Stem Cells International

Stem Cells International / 2021 / Article
Special Issue

Developing Clinical Applications of ESCs and iPSCs

View this Special Issue

Review Article | Open Access

Volume 2021 |Article ID 5588165 | https://doi.org/10.1155/2021/5588165

Meng-Xue Xu, Li-Ping Liu, Yu-Mei Li, Yun-Wen Zheng, "The Opportunities and Challenges regarding Induced Platelets from Human Pluripotent Stem Cells", Stem Cells International, vol. 2021, Article ID 5588165, 10 pages, 2021. https://doi.org/10.1155/2021/5588165

The Opportunities and Challenges regarding Induced Platelets from Human Pluripotent Stem Cells

Academic Editor: Andrea Ballini
Received11 Feb 2021
Revised14 Apr 2021
Accepted19 Apr 2021
Published04 May 2021

Abstract

As a standard clinical treatment, platelet transfusion has been employed to prevent hemorrhage in patients with thrombocytopenia or platelet dysfunctions. Platelets also show therapeutic potential for aiding liver regeneration and bone healing and regeneration and for treating dermatological conditions. However, the supply of platelets rarely meets the rising clinical demand. Other issues, including short shelf life, strict storage temperature, and allogeneic immunity caused by frequent platelet transfusions, have become serious challenges that require the development of high-yielding alternative sources of platelets. Human pluripotent stem cells (hPSCs) are an unlimited substitution source for regenerative medicine, and patient-derived iPSCs can provide novel research models to explore the pathogenesis of some diseases. Many studies have focused on establishing and modifying protocols for generating functional induced platelets (iPlatelets) from hPSCs. To reach high efficiency production and eliminate the exogenous antigens, media supplements and matrix have been optimized. In addition, the introduction of some critical transgenes, such as c-MYC, BMI1, and BCL-XL, can also significantly increase hPSC-derived platelet production; however, this may pose some safety concerns. Furthermore, many novel culture systems have been developed to scale up the production of iPlatelets, including 2D flow systems, 3D rotary systems, and vertical reciprocal motion liquid culture bioreactors. The development of new gene-editing techniques, such as CRISPR/Cas9, can be used to solve allogeneic immunity of platelet transfusions by knocking out the expression of B2M. Additionally, the functions of iPlatelets were also evaluated from multiple aspects, including but not limited to morphology, structure, cytoskeletal organization, granule content, DNA content, and gene expression. Although the production and functions of iPlatelets are close to meeting clinical application requirements in both quantity and quality, there is still a long way to go for their large-scale production and clinical application. Here, we summarize the diverse methods of platelet production and update the progresses of iPlatelets. Furthermore, we highlight recent advances in our understanding of key transcription factors or molecules that determine the platelet differentiation direction.

1. Introduction

In mammals, platelets are produced by mature megakaryocytes (MKs) in the bone marrow and differentiate from pluripotent stem cells in hematopoietic tissues. The primary function of platelets is coagulation and hemostasis; once blood vessel injury occurs, platelets are rapidly activated, adhere to the wound, and aggregate to form a platelet clot. As a result, they are known as the “band-aids” of the bloodstream. Platelets play an executive role in the clinical treatment of blood diseases, such as acute myeloid leukemia, immune thrombocytopenia, and idiopathic thrombocytopenic purpura [1]. Platelets are overlooked immune regulators; they play significant roles in inflammation and infection [2] as they can recognize exterior pathogens and produce many chemoattractants to activate and recruit leukocytes into the site of infection and inflammation, thereby enhancing their lethality to pathogens [3].

The roles of platelets in assisting liver regeneration, bone regeneration, and in the treatment of dermatological conditions, have also increased the demand for platelets in clinical treatment [46]. The discovery of platelet-derived serotonin involved in hepatic regeneration and the correlation between impaired platelets and liver cell proliferation suggest that platelets play a significant role in liver regeneration [7, 8]. Platelet transfusion can improve CCl4-induced liver fibrosis in mice with severe combined immune deficiency [9]. The transfer of coding and regulatory RNA between platelets and hepatocytes can promote hepatocyte proliferation and liver regeneration [1012]. After hepatectomy, platelets coordinate with liver sinusoidal endothelial cells and Kupffer cells via the release of various growth factors, including human growth factor, insulin-like growth factor, and vascular endothelial growth factor (VEGF), or through direct contact with hepatocytes [1315]. As the therapeutic role of platelets in many diseases is being studied, the application of platelet-rich plasma (PRP) products has gained extensive attention in regenerative medicine. PRP is an autologous biological product derived from centrifuging or apheresis of blood and is a solution with high concentration of platelets [16, 17]. PRP treatment utilizes platelets with abundant biological factors and chemoattractive cytokines associated with tissue regeneration and remodeling.

Moreover, the hydrogel properties of activated PRP make it a suitable medicine delivery vehicle [7, 8, 18]. Platelets dynamically regulate the process of bone remodeling by releasing proinflammatory cytokines to activate the inflammatory phase of early bone healing and then enhance the repair phase of the healing process [19, 20]. PRP treatment has been widely studied in orthopedic and oral/maxillofacial injuries to aid hemostasis and musculoskeletal regeneration [5, 18, 21, 22]. Moreover, in aesthetic dermatology, PRP has been reported to have a therapeutic effect in treating hair loss caused by androgenetic alopecia [23]. Combining platelets with fractional laser or fat grafting can improve scar revision [24, 25] and may provide benefits in skin rejuvenation and dermal augmentation [26, 27]. Thus, platelet therapy is expected to be a new therapeutic avenue for regenerative medicine and tissue engineering.

Previously, donor-derived platelets were the primary platelet source for the treatment of certain clinical diseases such as idiopathic thrombocytopenic purpura (ITP). However, the insufficient supply of donor blood limits its application worldwide. The complexity and doubts surrounding platelet donation have discouraged many donors, and current blood supplies do not meet clinical needs, causing severe shortages [28]. In addition to this problem, there are also several inevitable challenges in platelet transfusion. The first is platelet preservation; platelets can only be stored at room temperature for a short time; otherwise, there is a significant risk of bacterial contamination. Although cold storage can reduce bacterial reproduction and prolong shelf life of the platelets, it also changes platelet structure, molecules, and metabolism [29]. Second, exogenous platelets may cause excessive immune rejection in platelet recipients. Frequent platelet transfusions will cause allogeneic immunity, which results from the generation of multiple antibodies, such as human leukocyte antigen (HLA) antibodies and human platelet antigen antibodies in patients. Residual red blood cells (RBCs) in platelets can also induce RBC antibody production after transfusion [30]. Exploring safe and high-quality alternative sources of platelets for clinical use will markedly benefit the field of regenerative medicine.

