung injury, compared to UCMSCs or PFD treatments (Fig. 6k). Kaplan-Meier survival curves indicated that the IMRC treatments also resulted in the highest overall survival rates compared to UCMSCs or PFD treatments (BLM group 39.02%, vs IMRCs 70% (P < 0.01), UCMSCs 52.63%, PFD 65% (P < 0.05); Fig. 6l). Moreover, IMRC treatment showed the best improvement in lung morphology (Supplementary information, Fig. S11a) and the best reduction in BLM-induced edema, as measured by the lung coefficient (lung wet weight/total body weight), compared to UCMSCs or PFD treatments (Supplementary information, Fig. S11b).
Functionally, mice treated with IMRCs showed the best improvement in indices for lung capacity, including pressure-volume (PV), inspiratory capacity (IC), static compliance (Crs) and forced vital capacity (FVC) (Supplementary information, Fig. S12a–d). IMRC treatment also showed the best reduction in functional indices for lung fibrosis, including respiratory resistance (Rrs), elastic resistance (Ers), tissue damping (G) and tissue elasticity (H) were observed (Supplementary information, Fig. S12e–h). Computed tomography (CT) scans also showed that IMRC treatment led to the best improvement in lung morphology, compared to UCMSCs or PFD treatments (Supplementary information, Fig. S12i, j). In fact, measurements of the lung volume indicated that mice treated with IMRCs had the best improvement in lung volume compared to UCMSCs or PFD treatments. These results indicated that the IMRC therapy is superior to primary UCMSCs and PFD in treating lung injury and fibrosis.
Encouraged by these results, and in response to the urgency of the COVID-19 crisis in China, we pilot-tested IMRC transfusion as compassionate treatments in two severely ill COVID-19 patients who were diagnosed with ALI, as part of an expanded access program. After patient consent, IMRCs were administered intravenously in both severely ill patients. Within 14 days after IMRC transfusion, both the severely ill COVID-19 patients showed significant recovery from pneumonia, tested negative for SARS-CoV-2, and were recommended for discharge. Cytokine analysis of both patients’ plasma showed very high levels of inflammatory cytokines initially in days 1–2, as expected of the ALI-induced cytokine release syndrome that was manifesting at the point of treatment (Fig. 6m). However, by day 4–8, many pro-inflammatory cytokines were suppressed after IMRC infusion, including GRO-α, IFN-α2, IL-3, IL-9, IL-13, MCP-3, M-CSF, sCD40L and TNF-α (Fig. 6m). These results suggested that IMRCs might possess a hyper-immunomodulatory function with potential therapeutic benefits to ALI patients without other treatment options.
In this study, IMRCs were derived from self-renewing hESC cultures with serum-free reagents. Our results showed that IMRCs, while similar to primary UCMSCs, were superior in their long-term proliferative capacity, hyper-immunomodulatory and anti-fibrotic functions. In addition, the cell diameters of IMRCs were generally smaller than UCMSCs, suggesting that they pose lower risks for pulmonary embolism after injection. Detailed analysis of mice and monkeys after IMRC injections indicates that IMRCs do not engraft, nor transdifferentiate nor initiate tumorigenesis, showing excellent potential for short- and long-term safety profiles by a range of in vitro and in vivo assays. Most importantly, our experiments with the bleomycin mouse model of lung injury showed that treatments with IMRCs are superior to primary UCMSCs and the FDA-approved pirfenidone in therapeutic efficacy.
In recent years, MSC-like cells have been generated from hESCs using various protocols.18,19,22,23 However, to the best of our knowledge and in spite of significant efforts by numerous groups, previously reported studies lacked biosafety-related experiments. This has hindered their translation to clinical application. To ensure safety, a series of biosafety-related experiments were performed according to the “Guidelines for Human Somatic Cell Therapies and Quality Control of Cell-based Products” and the IMRCs were verified as suitable for use in human therapy. Our data showed that there was no teratoma formation observed after IMRC injection into the testes of NOD-SCID mice. In addition, scRNA-seq data showed no residual hESCs were detected in IMRCs and soft agar assays also showed that no colonies were formed by IMRCs. The somatic mutation analysis by whole-genome sequencing also showed no mutations in proto-oncogenes and tumor suppressor genes, nor any coding and non-coding exon regions of IMRCs. These results indicated that IMRCs have no demonstrable potential to form tumors. Moreover, IMRCs could not undergo long-term engraftment and disappeared around day 46. IMRCs did not transdifferentiate into endothelial cells nor alveolar epithelial cells in the lung. To evaluate the risks of clinical application, short- and long-term toxicity tests were performed in cynomolgus monkeys. After 6 months, both acute toxicity tests and long-term toxicity test data showed that no abnormalities were observed. These results proved that IMRCs could have an excellent safety profile and clinical potential. Moreover, the above data suggested that the therapeutic efficacy of IMRCs may not be due to long-term engraftment and direct repair of tissue, but due to their hyper-immunomodulatory and anti-fibrotic functions at inflammatory sites of tissue interstitium.
