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Introduction
Since Schofield presented the “niche concept” in the 1970s (1), it has been recognized that the bone marrow (BM) microenvironment is important in controlling the biological characteristics of hematopoietic stem cells (HSC) with the support of cell populations such as osteoblasts, neurons, mesenchymal stem cells (MSC) and endothelial cells (Ec), among other cells (2, 3). Several studies have shown that these interactions between HSC and other cellular populations in the BM are organized in two main complex niches: endosteal, close to the bone and influenced by osteoblasts, osteocytes, osteoclasts and vascular formed by sinusoids, arterioles and different populations of mesenchymal cells (stem cells and progenitors of bone lineage, cartilage and adipose tissue) (3, 4). In particular, the vascular niche is constituted of Ec, which forms a network of sinusoids and arterioles to which perivascular stromal cells from the heterogeneous group of BM-MSC are associated (5, 6). Ec participate in the homeostasis of hematopoiesis by secreting angiogenic factors that stimulate the proliferation and self-renewal of HSC by increasing the expression of factors such as IGFBP2, FGF2, BMP4 and DHH (7) and direct contact through E-selectin that promotes the quiescence of hematopoietic cells (8); furthermore, Ec has been shown to promote the long-term maintenance of HSC in vitro (9, 10).
Similarly, BM-MSC have an important role in the regulation of HSC. These cells, which express common mesenchymal antigens such as CD73 and CD105 or particular antigens (according to the subtype) such as CD146, CXCL-12 (CAR cells), nestin and leptin receptor (LepR), have in common the secretion of two determining soluble factors for HSC: CXCL-12 (SDF-1) and SCF (11, 12), which participate in maintaining the viability, self-renewal and mobilization of hematopoietic cells. Some MSC populations of the vascular niche are more resistant to chemotherapy and induce the regeneration of HSC after exposure to cytotoxic agents (13), and in vitro, they can maintain the phenotypic and functional characteristics of HSC of umbilical cord blood and leukemic cells (14, 15).
These findings demonstrate that the Ec and MSC of the microenvironment BM have a determining role in the regulation of the mechanisms that maintain the homeostasis of the HSC; however, to deepen our understanding of role of the microenvironment in the regenerative capacity of HSC and the knowledge about the maintenance of cancer stem cells and thus be able to propose therapeutic strategies, it is necessary to develop experimental systems that imitate the microenvironment of human HSC with the simultaneous use of the different cell populations that reside in the niches of the hematopoietic cells. The use of animal models has allowed significant advancements in the knowledge of the microenvironment of HSC (16–18); however, studies show that murine HSC and human HSC interact differently with cells in the bone marrow microenvironment (19) and that species-specific differences may exist (20). An interesting alternative for the study of the microenvironment of human HSC is the development of organotypic multicellular spheres (OMS) that mimic the niches of human cells (21). In this work, we propose a new system of 3D culture by magnetic levitation, which does not use scaffolds or exogenous matrices and allows the cells to form their own extracellular matrix, to evaluate the role of Ec and MSC in the behavior of the human HSC as a future tool for the development of a complex organoid that imitates the microenvironment of the human BM.
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Materials and Methods
Isolation and culture conditions of human MSC and Ec
To obtain MSC, bone marrow (BM) samples were obtained with the support of the Department of Orthopedics and Traumatology of Hospital Universitario San Ignacio (Bogota, Colombia) from volunteer donors (undergoing hip replacement surgery) after signing the informed consent form approved by the Hospital Ethics Committee. BM-MSC were isolated and cultured as previously published (14, 15), and they were used in passages 3–5 for a 3D culture system. The BM-MSC phenotype was assessed by flow cytometry with a FACS Aria-II cytometer (BD Biosciences). For data analysis, the DIVA (BD Biosciences) and FlowJo software were used. A BM-MSC functional assay was performed according to previous reports (14, 15) with StemPro Osteogenesis, StemPro Adipogenesis and StemPro Chondrogenesis Differentiation Kits (Invitrogen). A non-tumor cell line, Human Dermal Microvascular Endothelial Cells (CC-2811, Lonza), was used. The endothelial cells were cultured in an EGM-2 Bullet medium kit (Lonza) at a density of 5×103/cm2 at 37°C and 5% CO2. The viability of the cell populations was monitored permanently with trypan blue staining.