Pluripotent stem cells (PSCs), including embryonic stem cells (ESCs) and induced pluripotent stem cells (iPSCs), which have the advantages of unlimited self-renewal and multiple directional differentiation capabilities, have become reliable platelet sources in regenerative medicine. Numerous studies have demonstrated that iPSCs can differentiate into various functional cell types, such as cardiomyocytes, nephron progenitor cells, kidney organoids, oligodendrocyte progenitor cells, and melanocytes [3134]. Systems for generating induced platelets (iPlatelets) from human PSCs (hPSCs) have also been established using various methods [3538]. Using gene-editing techniques, such as CRISPR/CAS9, PSCs with great genetic maneuverability can be developed; this makes PSCs more convenient and useful for overcoming some difficulties currently encountered by the use of platelets, such as allogeneic immunity. Therefore, hPSC-derived iPlatelets can overcome the limitations in the current blood donor-dependent system and solve a series of problems in platelet production for clinical application in the near future. However, there are still many challenges to overcome.

This review summarizes current approaches for generating hPSC-derived iPlatelets, presents the current status, compares the advantages and disadvantages, limitations, and defects, and suggests future research direction.

2. The Progress and the Current Approaches for iPlatelets

Many previous studies have reported that MKs are an essential intermediate product during hPSC differentiation into platelets, providing a new perspective for research and blood transfusion medicine. These studies are listed in Table 1; they describe MK differentiation and platelet generation in vitro (Figure 1).


Cell sourceFeeder cellsMultiple stagesIntervention factorsSpecific markersProductionYear

hESCsOP9MKTPONot reportedHardly2006 [39]
hESCsC3H10T1/2, OP9HPC, MKVEGF, TPO, SCF, heparinCD41a+CD42b+ platelets/hESC2008 [35]
hESCsAccording to stageHemangioblasts/blast, MKBMP4, VEGF, SCF, TPOCD41a+CD42b+ platelets/MK2011 [40]
hESCs/HPC, MKBMP4, SCF, VEGF, FGF2CD41a+CD42b+Not provided2013 [41]
hPSCsC3H10T1/2HPC, MKHUVECs (2D bioreactor)CD41a+ or CD42b+Higher than static condition2013 [42]
hiPSCs/HPC, HEC, MKP, MKMultiple cytokinesCD41a+CD42b+About 30 platelets/MK2014 [38]
hPSCsC3H10T1/2, OP9HPCTAL1, GATA2Not reportedNot provided2014 [43]
hiPSCsC3H10T1/2imMKCLsBMI1, BCL-XL, c-MYCCD41a+CD42b+250 MKs/imMKCL2014 [44]
hPSCs/HPC, MKGATA1, FLI1, TAL1CD41a+/CD42b+About 7 platelets/MK2016 [45]
hPSCs/MKShear stress (3D bioreactor)β1-Tubulin1+Hoechst-CD41+CD42b+~42 platelets/MK, ~350 platelets/h2014 [46] 2016 [47]
hiPSCs/HG/CD42b+MKSCF, TPO, IL-9, IL-6FV+CD42b+Not provided2017 [48]
hiPSCsC3H10T1/2imMKCLsTurbulent flow, shear stressCD41+CD42b+~70–80 platelets/MK2018 [49]
hiPSCsC3H10T1/2, OP9HSC, HPC, MKB2M KOCD41+CD42b+Not provided2020 [50]

hESCs: human embryonic stem cells; hPSCs: human pluripotent stem cells; hiPSCs: human induced pluripotent stem cells; MK: megakaryocyte; HPC: hematopoietic progenitor cell; HEC: hematopoietic endothelial cell; MKP: megakaryocyte progenitor; HSC: hematopoietic stem cell; imMKCL: immortalized megakaryocyte progenitor cell line; TPO: thrombopoietin; VEGF: vascular endothelial growth factor; BMP4: bone morphogenetic protein 4.

As early as 2006, Gaur and his team established a genetically tractable system to differentiate human ESCs (hESCs) into MKs [39]. A coculture of OP9 stromal cells and hESCs was used to explore MK production in vitro for the first time. It was also called the conventional method or multiround replating method. On days 7 and 11, single cells derived from differentiated hESC colonies were transferred onto fresh OP9 cells and further cultured up to 17 days. Fluorescence analysis showed that approximately 20–60% of floating and loosely adherent cells expressed CD41a/CD42b, characteristic of the megakaryocyte lineage. However, this system yielded few platelets. Furthermore, hematopoietic progenitor cells (HPCs) derived from hPSCs were differentiated into MKs by adding cytokines SCF, Flt3L, and TPO [51, 52]. However, platelet production capacity was still limited. Since then, in attempts to address low yields, different differentiation systems have been established for obtaining hESC-derived platelets. Growth factors such as VEGF and ESC/iPSC-derived sacs (ES/iPS-sacs) differentiated into HPCs, thereby inducing the development of mature MKs and released platelets [35]. In this system, hESCs were cocultured with 10T1/2 or OP9 stromal cells. On day 14 of culture, ES/iPS-sacs were collected to concentrate HPCs, and the latter were then transferred onto fresh 10T1/2 or OP9 stromal cells and cultured up to day 26. With this protocol, a large number of mature platelets were efficiently obtained.

Another successful system was established by Lu et al. who found that hemangioblasts/blast cells (BCs) acted as intermediates in hPSC-derived platelet production and further produced functional MKs on a large scale [40]. In detail, hESCs were cultured in ultra-low attached plates with the addition of multiple cytokine combinations, including BMP4, VEGF, SCF, TPO, and FLT3L, in a serum-free medium for four days. This process involved the embryoid body (EB) formation, which showed excellent potential for industrial iPlatelet production and improvement in differentiation efficiency [40, 53]. The single cells generated from the EB stage were cultured in serum-free medium with multiple cytokines added for blast colony formation on day 8 and further differentiated into MKs in the presence of SCF, TPO, and IL-11 up to days 10–14. For platelet generation, OP9 stromal cells and cytokines, including SCF, TPO, and heparin, were used up to day 22 [40]. The number of platelets derived from these methods is considerable. It has been demonstrated that platelets generated from hESC-derived MKs displayed comparable ultrastructure and morphology with natural platelets and had similar characteristic properties to those of functional platelets [54, 55].