Like MSCs, the IMRCs are immunoprivileged, and can escape allogeneic immune responses through their lack of expression of HLA class II and their weak expression of HLA class I, thus making them valuable choices for allogeneic cell therapy. Moreover, it has been reported that MSCs could release immunomodulatory factors, alter the expression of surface molecules, and produce growth factors during an immune response to the inflammatory cytokines produced by T cells and antigen-presenting cells.24 These immunomodulatory factors are crucial for regulating the immune system and promoting tissue repair. Accordingly, expression of the T cell-suppressive IDO1 greatly increased in IMRCs after stimulation with the pro-inflammatory cytokine IFN-γ, even more than primary MSCs. Genome-wide RNA sequencing revealed that IMRCs and UCMSCs had different expression profiles after exposure to IFN-γ. Analysis of the secretomes of IMRCs and UCMSCs confirmed at least 9 pro-inflammatory cytokines that were lower, and several anti-inflammatory cytokines and pro-regenerative factors that were higher in IMRCs than UCMSCs. All these results suggested that IMRCs possess a hyper-immunomodulatory capacity compared to primary UCMSCs, after stimulation with IFN-γ. Thus, these cells can be administered to immunocompetent animals and human patients without the need for further immunosuppression.
Moreover, higher levels of MMP1 were secreted by IMRCs than primary UCMSCs. MMP1 plays a very important role in the process of fibrosis, by degrading existing collagens and promoting the early stages of tissue remodeling that are critical for the progression of fibrogenesis.25,26 In general, an imbalance between MMPs and TIMPs is the direct cause of fibrosis and tissue scarring. It has been reported that transplantation of human MMP1-overexpressing bone marrow-derived mesenchymal stem cells can attenuate CCL4-induced liver fibrosis in rats.27 Therefore, it is conceivable that IMRCs that highly express MMP1 may also reverse lung fibrosis. Accordingly, our data showed that the secretomes from IMRCs could reduce collagen I levels during fibrogenesis induced by TGF-β1. However, it is still unclear whether MMP1 played a direct role in the decrease of collagen I. Future work will focus on the role of MMP1 by using MMP1-knockout IMRCs in vitro and in vivo.
The mouse BLM model is similar to human ALI/ARDS during the acute inflammatory phase. Although fibroblastic foci, alveolar epithelial type 2 cells hyperplasia and honeycombing lesions are reduced compared with those in humans, indicating that the modeling of human ARDS is not complete in the mouse BLM model, injury to alveolar epithelial cells has been shown to be a common contributing factor to the pathogenesis of both human ARDS and BLM-induced mouse pulmonary injury.27,28 To test the therapeutic efficacy of IMRCs in the BLM mouse model, the delivery route and schedule of administration (e.g., single dose vs repeated doses) were carefully considered. Intravenous infusion is one of the principal delivery routes, considered to be minimally invasive, simple to use, and is the most common mode for primary MSCs delivery in diverse lung disorders.29,30 Furthermore, systemic intravenous transplantation may be a suitable administration route in other future clinical scenarios. In our present study, intravenous IMRCs improved the survival rate of mice with BLM-induced lung injury in a dose-dependent manner, by inhibiting both pulmonary inflammation and fibrosis. As demonstrated in vitro, IMRCs inhibited the production of pro-inflammatory cytokines and pro-fibrosis cytokines, such as TNF-α and TGF-β1, in lung tissue in vivo. Furthermore, lung function indicators such as PV, IC, Rrs, Crs, Ers, Rn, G, H and FVC were improved compared with the BLM group.