Isolation and characterization of HSC from human umbilical cord blood (UCB)
To obtain HSC, umbilical cord blood (UCB) samples were obtained with the support of the Department of Gynecology and Obstetrics of Hospital Universitario San Ignacio (Bogota, Colombia) from normal full-term deliveries after obtaining informed consent in accordance with the guidelines approved by the Hospital Ethics Committee. Mononuclear cells were isolated by Ficoll density gradient centrifugation (Histopaque d=1.077 g/cm3, Sigma-Aldrich), and CD34+ cells were isolated using a previously described magnetic-activated cell-sorting (MACS) CD34 isolation kit (Miltenyi Biotec) (15). Cell purity was evaluated by flow cytometry, and cell viability was determined using trypan blue staining.
Generation of the 3D cultivation system by magnetic levitation
To develop a 3D culture system that mimics the microenvironment of the bone marrow, a 3D Bio AssemblerTM System (Nano3D Biosciences, Inc.) was used with the three cell populations of interest (MSC, Ec and HSC). It was formed of a 24-Well Bio-AssemblerTM Kit with nanoparticles (NanoShuttleTM-PL) coated with iron oxide (Fe2O3), gold and poly-lysine-L, magnetic drag plates (24-Well Magnetic Drive®) and ultra-low adhesion plates (Ultra Low Adhesion 24-Well Plates®). Each of the isolated and characterized cell populations (MSC, Ec and HSC) was independently cultured with 400 μl of triple medium formed in equal parts of serum-free medium for MSC (StemPro MSC SFM CTSTM, GIBCO, Life Technologies), HSC (StemPro34 SFM, GIBCO, Life Technologies) and Ec (Endothelial Cell Growth Medium, EGMTM -2 BulletKitTM Lonza), with a ratio of 1 μl of nanoparticles per 1×104 cells (22) for 12 hours at 37°C and 5% CO2. Then, all cells were collected and mixed in the ultra-low adhesion plate (Ultra Low Adhesion 24-Well Plates®) with 400 μl of triple medium, and a magnetic drag plate (24-Well Magnetic Drive®) was assembled and incubated for 120 hours at 37°C and 5% CO2. To define the optimal relationship between the volume of nanoparticles and cell density in the 3D culture system, the morphology of the structure obtained (organotypic multicellular spheres, OMS) was evaluated by inverted microscopy, and the global DNA content was determined with a High Pure PCR Template Preparation Kit (Roche) and NanoDrop 2000 (Thermo Scientific) in two different cell-to-cell densities, MSC: Ec: HSC=1:5:5 and 1:2:2 with 1×105 total cell density per well.
Evaluation of OMS: volume, sphericity, aggregation and viability
To calculate the volume and sphericity of the structures obtained by the 3D culture method by magnetic levitation, a photographic record of the spheres was made during days 5, 10 and 15 of culture; then, with the ImageJ® software, the data of area (A), perimeter (P) and diameter (D) were obtained. The volume (V) was determined according to V=4π/3 (P/π)3 (23), and the sphericity (Φ) was determined with the calculation Φ=π(✓4A/π)/P (23). The percentage of aggregation (%Ag) in the sphere was calculated to determine the loss of cells during the formation of the structure (5 day), it was determined according to Martin et al. (24) (% Ag=100 (TC-SC)/TC; TC: total number of plated cells, SC: number of single cells counted after filtering. To determine the viability of the OMS, a LIVE/DEADTM Cell Imaging Kit (Invitrogen) was used following the manufacturer’s instructions. 3D structures were imaged with laser scanning confocal microscope FV1000 (Olympus) using an UPLSAPO 20X (1.35 NA oil immersion objective), 488 nm argon laser line for green fluorescence (living cells) and HeNe 543 nm laser for red fluorescence (dead cells). Data analysis was performed with the FlowView and Fiji software. Previous studies have shown that the addition of cytokines during the in vitro expansion of HSC favors their viability and proliferation (25, 26). To determine whether the OMS obtained were autonomous in the maintenance of long-term HSC (10 and 15 days of culture) or required exogenous cytokines, an addition of Flt3-L (100 ng/ml) was used (27).
Histochemical characteristics of spheres
To evaluate the internal structure of the OMS, they were manipulated with the MagPenTM (Nano3D Biosciences, Inc.) and embedded in paraffin. Then, 3-μm-thick sections were cute, deparaffinized and stained in the Pathology Department of San Ignacio University Hospital (Bogotá, Colombia). The sections were stained with hematoxylin-eosin. The expression of vimentin (clone V9, IgG1. Agilent®) was determined by immunohistochemistry and Ki67 antigen was detected by confocal microscopy (clone 4A1, Thermo Scientific®, dilution 1/200). To determine the percentage of expression of Ki67, the total area of the sphere was determined according to the expression of α-tubulin and the expression area of Ki67 with the use of ImageJ® software, then the area of expression of the antigen (Ki67) was calculated with the following formula: Ki67 (%)=Ki67 area (μm)*100/α-tubulin area (μm).