Since the feeder cells and serum addition used in the above culture systems have potential risk for introducing foreign pathogens and induce an immunogenic response in patients, substituting feeder cells and serum was researched. Salvagiotto et al. used collagen IV and a serum-free medium to induce feeder-free iPSCs into early hematopoietic progenitors, displaying the MK lineage characteristics [36]. Further technological innovation, a “spin embryoid body” method, was established for hESC differentiation towards the MK lineage in feeder-free and serum-free differentiation medium [41]. In this protocol, hESCs were cultured in a serum-free medium supplemented with BMP4, VEGF, SCF, and FGF2 to form EBs and commit cells to hematopoiesis. The cells were cultured for an additional 3–10 days in a serum-free medium with TPO, SCF, and IL-3 to stimulate megakaryopoiesis [41]. This serum- and feeder-free culture system enabled the formation of MK progenitors generated from hPSCs and then that of induced platelet-like particles; however, the platelet yield was not provided in this method.

As mentioned earlier, iPSCs provide a promising opportunity to study the ontogeny of hematopoiesis; however, xeno components, such as feeder cells or serum from foreign species, limit the clinical application of iPlatelets. Therefore, Lanza and his team established a three-step protocol that may provide scalable and fully functional platelets for clinical use [38]. This protocol was performed under feeder-free and xeno-free culture conditions, significantly reducing the contamination and immunogenicity caused by foreign serum. Human iPSCs (hiPSCs) were suspended and seeded on human collagen IV-coated plates and incubated for 24 h at 37°C under normoxic conditions in a specific medium. The next day, the cells were transferred to hypoxic conditions and cultured for 4 days, followed by normoxia. The medium contained BMP4, VEGF, and FGF. The cells were cultured in a medium containing TPO, SCF, FLT3L, IL-3, IL-6, and heparin for up to 7 days to generate MK progenitors (MKPs). Finally, MKPs were collected and cultured in an MK maturation medium containing TPO, SCF, IL-6, IL-9, and heparin in ultra-low attachment plates at 39°C for MK maturation and platelet formation. This feeder-free system produced approximately 30 platelets per iPSC-derived MK [38]. In this culture method, proportion of CD41a+CD42b+ double-positive mature MKs was as high as 80%. The subsequently produced platelets were of high purity, with a further advantage that MKP cells can be cryopreserved [38].

With the rapid breakthrough in technological manipulation, the safety and purity of platelets have improved. At the same time, a method for stable output still needs to be explored for clinical or commercial use. These developed protocols suggest that feeder cells are dispensable for platelet generation in vitro and highlight the importance of media supplements and matrix optimization for future investigation.

2.1. Key Genetic Factors during iPlatelet Generation

In addition to improving the differentiation methods mentioned above, specific genetic modifications directly affect platelet production. Previous studies have demonstrated that various tissue lineages can be differentiated from hPSCs by regulating the expression of master transcription factors [56]. Therefore, by manipulating the gene expression of hiPSCs, Takayama et al. found that the expression pattern of c-Myc was a crucial factor in determining platelet production during hiPSC differentiation into MKs in vitro [57]. Transient activation of c-Myc followed by c-Myc expression reduction was critical for MK maturation and functional platelet production. Without this intervention, the constant expression of c-Myc decreased the expression of GATA1 and nuclear factor erythroid-derived 2 p45 unit (p45NF-E2), leading to impaired production of functional platelets [57, 58]. In 2014, Igor Slukvin and his team found that transcription factors GATA2 and TAL1 induced hESC differentiation into designated erythrocyte MKPs through hemogenic endothelium intermediates [43]. Two years later, Moreau and his colleagues found that the overexpression of GATA1, FLI1, and TAL1 promoted the proliferation and differentiation of MKs. Very high cell yields and purity of MKs could be achieved using entirely chemically defined nonheterogeneous culture conditions [45].

Similarly, immortalized megakaryocyte progenitor cell lines (imMKCLs) were produced after the overexpression of exogenous genes BMI1, BCL-XL, and c-MYC under the control of the Tet-on system in PSCs, and these imMKCLs could expand for a long time and be frozen and thawed [44]. Although these methods involving viral transduction may have specific safety concerns with regards to clinical-grade manufacturing, genetic manipulations offer novel insights into the mechanisms behind megakaryopoiesis; to help develop clinically safe protocols, nonviral or nonintegrated methods or alternative small-molecule compounds should be used in the future.

CD42b (GPIba) is a key marker of functional platelets that can bind to vWF and then initially mediate the adhesion of circulating platelets to an injured site [59, 60]. A study at the Children’s Hospital of Philadelphia showed that the expression of CD42b was associated with MK maturation [48]. MKs can be classified into three subsets: low granular MKs (LGMKs), high granular MKs (HGMKs) with CD42b expression, and HGMKs without CD42b expression. A gradual decrease in the percentage of LGMKs and HG/CD42b+MKs and accumulation of apoptotic HG/CD42b-MKs indicates a reduction in platelet yield, and apoptosis inhibition plays a protective effect on MK apoptosis and CD42b exfoliation. The same study also found that HG/CD42b+MKs were more likely to induce a response in platelet activators. These MKs may be close to the peak of maturation and have the ability to endocytose coagulation factor FV into alpha-granules. Interestingly, CD42bhigh/FV+ MKs represent a subpopulation of HG/CD42b+ MKs with larger size and granularity; this indicates that FV uptake may be one of the final markers of the full MK maturity. FV-labeled MKs can release functional platelets after infusion in immunodeficient NOD/Shi-scid/IL-2Rγnull (NSG) mice, and the same phenomenon can be found in iPSC-derived MKs [45]. Besides, the uptaken FV platelets have increased clot formation and aggregation ability compared to platelets without FV. These results provide new insight into the specific stage of MK maturation and show an experimental basis for PSC differentiation into platelets. FV labeling could be a useful tool to screen mature HG/CD42b+MKs during iPlatelet generation and promote high platelet yield if further combined with bioreactors [42, 61].