It should be noted that IMRCs were administered at 1 and 7 days after initiation of BLM injury, but before fibrosis has fully developed. In fact several studies have reported that primary MSCs treatments do not improve pre-established pulmonary fibrosis, while some studies suggest that primary MSCs actually exacerbate pulmonary fibrosis.31 Regarding the efficacy of IMRCs in established fibrosis, further studies are necessary and our own investigation is still ongoing. It is unclear whether primary MSCs do promote pulmonary fibrosis, but their lack of positive therapeutic effect may be due to the differences in MSC subtypes and functions, fibrosis stages after induction, species of model animals, and routes of administration of MSCs. Thus, clinical applications with MSCs should be considered carefully. As noted in this study, it is important to carefully document the origin, preparation and characterization of MSC-like cells. Here we have established a substantial profile of efficacy and safety for the hESC-derived IMRCs. These efforts provide considerable grounds for hope that this artificial cell type could provide significant clinical benefit to the treatment of inflammatory and fibrotic disease conditions.
In summary, our findings show that intravenously-delivered IMRCs inhibited both pulmonary inflammation and fibrosis after acute lung injury in vivo. IMRCs significantly improved the survival rate in a dose-dependent manner. Furthermore, the mechanism for amelioration of pulmonary injury may be mediated by the IMRCs’ paracrine action rather than their potential to differentiate and replace the damaged alveolar epithelial cells. The IMRCs’ functional inhibition of TGF-β1-induced fibrosis could also be part of its mechanism. IMRCs were superior to UCMSCs and pirfenidone in therapeutic efficacy against lung injury and fibrosis. Furthermore, IMRCs showed an excellent safety profile in both mice and monkeys. In light of recent public health crises involving pneumonia, respiratory failure, ALI and ARDS, our pre-clinical results indicate that IMRCs are ready to be carefully considered for human trials in the treatment of lung injury and fibrosis.
Materials and methods
Generation of hESC-derived IMRCs
The hESC-derived IMRCs were generated by passaging cells that are migrating out from hEBs, with serum-free reagents. The clinical hESC line (Q-CTS-hESC-2) was prepared as described previously.20 Clinical hESCs were maintained in commercially available Essential 8TM (E8) basal medium (Gibco, Carlsbad, MO, USA; A15169-01) with Essential 8TM Supplement (Gibco, A15171-01) on vitronectin-coated plates (1 µg/cm2). To generate hEBs, hESCs were dissociated into small clumps by incubating at 37 °C for 5 min with 1 mg/mL dispase (Gibco, 17105-04) and cultured to form hEBs for 5 days in KO-DMEM (Gibco, A12861-01) supplemented with 20% KOSR (Gibco, A3020902), 1 × L-glutamine (Gibco, A12860-01), 1 × NEAA (Gibco, 11140050) and 10 ng/mL bFGF (R&D systems, Minneapolis, MN, USA; 233-FB). Then, hEBs were transferred onto vitronectin-coated plates and cultured for 14 additional days. During this period, the outgrowth from the hEBs occurred. The outgrowth cells were dissociated by using Tryple (Gibco, A12859-01) and passaged at a low cell density of 1 × 104 cells per cm2 in “IMRCs Medium” consisting of α-MEM (Gibco, 12561-049) supplemented with 5% KOSR, 1% Ultroser G (Pall corporation, New York, NY, USA; 15950-017), 1 × L-glutamine, 1 × NEAA, 5 ng/mL bFGF and 5 ng/mL TGF-β (Peprotech, 96-100-21-10). Cells were passaged upon reaching ~80% confluence in IMRCs Medium. After 5 passages in culture, differentiated cultures were harvested for characterization. By this time, IMRCs displayed a fibroblastic morphology, expressed canonical “MSC-specific” surface markers including CD73, CD90, CD105 and CD29 and were negative for typical hematopoietic markers (CD45, CD34, HLA− DR).32,33
Isolation and culture of UCMSCs
Healthy full-term human placental samples were collected according to the policy of the Ethics Committee of the 306th Hospital of the Chinese People’s Liberation Army, Beijing, China. Written informed consents were obtained from all donors before this study. All the samples were used in accordance with standard experimental protocols approved by the Animal and Medical Ethical Committee of Institute of Zoology, Chinese Academy of Sciences, Beijing, China.
Briefly, the newborn umbilical cords of full-term pregnancies were obtained from the clinic and washed by PBS to remove all remnant blood. Then, the umbilical cords were cut to ~2 mm in size after removing the artery and vein. The pieces of umbilical cords were directly transferred into a 10 cm2 culture flasks in α-MEM supplemented with 5% KOSR, 1% Ultroser G, 1 × L-glutamine, 1 × NEAA and 5 ng/mL bFGF, and cultured in an atmosphere of 5% CO2 at 37 °C. UCMSCs were passaged upon reaching ~80% confluence. After 5 passages in culture, cells were harvested for characterization.