Functional evaluation of HSC
To evaluate the maintenance of the biological characteristics of the HSC cultured in the OMS, the multipotent capacity of HSC was evaluated after 10 and 15 days of the 3D culture. To isolate the HSC from the OMS, an enzymatic treatment with 1X trypsin and EDTA (Gibco Life Technologies) was performed for 30 minutes at 37°C. Subsequently, HSC were sorted by a negative selection using anti-CD105 antibody (antigen expressed by MSC and Ec) and LS columns (magnetic-activated cell-sorting, MACS. Miltenyi Biotec). From the collected HSC, a new determination was made by flow cytometry to evaluate the purity of the recovered hematopoietic cell population, and a multipotency test was performed with the use of the HSC-CFU complete with EPO medium (Miltenyi Biotec®) during 15 days at 37°C and 5% CO2.
Statistical analysis
Shapiro-Wilk test was applied to contrast the normality of the data. Mann-Whitney U test was used for the comparison of means and Tukey test for multiple comparisons. A 95% confidence interval was defined to accept a difference as significant when p less was than 0.05 (p<0.05) (Software Graph PadPrism6).
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Results
Isolation, culture and characterization of cell populations: MSC, Ec and HSC
To collect and isolate MSC, eight BM samples were collected from voluntary donors (Table 1). According to the ISCT recommendations (28), MSCs isolated from all the samples showed the morphological characteristics, immunophenotype and differentiation capacity (osteogenesis, chondrogenesis and adipogenesis) of this cell population (Fig. 1, Table 2). Eleven UCB samples were collected to isolate CD34+HSC with a percentage of isolation greater than 80% (Table 3). The morphological and immunophenotypic characteristics of UCB-HSC and endothelial cells (Ec) are presented in Fig. 2.
 | Fig. 1MSC characteristics isolated from human BM. (A) MSC Morphology (3 passage): cells with an eccentric nucleus, loose chromatin and nucleoli; presence of granular basophilic cytoplasm (×100 Cythospin, hematoxylin and eosin stain, optical microscopy. Scale bar: 20 μm), (B) MSC Morphology (3 passage): Fibroblastoid cells associated with MSC (×20, inverted microscopy. Scale bar: 5 μm), (C, D) Immunophenotype (3 passage): MSCs do not express hematopoietic antigens (CD34 and CD45) and co-express CD73 and CD105, (E) Osteogenic differentiation (×20, red alizarin stain, inverted microscopy. Scale bar: 5 μm), (F) Adipogenic differentiation (×40, sudan black stain, inverted microscopy. Scale bar: 5 μm), (G) Chondrogenic differentiation (×20, safranin O stain, inverted microscopy. Scale bar: 5 μm).
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 | Fig. 2UCB-HSC and Ec characteristics (cell line CC-2811. Lonza®). (A) HSC Morphology: cells with a predominant nucleus, nucleoli and basophil cytoplasm (×100 Cythospin, hematoxylin and eosin stain, optical microscopy. Scale bar: 20 μm), (B) Non-adherent cells compatible with UCB-HSC (×20, inverted microscopy. Scale bar: 5 μm), (C) HSC phenotype: CD34+, (D) Ec Morphology: cells with metacentric nucleus and abundant cytoplasm (×100 Cythospin, hematoxylin and eosin stain, optical microscopy. Scale bar: 20 μm), (E) Adherent cells compatible with Ec (×20, inverted microscopy. Scale bar: 5 μm), (F) Ec phenotype: CD34+, CD31+, CD105+.