Since mismatched HLA antigens are one reason for platelet transfusion failure, a new system was constructed to solve alloimmunity. Using the CRISPR/Cas9 technology to knock out the expression of the β2-microglobulin gene (B2M), an essential component of HLA class I molecules, the HLA I expression on the cell surface was successfully eliminated [38, 50]. As a result, the functional platelets produced could escape antibody-mediated cytotoxicity both in vitro and in vivo.

2.2. Scale-Up System for iPlatelet Production

The efficiency of platelet production from iPSCs in vitro under static culture conditions is lower than that observed in vivo. Many bioreactors or novel culture systems have been developed and refined to scale up iPSC-derived platelet production. A two-dimensional flow culture system was proposed by Nakagawa et al. [42], and it was a biomimetic artificial vascular system consisting of a biodegradable scaffold with an ordered array of holes that were arranged to mimic bone marrow in vivo through salt leaching. In the method, two different flows (the angle between them was 60° instead of 90°) helped to apply appropriate pressure and shear stress to the MKs, thereby promoting platelet production. Platelets derived from hESCs or hiPSCs at a 60° angle through this bioreactor showed complete integrin αIIbβ3 activation after agonist stimulation.

A rotary cell culture system was developed and applied to potentiate megakaryopoiesis, which significantly enhanced platelet generation [62]. This 3D dynamic culture system has advantages in supplying shear force, simulated microgravity, and better diffusion of nutrients and oxygen. By screening chemical compounds, growth factors, and the rotary suspension culture system, the platelet yield was ∼3.7-fold higher than that under static conditions.

Interestingly, turbulence energy, which acts as a physical regulator in thrombopoiesis in vivo, can be applied in platelet production ex vivo. Ito et al. [49] successfully generated highly efficient iPSC-derived platelets using another newly developed vertical reciprocal motion liquid culture bioreactor, VerMES. An optimal level of turbulent energy and shear stress was included in this system, which improved the platelet yield for the generation of 100 billion functional platelets from hiPSC-MKs in an 8 L VerMES independent of the cultivation scale size. The morphology and function of iPSC-derived platelets were comparable to those of donor-derived platelets. The possible explanation was that turbulent energy might promote proplatelet shedding via a cell-autonomous mechanism by soluble factors IGFBP2, MIF, and NRDC [49].

The platelet tracer technology has been further refined. It was found that the level of microtubule component molecule β1-tubulin (TUBB1), which is the main component of the cytoplasm of MKs, gradually increases with the maturation of MKs. Therefore, using CRISPR/Cas9 in β1-tubulin tagging can help monitor MK development and the generation of platelet-like particles. CRISPR/Cas9 can be applied to the high-throughput identification and validation of novel inducers of large-scale ex vivo platelet production [63]. These highly efficient and controllable methodologies represent a considerable leap in large-scale platelet production for future biomedical and clinical applications.

2.3. Functionality of iPlatelets

Many studies have been designed to evaluate whether hPSC-derived MKs and platelets have good purity and appropriate quality as normal human platelets and identify their essential functions both in vitro and in vivo. The assessment criteria for in vitro functionality and safety validation of platelets include, but are not limited to, morphology, ultrastructure, cytoskeletal organization, granule content, ploidy, gene expression, and biomarker expression [64]. Ultrastructural/morphological analyses showed that imMKCLs or other iPSC-derived MKs had similar polyploid states as primary human MKs [44]. iPlatelets have similar surface markers as blood-derived platelets; however, they have fewer platelet granules and larger cell sizes [38, 44]. iPSC-derived MKs expressed many functional specific markers such as CD41a, CD42b, and CD61, which can be used for platelet identification [35, 41]. Further, the relative expression of megakaryocytic marker gene mRNAs, such as c-Myc, GATA1, TAL1, and RUNX1, was higher in hPSC-derived MKs [41, 43, 44]. Typically, platelets show aggregated responsiveness after activation by the agonist adenosine diphosphate (ADP) because there are sites on platelets that can bind to ADP and cause a conformational change in integrin αIIbβ3 [35]. Flow cytometry analysis showed the high binding ability of iPlatelets to PAC-1 in the absence of ADP. Upon activation, iPlatelets on immobilized fibrinogen exhibited aggregates, lamellipodia, filopodia, and actin stress fibers, which induced cytoskeletal reorganization [44, 57].

Undoubtedly, the strongest evidence comes from in vivo experiments. Human normal platelets and iPSC-platelets were intravenously infused into macrophage-depleted mice to analyze the iPlatelet function in live animals. It was shown that iPSC-platelets were incorporated into developing mouse thrombus, similar to blood-derived platelets [38]. There is also evidence that iPSC-platelet kinetics is the same as that of fresh normal platelets. With high spatiotemporal resolution confocal laser microscopy, the behavior of iPlatelets upon initiation of adhesion to the injured vessel wall was dynamically observed in immunodeficient NSG mice irradiated with 2.0 Gy to induce thrombocytopenia [57, 65]. Several studies have evaluated the in vivo functions of iPlatelets, and it has been shown that iPlatelets adhered to the injured site initially, leading to thrombus formation and clot retraction [38, 40, 45]. However, some of these studies showed a limited iPlatelet thrombosis capacity compared to normal platelets [44, 45, 57].

2.4. Advantages, Limitations, and Potential Applications

Due to the unlimited self-renewal capacity of hPSCs, iPlatelets can be an ideal substitution for current donor-dependent systems. Besides, combination with CRISPR/Cas9 or other gene-editing technologies can help reduce alloimmune rejection [38, 45]. In terms of safety, iPSC-derived platelets can be irradiated to eliminate pathogens and other cell contaminations. As an intermediate, imMKCLs can expand for a long time and can also be frozen and thawed for utilization in emergencies [44]. However, there are still limitations to iPlatelet production, such as potential tumorigenicity, low yield, low functionality, and high cost [37, 38, 42, 44, 45]. The advantages and limitations of iPlatelets have been summarized and listed in Table 2.