The clinical hESC line (Q-CTS-hESC-2) was prepared as described previously.20 Clinical hESCs were maintained in the commercially available Essential 8TM (E8) basal medium on vitronectin-coated plates. Cells were passaged every 5 or 6 days using Versene (Gibco, A4239101). Clinical hESCs were tested weekly for mycoplasma contamination using a Myco-detection Kit (InvivoGen, San Diego, CA, USA; rep-pt1) and endotoxin contamination was tested using a ToxinSensorTM Chromogenic LAL Endotoxin Assay Kit (GenScript, Piscataway, NJ, USA; L00350). All cultures were maintained at 37 °C, 5% CO2 and atmospheric O2 in a humidified incubator (Thermo Fisher Scientific, Waltham, MA, USA). A549 cells were purchased from Beina Biology (Shanghai, China). The cells were cultured in Ham’s F-12K medium (Gibco, 21127022) with 10% fetal bovine serum (FBS; Gibco, 10091-148) at 37 °C in 5% CO2, and were treated with 10 ng/mL TGF-β1 (R&D systems, 240-B) or IMRC conditioned medium where specified. To prepare the conditioned medium of IMRCs, IMRCs were cultured to 50% confluence in culture dishes, then, were changed to new medium. The conditioned medium was harvested after incubating IMRCs for 24 h.
At passage 5, IMRCs were harvested. Karyotype analysis and G-binding were conducted at the Chinese Academy of Medical Science & Peking Union Medical College (Beijing, China).
RNA-seq library preparation and data analysis
Total RNA was isolated from hESCs, IMRCs and UCMSCs by Trizol (Invitrogen, Waltham, MA, USA; 15596018). RNA-seq libraries were prepared with the NEBNext®UltraTM RNA Library Prep Kit for Illumina®. Sequencing was performed on an Illumina HiSeq X-Ten sequencer with 150 bp paired-end sequencing reaction. The bulk RNA-Seq data for hESCs were downloaded from GEO database.21 All RNA-sequencing data analysis was performed with Hisat2 (version 2.1.0)34 and Cufflinks (version 2.2.1)35 using the UCSC hg19 annotation with default settings. Reads with unique genome locations and genes with no less than 1 FPKM in at least one sample were used for the next step of analysis. Twofold change was used as the threshold to filter for DEGs i.e., increased or decreased expression of less than twofold was not considered significant. The Gene Ontology analysis for differentially expressed genes was performed by DAVID (version 6.8).36 Clustering, heatmap, Venn diagram and scatterplots analysis were performed with hierarchical cluster and heatmap.2 functions in R. Pearson correlation coefficient was calculated by cor.test in R. Gene set enrichment analysis were performed by GSEA.37
Cells were harvested and blocked with 2% bovine serum albumin (BSA; Sigma-Aldrich, B2064) for 20 min at room temperature. Then, the cells were stained with fluorescein-conjugated antibodies for 40 min at room temperature in 1% BSA. After incubation, cells were washed 3 times and analyzed with MoFlo (Beckman, Brea, CA, USA) and associated software. The antibodies used for flow cytometry were as follows: PE-conjugated mouse anti-human CD29 (Biolegend, San Diego, CA, USA; 303004), PE-conjugated mouse anti-human CD73 (BD Biosciences, San Jose, CA, USA; 550257), PE-conjugated mouse anti-human CD90 (eBioscience, San Diego, CA, USA; 12-0909-42), PE-conjugated mouse anti-human CD105 (Biolegend, 323206), PE-conjugated mouse anti-human CD34 (BD Biosciences, 555822), PE-conjugated mouse anti-human CD45 (BD Biosciences, 560957), PE-conjugated mouse anti-human HLA−DR (BD Biosciences, 555561), and the PE-conjugated mouse IgG1 (BD Biosciences, 551436) as an isotype control.
Osteogenic, adipogenic, and chondrogenic differentiation experiments were performed following the instructions of the human mesenchymal stem cell functional identification kit (R&D systems, SC006). For osteogenic differentiation, 4.2 × 103 cells were seeded per well in 96-well plates. When cells reached 50%–70% confluency, the medium was replaced with osteogenic differentiation medium and kept for 3 weeks. To assess osteogenic differentiation, immunofluorescence (Osteocalcin) and Alizarin Red S (Sigma-Aldrich, A5533) staining was performed for the calcium-rich extracellular matrix. For adipogenic differentiation, cells were seeded into a 24-well plate at the density of 3.7 × 104 cells/well, and maintained in culture medium until 100% confluency. Then, cells were cultured in adipogenic differentiation medium for 3 weeks. Lipid droplets of the resultant differentiated cells were detected using immunofluorescence (FABP-4) and Oil red O (Sigma-Aldrich, O0625) staining. For chondrogenic differentiation, 2.5 × 105 cells resuspended in chondrogenic differentiation medium were centrifuged for 5 min at 200 × g in a 15-mL conical tube (Corning, NY, USA). Then, cells were cultured for 3 weeks. After 3 weeks, chondrogenic pellet was harvested and fixed in 4% paraformaldehyde (Aladdin Chemical Co., Ltd., Shanghai, China; C104190). Cryosectioning was performed by OTF Cryostat (Leica, Germany) and 10 µm sections were stained with immunofluorescence (Aggrecan) and Alcian Blue (Sigma-Aldrich, A5268) staining.
IMRCs and UCMSCs were seeded into 96-well plates at a density of 8 × 103 cells per well. Cell Counting Kit-8 (CCK8; Thermo Fisher Scientific, CK04) was used to measure the cells’ growth. CCK8 solution was added at day 1, day 3, day 5 and day 7 by following the CCK8 kit manufacturer’s protocol. After 2 h of incubation, absorbance was measured at 450 nm.
Cell diameter analysis
The IMRCs and UCMSCs were harvested at passage 5 and the cell diameters were measured with ImageJ software (NIH) software analysis. Normal Distribution curves were fitted to the cell diameter data to analyze the cell size distribution characteristics.
Cell viability test
The IMRCs and UCMSCs were cryopreserved in a published clinical injection38 for 15 days in liquid nitrogen. After complete recovery of the cells, cells were suspended in clinical injection and remained under 4 °C. Then, cell viability was determined using 0.4% (w/v) Trypan Blue (Gibco, 15250061) at different time points by a Cell Counter (Invitrogen, Countess II) using the average of 3 replicates.
ScRNA-seq library preparation and sequencing
IMRCs and UCMSCs were harvested and suspended in PBS. Then, cell suspensions were loaded onto the Chromium Single Cell Controller (10 × Genomics) to generate single Gel Beads-in-Emulsion (GEMs) by using Single Cell 30 Library and Gel Bead Kit V2 (10 × Genomics, 120237). Cells were lysed and the released RNA was barcoded through reverse transcription in individual GEMs. Following reverse transcription, cDNAs with both barcodes were amplified, and a library was constructed using the Single Cell 30 Reagent Kit (v2 chemistry) for each sample following the manufacture’s introduction (performed by CapitalBio Technology, Beijing). Sequencing was performed on an Illumina NovaSeq 6000 System in the 2 × 150 bp paired-end mode. Raw files were processed with Cell Ranger using default mapping arguments. Gene expression analysis and cell type identification were performed by Seurat V3.1. Briefly, after normalizing and quality control, the tSNE was used for non-linear dimensional reduction. The figures were produced by DimPlot and VlnPlot functions in Seurat.
Cell culture with IFN-γ treatment
Cells at passage 4 were digested and seeded into 6-well plates. IMRCs were seeded at a density of 3 × 105 cells/well, and UCMSCs were seeded at a density of 2 × 105 cells/well. After adherence for 24 h, IFN-γ (0, 25 ng/mL, 50 ng/mL, 100 ng/mL) (R&D systems, 285-IF) was added into the culture medium to culture for 24 h. Cells and conditioned medium were harvested after IFN-γ stimulation for qPCR and cytokine analysis.
Conditioned medium of UCMSCs and IMRCs were collected after IFN-γ (100 ng/mL) stimulation for 24 h. Forty-eight cytokines including FGF basic, Eotaxin (also known as CCL11), G-CSF (CSF3), GMCSF (CSF2), IFN-γ, IL-1β, IL-1RA, IL-2, IL-4, IL-5, IL-6, IL-7, IL-8 (also known as CXCL8), IL-9, IL-10, IL-12 (p70), IL-13, IL-15, IL-17α, IP10 (CXCL10), MCP1 (CCL2), MIP-1α (CCL3), MIP-1β (CCL4), PDGFB, RANTES (CCL5), TNF-α, VEGF, IL-1α, IL-2Rα, IL-3, IL-12 (p40), IL-16, GRO-α, HGF, IFN-α2, LIF, MCP-3, MIG, β-NGF, SCF, SCGF-β, SDF-1α, CTACK, MIF, TRAIL, IL-18, M-CSF, TNF-β were detected by using the premixed 48-plex Bio-Plex Pro Human Cytokine Assay (Bio-Rad, Hercules, CA, USA; 12007283) according to the manufacturer’s instructions.