MethodsAdvantagesLimitations

OP9/C3H10T1/2 feeder system [39]The cornerstone of hPSC-MK generationLow platelet production
Long induction period
Potential xenogenous contamination
ES-sac system [35]Identifies most effective cytokines during hPSC-MK generation
The basis for efficient production of platelets
Long induction period
Potential xenogenous contamination
Low platelet production
EB formation system [40, 66]Improves the efficiency of MK generationbased on the ES-sac system
Combined with defined serum- and animal feeder-free conditions
Provides evidence for the functionality of iPlatelets in vivo
Limited efficiency in platelet production
Feeder- or serum-free system [36]Without pathogen contaminationLimited efficiency in platelet production
HLA-universal iPlatelets [38, 50, 67]Shortens platelet production time
Increases MKP yield
Reduces the immunoreactivity of iPlatelets
Inevitable off-target effects or genome toxicity effects
Limited efficiency in platelet production
imMKCLs [44, 49]High stability and cryopreserved storage
Widely used in future clinical applications
Combined with a bioreactor system
High cost
The potential risk of exogene integration
Other genetic manipulation [43]Feasibility in genetic manipulation
Discovers new critical factors that determine the fate of iPlatelets
Inevitable off-target effects
Exogene integration may have some specific safety concerns in clinical treatment
Limited efficiency in platelet production

Lack of proper models largely restricts the exploration of pathogenesis of many diseases. Thus, patient-derived iPSCs can provide great research models that may address the above issue. For example, the induction of PSCs from patients with familial thrombocytopenia/acute myeloid leukemia showed that their ability to differentiate into HPCs and MKs was affected, which is associated with RUNX1 germline mutations in these diseases [68]. Further, Paris-Trousseau syndrome (PTSx) is caused by the lack of FLI transcription factor, an essential factor in the process of MK differentiation. To better understand the role of FLI in this disease, the platelet production ability of iPSCs derived from PTSx patients was compared with that of wild-type iPSCs, and it was suggested that FLI might influence MK clonogenic potential and the production of platelets [69].

Similarly, because MKs are rare in the bone marrow, it is difficult to explore the differences between healthy and pathological states and their effect on platelet production, especially in patients with severe megakaryocytopenia, including congenital amegakaryocytic thrombocytopenia (CAMT). In this case, iPSCs provide a useful model that mimics thrombocytopenia for patients with CAMT. Although these patient-derived iPSCs cannot produce MKs and platelets, the overexpression of MPL can restore their hematopoietic function [70].

3. Conclusion and Future Perspectives

Stable and reliable stem cells are ideal sources for advancing fundamental scientific discoveries and cell therapy in the context of megakaryopoiesis and platelet production. Many studies have demonstrated that platelets derived from hPSCs have certain features and functions analogous to normal platelets, such as the PAC-1 binding activity, the surface marker expression, and adhesion ability.

This review provides an overview of the possibilities and challenges regarding the production and use of hPSC-derived platelets. Firstly, autologous iPlatelet transfer becomes an effective avenue for averting allogeneic immune rejection. Moreover, the latest knockout technology, CRISPR/Cas9, can also effectively diminish alloimmune rejection due to the mismatched HLA. Then, platelet bioreactors are designed to mimic platelet production in vivo, exposing platelet progenitors to the architecture and intravascular shear stresses characteristic of their native microenvironment [61]. The combination of iPSCs and 3D bioreactors is a useful tool for improving platelet yields [49, 66]. Industrialized production of iPSC-derived platelets is an irresistible general trend for clinical application. With continuous efforts, platelets derived from PSCs have remarkable improvement both in quality and quantity; safety assessment and full functionality evaluation of iPlatelet transfusion are still essential, and the cost needs to be controlled. There is still a long way to go for the large-scale production and clinical application of iPlatelets. iPSC-derived platelets need further technological innovation to realize optimization in terms of scalable production and clinical feasibility.

Conflicts of Interest

There is no conflict of interest regarding the publication of this paper.

Authors’ Contributions

LPL and YWZ conceived and designed the study. MXX drafted the manuscript. LPL, YWZ, and MXX contributed to reviewing, discussing, and revising the manuscript. All authors approved the final manuscript. LPL and MXX contributed equally to this work. YML supplied resources and materials. YML and YWZ are senior authors and co-correspondents of this work.

Acknowledgments

We thank Dr. YX Zhang, Dr. H Sun, and other members of staff at our laboratory for scientific comments and valuable discussion. This research was supported partly by the National Natural Science Foundation of China (82070638 and 81770621), the Ministry of Education, Culture, Sports, Science, and Technology of Japan, KAKENHI (18H02866), and the Natural Science Foundation of Jiangsu Province (BK20180281).