Lymphocyte proliferation assay
For the proliferation analysis, peripheral blood mononuclear cells (PBMCs) from umbilical cord blood of healthy donors were stimulated by 5 µg/mL phytohaemagglutinin (PHA; Sigma-Aldrich, L4144) in a 96-well plate for 3 days in the presence or absence of IMRCs (2 × 105/well) at a ratio of 1:1. At day 3, the proliferation of PBMCs was analyzed by CCK8.
For reverse transcription (RT), RNA was extracted using an RNAprep Pure Cell/Bacteria Kit (TIANGEN, Beijing, China; DP430). Two micrograms of RNA were reverse transcribed into cDNA using a PrimeScript™ First-Strand cDNA Synthesis Kit (TaKaRa, Shiga, Japan; 6110B). qPCR was performed and analyzed using a Stratagene Mx3005P system (Agilent Technologies, Santa Clara, CA, USA) with SYBR Green Real-Time PCR Master Mix Plus (Toyobo, Osaka, Japan; QPS-201). GAPDH was used for internal normalization. Primers for real-time PCR in this study are as shown in Supplementary information, Table S2.
To determine the secretion of human MMP1, cell culture supernatants were collected after 48 h of culture. The levels of human MMP1 protein were measured by a Human MMP1 ELISA Kit (Cusabio, Wuhan, China; CSB-E04672h) according to the manufacturer’s instructions. Concentrations of TNF-α (Expandbio, Beijing, China; Exp210030) and TGF-β1 (Expandbio, Exp210089) in the mouse lung homogenates were measured using ELISA kits according to the manufacturer’s instructions.
Human MMP1 activity
To determine the activity of human MMP1, cell culture supernatants were collected after 48 h of culture. The activity of human MMP1 were measured by a SensoLyte® Plus 520 MMP-1 Assay Kit (AnaSpec, San Jose, CA, USA; AS-72012) according to the manufacturer’s instructions. A specific anti-MMP-1 monoclonal antibody was used in combination with an MMP1 fluorogenic substrate, 5-FAM/QXL®520 FRET peptide. The fluorescence signal is monitored at Ex/Em = 490 nm/520 nm upon MMP-1-induced cleavage of the FRET substrate.
Cells were fixed with 4% paraformaldehyde for 15 min, permeabilized with 0.5% Triton X-100 for 15 min and blocked with 2% BSA for 60 min at room temperature. Then, the cells were stained with 1:200 mouse monoclonal IgG E-cadherin (Abcam, San Francisco, CA, USA; ab1416), 1:200 rabbit monoclonal IgG Collagen I (Cell Signaling Technology, Danvers, MA, USA; 84336), 1:200 rabbit anti-FABP-4 (Thermo Fisher Scientific, PA5-30591), 1:200 rabbit anti-Osteocalcin (Thermo Fisher Scientific, PA5-11849), 1:200 mouse anti-Aggrecan (Thermo Fisher Scientific, MA3-16888) overnight at 4 °C in 2% BSA in PBS. The cells were washed 3 times with PBS and then incubated with 1:200 Alexa Fluor 488 donkey anti-mouse IgG (H + L) (Jackson ImmunoResearch, West Grove, PA, USA; 715-545-151), 1:200 Fluorescein (Cy3) donkey anti-rabbit IgG (H + L) (Jackson ImmunoResearch, 711-165-152), 1:200 Fluorescein (Cy3) donkey anti-mouse IgG (H + L) (Jackson ImmunoResearch, 715-165-151) or Fluorescein (Cy2) donkey anti-rabbit IgG (H + L) (Jackson ImmunoResearch, 711-545-152) secondary antibodies in 2% BSA for 60 min at room temperature in the dark. The washing step was repeated before staining the nuclei with Hoechst 33342 (Invitrogen, H3570).
Cells were harvested in RIPA Lysis Buffer (strong) (CWbio, Taizhou, China; CW2333S) containing protease inhibitors (Roche, 4693124001). A total of 40 µg proteins were separated by 4%–20% gradient SDS-PAGE gels (GenScript, M42015C) and transferred to PVDF membranes (Millipore, Billerica, MA, USA; IPVH00010). The membranes were blocked at room temperature with 1% BSA for 1 h and incubated overnight at 4 °C with primary antibodies: rabbit Collagen I antibody (Cell Signaling Technology, 84336), mouse E-cadherin antibody (Abcam, ab1416), mouse α-SMA antibody (Sigma-Aldrich, A5228) and mouse β-actin antibody (Sigma-Aldrich, A1978). Then, the membranes were washed with TBST for 3 times and incubated for 1 h with a secondary antibody: anti-mouse IgG antibody (HRD) (Sigma-Aldrich, A9044) and anti-rabbit IgG antibody (HRD) (Sigma-Aldrich, A0545) at room temperature. Images were obtained using the ChemiDoc XRS + imaging system (Bio-Rad) and quantified using the Quantity One software.
Soft agar colony formation assay
Soft agarose gels were prepared according to previously published protocols.39 Cells were harvested and diluted to a cell concentration of 2.5 × 104 cells/mL, before mixing with the agarose mixture in 6-well culture plates. The plates were incubated in a 37 °C incubator for 21 days.
Adult female and male cynomolgus monkeys (3–5 years old) were housed in single quarters with a 12/12 h light/dark cycle. Animals were provided with monkey chow and enrichment food twice a day and water ad libitum. The monkey experiments were performed at the National Center for Safety Evaluation of Drugs, National Institutes of Food and Drug Control (Beijing, China). The Institutional Animal Care and Use Committee of the National Center for Safety Evaluation of Drugs approved all monkey studies (NO. IACUC-2018-k001).
Specific pathogen-free (SPF) 11- to 13-week-old C57BL/6 male mice were purchased from the Animal Center of Peking University (Beijing, China). All experimental and control mice were weight-matched, and their weights ranged from 25 to 30 g. All mice were housed in the animal care facility of the Institute of Medical Science, China-Japan Friendship Hospital. Mice were maintained under SPF conditions at room temperature (between 20 °C–24 °C), with humidity between 35%–55%, in a 12/12 h light/dark cycle, with food and water ad libitum and monitored with respect to their general state, fur condition, activity, and weight according to institutional guidelines. The mice were sacrificed at each observational time point by using intraperitoneal pentobarbital overdose. The Animal Studies Committee of the China-Japan Friendship Hospital (Beijing, China) approved all mice studies (NO.190108).
Acute toxicity and long-term toxicity test
Acute toxicity test: Low dose (2.6 × 106 cells/monkey), middle dose (2.6 × 107 cells/monkey) and high dose (1 × 108 cells/monkey) IMRCs were infused into cynomolgus monkeys (3–5 years old) by single intravenous infusion. After 6 months, their body weight, ophthalmology status, hematology, blood chemistry and urine chemistry were measured.
Long-term toxicity test: Low dose (2.6 × 106 cells/monkey) and high dose (1 × 108 cells/monkey) IMRCs, or saline, were injected into cynomolgus monkeys (3–5 years old) by intravenous infusion once a week for 22 times, after which their body weight, body temperature, food intake and organ weights were measured.
Copy number variation calling
30 × whole-genome sequencing data was produced by HiSeq X-Ten (Annoroad Gene Technology Co., Ltd) and used to analyze single nucleotide mutation changes between IMRCs and hESCs. As previously described,40 the whole-genome sequencing data was mapped to the hg19 reference genome by BWA (version 0.7.15) using the “mem” mode with default parameters. The genome coverage was calculated by bedtools.41 The normalized coverage depth for each bin was calculated by dividing the raw coverage depth by the average sequencing depth. Duplicate reads were removed and the uniquely mapped reads were retained for the copy-number variation (CNV) analysis, in which chromosomal sequences were placed into bins of 500 kb in length. The hg19 genome repeat regions annotated by RepeatMasker (http://www.repeatmasker.org) were removed from the genomic sequence before calculating the coverage. The CNV scatterplot was drawn using ggplot2.
Histological staining and immunostaining staining analysis
Mouse lung histology was performed as follows. Briefly, the lung was dehydrated, paraffin-embedded and cut into 4 µm sections. Lung sections were stained with H&E and Masson’s trichrome stain for assessment of pathological changes. Immunohistochemical staining was performed using antibodies against α-SMA (Servicebio, Wuhan, China; GB13044), Fibronectin (Servicebio, GB13091), Collagen I (Servicebio, GB13091) and GFP (Servicebio, GB13227). Immunofluorescence staining was performed using antibodies against GFP (Servicebio, GB13227), CD31 (Servicebio, GB11063-3) and SPC (Millipore, AB3786).