References

  1. P. J. Vinholt, “The role of platelets in bleeding in patients with thrombocytopenia and hematological disease,” Clinical Chemistry and Laboratory Medicine (CCLM), vol. 57, no. 12, pp. 1808–1817, 2019. View at: Publisher Site | Google Scholar
  2. R. Storey and M. Thomas, “The role of platelets in inflammation,” Thrombosis and Haemostasis, vol. 114, no. 9, pp. 449–458, 2015. View at: Publisher Site | Google Scholar
  3. C. N. Jenne and P. Kubes, “Platelets in inflammation and infection,” Platelets, vol. 26, no. 4, pp. 286–292, 2015. View at: Publisher Site | Google Scholar
  4. X. Wang, Y. Zhang, J. Choukroun, S. Ghanaati, and R. J. Miron, “Effects of an injectable platelet-rich fibrin on osteoblast behavior and bone tissue formation in comparison to platelet-rich plasma,” Platelets, vol. 29, no. 1, pp. 48–55, 2018. View at: Publisher Site | Google Scholar
  5. L. C. Garbin and C. S. Olver, “Platelet-rich products and their application to osteoarthritis,” J Equine Vet Sci, vol. 86, article 102820, 2020. View at: Publisher Site | Google Scholar
  6. P. Samadi, M. Sheykhhasan, and H. M. Khoshinani, “The use of platelet-rich plasma in aesthetic and regenerative medicine: a comprehensive review,” Aesthetic Plastic Surgery, vol. 43, no. 3, pp. 803–814, 2019. View at: Publisher Site | Google Scholar
  7. M. Lesurtel, R. Graf, B. Aleil et al., “Platelet-derived serotonin mediates liver regeneration,” Science, vol. 312, no. 5770, pp. 104–107, 2006. View at: Publisher Site | Google Scholar
  8. S. Murata, N. Ohkohchi, R. Matsuo, O. Ikeda, A. Myronovych, and R. Hoshi, “Platelets promote liver regeneration in early period after hepatectomy in mice,” World Journal of Surgery, vol. 31, no. 4, pp. 808–816, 2007. View at: Publisher Site | Google Scholar
  9. K. Takahashi, S. Murata, K. Fukunaga, and N. Ohkohchi, “Human platelets inhibit liver fibrosis in severe combined immunodeficiency mice,” World Journal of Gastroenterology, vol. 19, no. 32, pp. 5250–5260, 2013. View at: Publisher Site | Google Scholar
  10. M. Kirschbaum, G. Karimian, J. Adelmeijer, B. N. G. Giepmans, R. J. Porte, and T. Lisman, “Horizontal RNA transfer mediates platelet-induced hepatocyte proliferation,” Blood, vol. 126, no. 6, pp. 798–806, 2015. View at: Publisher Site | Google Scholar
  11. T. Lisman, M. Kirschbaum, and R. J. Porte, “The role of platelets in liver regeneration - what don't we know?” Journal of Hepatology, vol. 63, no. 6, pp. 1537-1538, 2015. View at: Publisher Site | Google Scholar
  12. J. Meyer, E. Lejmi, P. Fontana, P. Morel, C. Gonelle-Gispert, and L. Bühler, “A focus on the role of platelets in liver regeneration: do platelet-endothelial cell interactions initiate the regenerative process?” Journal of Hepatology, vol. 63, no. 5, pp. 1263–1271, 2015. View at: Publisher Site | Google Scholar
  13. T. Kurokawa, Y. W. Zheng, and N. Ohkohchi, “Novel functions of platelets in the liver,” Journal of Gastroenterology and Hepatology, vol. 31, no. 4, pp. 745–751, 2016. View at: Publisher Site | Google Scholar
  14. M. Bilzer, F. Roggel, and A. L. Gerbes, “Role of Kupffer cells in host defense and liver disease,” Liver International, vol. 26, no. 10, pp. 1175–1186, 2006. View at: Publisher Site | Google Scholar
  15. R. Malik, C. Selden, and H. Hodgson, “The role of non-parenchymal cells in liver growth,” Seminars in Cell & Developmental Biology, vol. 13, no. 6, pp. 425–431, 2002. View at: Publisher Site | Google Scholar
  16. R. E. Marx, “Platelet-rich plasma: evidence to support its use,” Journal of Oral and Maxillofacial Surgery, vol. 62, no. 4, pp. 489–496, 2004. View at: Publisher Site | Google Scholar
  17. S. Lang, M. Loibl, and M. Herrmann, “Platelet-rich plasma in tissue engineering: hype and hope,” European Surgical Research, vol. 59, no. 3-4, pp. 265–275, 2018. View at: Publisher Site | Google Scholar
  18. J. Etulain, “Platelets in wound healing and regenerative medicine,” Platelets, vol. 29, no. 6, pp. 556–568, 2018. View at: Publisher Site | Google Scholar
  19. A. Moshiri, A. Oryan, and A. Meimandi-Parizi, “Role of embedded pure xenogenous bovine platelet gel on experimental tendon healing, modelling and remodelling,” BioDrugs, vol. 28, no. 6, pp. 537–556, 2014. View at: Publisher Site | Google Scholar
  20. G. Y. Li, J. M. Yin, H. Ding, W. T. Jia, and C. Q. Zhang, “Efficacy of leukocyte- and platelet-rich plasma gel (L-PRP gel) in treating osteomyelitis in a rabbit model,” Journal of Orthopaedic Research, vol. 31, no. 6, pp. 949–956, 2013. View at: Publisher Site | Google Scholar
  21. S. Ahmadipour, J. Varshosaz, B. Hashemibeni, L. Safaeian, and M. Manshaei, “Polyhedral oligomeric silsesquioxane /platelets rich plasma/gelrite-based hydrogel scaffold for bone tissue engineering,” Current Pharmaceutical Design, vol. 26, no. 26, pp. 3147–3160, 2020. View at: Publisher Site | Google Scholar
  22. A. Oryan, S. Alidadi, and A. Moshiri, “Platelet-rich plasma for bone healing and regeneration,” Expert Opinion on Biological Therapy, vol. 16, no. 2, pp. 213–232, 2016. View at: Publisher Site | Google Scholar
  23. K. W. Badran and J. P. Sand, “Platelet-rich plasma for hair loss: review of methods and results,” Facial Plastic Surgery Clinics of North America, vol. 26, no. 4, pp. 469–485, 2018. View at: Publisher Site | Google Scholar
  24. V. Cervelli, F. Nicoli, D. Spallone et al., “Treatment of traumatic scars using fat grafts mixed with platelet-rich plasma, and resurfacing of skin with the 1540 nm nonablative laser,” Clinical and Experimental Dermatology, vol. 37, no. 1, pp. 55–61, 2012. View at: Publisher Site | Google Scholar
  25. J. T. ZHU, M. XUAN, Y. N. ZHANG et al., “The efficacy of autologous platelet-rich plasma combined with erbium fractional laser therapy for facial acne scars or acne,” Molecular Medicine Reports, vol. 8, no. 1, pp. 233–237, 2013. View at: Publisher Site | Google Scholar
  26. A. Trink, E. Sorbellini, P. Bezzola et al., “A randomized, double-blind, placebo- and active-controlled, half-head study to evaluate the effects of platelet-rich plasma on alopecia areata,” The British Journal of Dermatology, vol. 169, no. 3, pp. 690–694, 2013. View at: Publisher Site | Google Scholar
  27. M. S. Leo, A. S. Kumar, R. Kirit, R. Konathan, and R. K. Sivamani, “Systematic review of the use of platelet-rich plasma in aesthetic dermatology,” Journal of Cosmetic Dermatology, vol. 14, no. 4, pp. 315–323, 2015. View at: Publisher Site | Google Scholar
  28. X. H. Liang, S. H. Zhou, Y. X. Fan et al., “A survey of the blood supply in China during 2012-2014,” Transfusion Medicine, vol. 29, no. 1, pp. 28–32, 2019. View at: Publisher Site | Google Scholar
  29. T. M. Getz, “Physiology of cold-stored platelets,” Transfusion and Apheresis Science, vol. 58, no. 1, pp. 12–15, 2019. View at: Publisher Site | Google Scholar
  30. P. Moncharmont, “Platelet component transfusion and alloimmunization: where do we stand?” Transfusion Clinique et Biologique, vol. 25, no. 3, pp. 172–178, 2018. View at: Publisher Site | Google Scholar
  31. P. Douvaras and V. Fossati, “Generation and isolation of oligodendrocyte progenitor cells from human pluripotent stem cells,” Nature Protocols, vol. 10, no. 8, pp. 1143–1154, 2015. View at: Publisher Site | Google Scholar
  32. L. P. Liu, Y. M. Li, N. N. Guo et al., “Therapeutic potential of patient iPSC-derived iMelanocytes in autologous transplantation,” Cell Reports, vol. 27, no. 2, pp. 455–466.e5, 2019, e5. View at: Publisher Site | Google Scholar
  33. C. L. Mummery, J. Zhang, E. S. Ng, D. A. Elliott, A. G. Elefanty, and T. J. Kamp, “Differentiation of human embryonic stem cells and induced pluripotent stem cells to cardiomyocytes,” Circulation Research, vol. 111, no. 3, pp. 344–358, 2012. View at: Publisher Site | Google Scholar
  34. R. Morizane and J. V. Bonventre, “Generation of nephron progenitor cells and kidney organoids from human pluripotent stem cells,” Nature Protocols, vol. 12, no. 1, pp. 195–207, 2017. View at: Publisher Site | Google Scholar
  35. N. Takayama, H. Nishikii, J. Usui et al., “Generation of functional platelets from human embryonic stem cells in vitro via ES-sacs, VEGF-promoted structures that concentrate hematopoietic progenitors,” Blood, vol. 111, no. 11, pp. 5298–5306, 2008. View at: Publisher Site | Google Scholar
  36. G. Salvagiotto, S. Burton, C. A. Daigh, D. Rajesh, I. I. Slukvin, and N. J. Seay, “A defined, feeder-free, serum-free system to generate in vitro hematopoietic progenitors and differentiated blood cells from hESCs and hiPSCs,” PLoS One, vol. 6, no. 3, article e17829, 2011. View at: Publisher Site | Google Scholar
  37. N. Takayama and K. Eto, “In vitro generation of megakaryocytes and platelets from human embryonic stem cells and induced pluripotent stem cells,” Methods in Molecular Biology, vol. 788, pp. 205–217, 2012. View at: Publisher Site | Google Scholar
  38. Q. Feng, N. Shabrani, J. N. Thon et al., “Scalable generation of universal platelets from human induced pluripotent stem cells,” Stem Cell Reports, vol. 3, no. 5, pp. 817–831, 2014. View at: Publisher Site | Google Scholar
  39. M. GAUR, T. KAMATA, S. WANG, B. MORAN, S. J. SHATTIL, and A. D. LEAVITT, “Megakaryocytes derived from human embryonic stem cells: a genetically tractable system to study megakaryocytopoiesis and integrin function,” Journal of Thrombosis and Haemostasis, vol. 4, no. 2, pp. 436–442, 2006. View at: Publisher Site | Google Scholar
  40. S.-J. Lu, F. Li, H. Yin et al., “Platelets generated from human embryonic stem cells are functional in vitro and in the microcirculation of living mice,” Cell Research, vol. 21, no. 3, pp. 530–545, 2011. View at: Publisher Site | Google Scholar
  41. M. Pick, L. Azzola, E. Osborne, E. G. Stanley, and A. G. Elefanty, “Generation of megakaryocytic progenitors from human embryonic stem cells in a feeder- and serum-free medium,” PLoS One, vol. 8, no. 2, article e55530, 2013. View at: Publisher Site | Google Scholar
  42. Y. Nakagawa, S. Nakamura, M. Nakajima et al., “Two differential flows in a bioreactor promoted platelet generation from human pluripotent stem cell-derived megakaryocytes,” Experimental Hematology, vol. 41, no. 8, pp. 742–748, 2013. View at: Publisher Site | Google Scholar
  43. I. Elcheva, A. Kumar, P. Liu et al., “Direct induction of haematoendothelial programs in human pluripotent stem cells by transcriptional regulators,” Nature Communications, vol. 5, no. 1, p. 4372, 2014. View at: Publisher Site | Google Scholar
  44. S. Nakamura, N. Takayama, S. Hirata et al., “Expandable megakaryocyte cell lines enable clinically applicable generation of platelets from human induced pluripotent stem cells,” Cell Stem Cell, vol. 14, no. 4, pp. 535–548, 2014. View at: Publisher Site | Google Scholar
  45. T. Moreau, A. L. Evans, L. Vasquez et al., “Large-scale production of megakaryocytes from human pluripotent stem cells by chemically defined forward programming,” Nature Communications, vol. 7, no. 1, article 11208, 2016. View at: Publisher Site | Google Scholar
  46. J. N. Thon, L. Mazutis, S. Wu et al., “Platelet bioreactor-on-a-chip,” Blood, vol. 124, no. 12, pp. 1857–1867, 2014. View at: Publisher Site | Google Scholar
  47. A. Blin, A. le Goff, A. Magniez et al., “Microfluidic model of the platelet-generating organ: beyond bone marrow biomimetics,” Scientific Reports, vol. 6, no. 1, article 21700, 2016. View at: Publisher Site | Google Scholar
  48. X. Sim, D. Jarocha, V. Hayes et al., “Identifying and enriching platelet-producing human stem cell-derived megakaryocytes using factor V uptake,” Blood, vol. 130, no. 2, pp. 192–204, 2017. View at: Publisher Site | Google Scholar