Labeling IMRCs with DiR dye
IMRCs were labeled with a lipophilic, near-infrared fluorescent dye 1,1-dioctadecyl-3,3,3,3-tetramethyl indotricarbocyanine iodide (DiR; YEASEN, Shanghai, China; 40757ES25). IMRCs were suspended at a concentration of 1 × 106 cells/mL and incubated with DiR buffer for 20 min at 37 °C according to the manufacturer’s protocol. After incubation, cells were centrifuged at 1000 rpm–1500 rpm for 5 min. After washing twice with PBS and resuspension, the IMRCs were preheated at 37 °C before infusion. Both DiR-labeled and unlabeled cells (5 × 106 cells in 200 µL saline) were injected via the tail vein.
In vivo imaging of IMRCs’ biodistribution
Mice were lightly anesthetized and were monitored using the in vivo imaging systems at day 0, day 1, day 3, day 5, day 7, day 9, day 15, day 21, day 27, day 32, day 37 and day 46 after tail intravenous injection of DiR-labeled IMRCs (5 × 106 cells in 200 µL saline). Serial fluorescence images were also obtained in major organs ex vivo. In order to reduce autofluorescence, the ideal filter conditions for DiR imaging were an excitation/emission spectrum in the near infrared range (750/780 nm).42,43
The flexiVentFX experimental platform was set up according to the manufacturer’s instructions. At the day 21, after 3% pentobarbital sodium (40 mg/kg) intraperitoneal injection of anesthesia, mice were fixed supine within 5–8 min, and endotracheal intubation was inserted in the middle of a tracheotomy. After computer processing, indicators of lung function required were obtained, including the inspiratory capacity (IC), respiratory resistance (Rrs), static compliance (Crs), elastic resistance (Ers), Newtonian resistance, tissue damping (G), tissue elasticity (H) and forced vital capacity (FVC).44
The lung tissue was completely removed, weighed by electronic balance, and the lung coefficient was calculated according to the formula: wet lung weight (g)/total body weight (kg).
Cell therapy in BLM mouse model of pulmonary fibrosis
The BLM mouse model was generated by intratracheal injection of 1.5 mg/kg bleomycin sulfate (BLM; Bioway, China; DP721) in normal saline under light anesthesia. The IMRCs were delivered intravenously at day 0 or day 1 or day 7 or day 14 after injury. Mice were euthanized with 50 mg/mL sodium pentobarbital (0.6 mg/10 g weight) according to published guidelines.45 Animals were killed at day 21 after BLM injury. After perfusion with normal saline, the left lungs were used for morphometric analysis while the right lungs were removed and used for other analyses.
Mouse CT scans were performed according to the manufacturer’s instructions.
Compassionate use study of two severely ill COVID-19 patients
We conducted a pilot study using GMP-grade IMRCs, under an expanded access program for compassionate use in COVID-19 patients. The pilot study was approved by the Ethics Committee of the Beijing Youan Hospital, Capital Medical University (LL-2020-010-K, Youan EC 005). After two severely ill COVID-19 patients, who tested positive for SARS-CoV-2 by qPCR and were diagnosed with ALI (aged 44–46 years; 1 male and 1 female), gave their consent and met the eligibility criteria, their serum samples were collected and processed in accordance with the ethical legislation and the guidelines of the Ethics Committee of the Beijing Youan Hospital, Capital Medical University.
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This work was supported by Beijing Municipal Science & Technology Commission (Z181100003818005 to Q.Z.), National Key Research and Development Program (2018YFA0108400 and 2017YFA0104403 to J.H., 2017YFA0105001 and 2016YFA0101502 to Liu W., 2020YFC0843900 to Q.Z., 2020YFC0841900 to B.H.), the Strategic Priority Research Program of the Chinese Academy of Sciences (XDA16030701 to Liu W., XDA16030401 to W.L., XDA16040502 to J.H.), the National Natural Science Foundation of China (31621004 to Q.Z. and W.L.), the Key Research Projects of the Frontier Science of the Chinese Academy of Sciences (QYZDY-SSW-SMC002 to Q.Z.), and China Postdoctoral Science Foundation (2019M660791 to Lei W.).
The authors declare no competing interests.
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Wu, J., Song, D., Li, Z. et al. Immunity-and-matrix-regulatory cells derived from human embryonic stem cells safely and effectively treat mouse lung injury and fibrosis. Cell Res (2020). https://doi.org/10.1038/s41422-020-0354-1