  49. Y. Ito, S. Nakamura, N. Sugimoto et al., “Turbulence Activates Platelet Biogenesis to Enable Clinical Scale _Ex Vivo_ Production,” Cell, vol. 174, no. 3, pp. 636–648.e18, 2018. View at: Publisher Site | Google Scholar
  50. P. Norbnop, P. Ingrungruanglert, N. Israsena, K. Suphapeetiporn, and V. Shotelersuk, “Generation and characterization of HLA-universal platelets derived from induced pluripotent stem cells,” Scientific Reports, vol. 10, no. 1, p. 8472, 2020. View at: Publisher Site | Google Scholar
  51. C. E. Murry and G. Keller, “Differentiation of embryonic stem cells to clinically relevant populations: lessons from embryonic development,” Cell, vol. 132, no. 4, pp. 661–680, 2008. View at: Publisher Site | Google Scholar
  52. J. A. Mills, P. Paluru, M. J. Weiss, P. Gadue, and D. L. French, “Hematopoietic differentiation of pluripotent stem cells in culture,” Methods in Molecular Biology, vol. 1185, pp. 181–194, 2014. View at: Publisher Site | Google Scholar
  53. N.-N. Guo, L.-P. Liu, Y.-W. Zheng, and Y.-M. Li, “Inducing human induced pluripotent stem cell differentiation through embryoid bodies: a practical and stable approach,” World J Stem Cells, vol. 12, no. 1, pp. 25–34, 2020. View at: Publisher Site | Google Scholar
  54. S. J. Lu, C. Luo, K. Holton, Q. Feng, Y. Ivanova, and R. Lanza, “Robust generation of hemangioblastic progenitors from human embryonic stem cells,” Regenerative Medicine, vol. 3, no. 5, pp. 693–704, 2008. View at: Publisher Site | Google Scholar
  55. S. J. Lu, Q. Feng, S. Caballero et al., “Generation of functional hemangioblasts from human embryonic stem cells,” Nature Methods, vol. 4, no. 6, pp. 501–509, 2007. View at: Publisher Site | Google Scholar
  56. R. Sugimura, D. K. Jha, A. Han et al., “Haematopoietic stem and progenitor cells from human pluripotent stem cells,” Nature, vol. 545, no. 7655, pp. 432–438, 2017. View at: Publisher Site | Google Scholar
  57. N. Takayama, S. Nishimura, S. Nakamura et al., “Transient activation of c-MYC expression is critical for efficient platelet generation from human induced pluripotent stem cells,” The Journal of Experimental Medicine, vol. 207, no. 13, pp. 2817–2830, 2010. View at: Publisher Site | Google Scholar
  58. S. Masuda, M. Li, and J. C. Izpisua Belmonte, “In vitro generation of platelets through direct conversion: first report in my knowledge (iMK),” Cell Research, vol. 23, no. 2, pp. 176–178, 2013. View at: Publisher Site | Google Scholar
  59. J. Ware, S. Russell, and Z. M. Ruggeri, “Generation and rescue of a murine model of platelet dysfunction: the Bernard-Soulier syndrome,” Proceedings of the National Academy of Sciences of the United States of America, vol. 97, no. 6, pp. 2803–2808, 2000. View at: Publisher Site | Google Scholar
  60. W. Bergmeier, P. C. Burger, C. L. Piffath et al., “Metalloproteinase inhibitors improve the recovery and hemostatic function of in vitro-aged or -injured mouse platelets,” Blood, vol. 102, no. 12, pp. 4229–4235, 2003. View at: Publisher Site | Google Scholar
  61. J. N. Thon, B. J. Dykstra, and L. M. Beaulieu, “Platelet bioreactor: accelerated evolution of design and manufacture,” Platelets, vol. 28, no. 5, pp. 472–477, 2017. View at: Publisher Site | Google Scholar
  62. Y. Yang, C. C. Liu, X. Lei et al., “Integrated biophysical and biochemical signals augment megakaryopoiesis and thrombopoiesis in a three-dimensional rotary culture system,” Stem Cells Translational Medicine, vol. 5, no. 2, pp. 175–185, 2016. View at: Publisher Site | Google Scholar
  63. H. Seo, S. J. Chen, K. Hashimoto et al., “A β1-tubulin–based megakaryocyte maturation reporter system identifies novel drugs that promote platelet production,” Blood Advances, vol. 2, no. 17, pp. 2262–2272, 2018. View at: Publisher Site | Google Scholar
  64. J. N. Thon, D. A. Medvetz, S. M. Karlsson, and J. E. Italiano Jr., “Road blocks in making platelets for transfusion,” Journal of Thrombosis and Haemostasis, vol. 13, pp. S55–S62, 2015. View at: Publisher Site | Google Scholar
  65. H. Takizawa, S. Nishimura, N. Takayama et al., “Lnk regulates integrin alphaIIbbeta3 outside-in signaling in mouse platelets, leading to stabilization of thrombus development in vivo,” The Journal of Clinical Investigation, vol. 120, no. 1, pp. 179–190, 2010. View at: Publisher Site | Google Scholar
  66. S.-J. Lu, T. Kelley, and Q. Feng, “3D microcarrier system for efficient differentiation of human induced pluripotent stem cells into hematopoietic cells without feeders and serum,” Regenerative Medicine, vol. 8, no. 4, pp. 413–424, 2013. View at: Publisher Site | Google Scholar
  67. C. Gras, K. Schulze, L. Goudeva, C. A. Guzman, R. Blasczyk, and C. Figueiredo, “HLA-universal platelet transfusions prevent platelet refractoriness in a mouse model,” Human Gene Therapy, vol. 24, no. 12, pp. 1018–1028, 2013. View at: Publisher Site | Google Scholar
  68. M. Sakurai, H. Kunimoto, N. Watanabe et al., “Impaired hematopoietic differentiation of RUNX1-mutated induced pluripotent stem cells derived from FPD/AML patients,” Leukemia, vol. 28, no. 12, pp. 2344–2354, 2014. View at: Publisher Site | Google Scholar
  69. K. K. Vo, D. J. Jarocha, R. B. Lyde et al., “FLI1 level during megakaryopoiesis affects thrombopoiesis and platelet biology,” Blood, vol. 129, no. 26, pp. 3486–3494, 2017. View at: Publisher Site | Google Scholar
  70. S. Hirata, N. Takayama, R. Jono-Ohnishi et al., “Congenital amegakaryocytic thrombocytopenia iPS cells exhibit defective MPL-mediated signaling,” Journal of Clinical Investigation, vol. 123, no. 9, pp. 3802–3814, 2013. View at: Publisher Site | Google Scholar

Copyright © 2021 Meng-Xue Xu et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.


More related articles

 PDF Download Citation Citation
 Download other formatsMore
 Order printed copiesOrder
Views84
Downloads90
Citations

Related articles