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Table 1
Bone marrow donors for MSC in vitro expansion
Table 2
Percentage of antigens evaluated in mesenchymal cells isolated from bone marrow
Table 3
Umbilical cord blood (UCB) donors for HSC isolation
Relationship between cell populations and nanoparticles to obtain OMS
To generate stable OMS, the optimal relationship between the volume of nanoparticles and the density of each of the cell populations (MSC, Ec and HSC) was defined by evaluating the morphology and DNA content in each of the structures after 5 days. Fig. 3 shows the formation of the OMS according to the different cell-to-cell densities and DNA content for experimental conditions. Fig. 3G shows the internal structure of the OMS after 5 days of cultivation, and we observed that some cells are organized in the periphery of the structure “limiting” the sphere in an orderly manner. According to the morphological characteristics and DNA content of the OMS evaluated, MSC: Ec: HSC cell ratio of 1:2:2 was selected to evaluate the efficiency of the 3D culture system by magnetic levitation to mimic the human BM microenvironment.
 | Fig. 3Organotypic multicellular spheroid (OMS) formation after 5 days: time vs. cell density. (A~C) Relation 1:5:5 MSC:Ec:HSC (×20, inverted microscopy. Scale bar: 5 mm), (D~F) Relation 1:2:2 MSC:Ec:HSC (Total cell density 1×105 cells) (×20, inverted microscopy. Scale bar: 5 mm). (G) Morphology of OMS after 5 days of culture. It shows cells that are organized in the periphery of the structure demilitarizing the sphere (Relation 1:2:2 MSC:Ec:HSC. ×40, hematoxylin & eosin. Scale bar: 5 mm). (H) DNA quantification in the spheres of the two experimental conditions (p<0.05).
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General characteristics of multicellular spheres
The OMS (MSC: Ec: HSC of 1:2:2) was evaluated after 5, 10 and 15 days with and without the exogenous addition of 100 ng/ml of Flt3L to determine the autonomy of structures in long-term HSC maintenance. Fig. 4 shows OMS without and with the exogenous addition of the cytokine. Fig. 4F shows an OMS with peripheral halo possibly associated with cells in the proliferation state (15 days). It was demonstrated that there were no significant differences in the percentage of aggregation between the spheres with and without the exogenous addition of cytokines (Fig. 4G, 82.35% vs. 71.41%), showing that in this 3D culture system, there was only a loss of 30% of the cells with which the culture was started. Similarly, no significant differences were observed in the sphericity and volume of the spheres evaluated; it is still important to indicate that during the days of cultivation, while the sphericity increases the volume decreases (Fig. 5A, B). Interestingly, we observed that after 10 and 15 days, the OMS are structures that conserve a high cellular viability (Fig. 5C–F).
 | Fig. 4Organotypic multicellular spheroid (OMS) (MSC: Ec: HSC of 1:2:2). (A~C) 3D culture without addition of exogenous cytokines (Flt3L −) (×20, inverted microscopy. Scale bar: 100 μm), (D~F) 3D culture with 100 ng/ml Flt3-L (Flt3L +) (×20, inverted microscopy. Scale bar: 100 μm). (G) Percentage of aggregation of OMS cultivated without and with Flt3L (p>0.05).
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 | Fig. 5Sphericity, volume, viability and histological evaluation of organotypic multicellular spheroid (OMS). (A) Sphericity Index, non significant differences were observed between the spheres cultivated without and with Flt3L, (B) Volumen, similarly there are no differences between the experimental conditions (p>0.05). 3D structures were treated with exogenous Flt3L (100 ng/ml) (C, D) or without cytokine (E–F). Viability was evaluated with LIVE/DEADTM Cell Imaging Kit (Invitrogen) and confocal microscope FV1000 (Olympus) using an UPLSAPO 20× (1.35 NA oil immersion objective), 488 nm argon laser line for green fluorescence (living cells) and HeNe 543 nm laser for red fluorescence (dead cells). Data analysis was performed with the FlowView and Fiji software (green cells: alive, red cells: dead) (Scale bar: 100 um). For histological evaluation, after 15 days of culture, cells without pyknotic nuclei are observed in the OMS (G) without Flt3L (×40, hematoxylin & eosin. Scale bar: 5 mm) and (H) with Flt3L (×40, hematoxylin & eosin. Scale bar: 5 mm) (I) Negative control of vimentin (brain tissue) (×40. Scale bar: 5 mm), (J) Positive control of vimentin (lymph node) (×40. Scale bar: 5 mm), (K) Vimentina in OMS without Flt3L (×40. Scale bar: 5 mm) and (L) OMS with Flt3L (×40. Scale bar: 5 mm).
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Histological evaluation of the spheres
To evaluate the internal structure of the OMS (without and with Flt3L), a morphological assessment was made after 15 days of culture. Fig. 5G, H shows the structures of the OMS with hematoxylin and eosin staining, demonstrating that in the center of the spheres, no cells with pyknotic nuclei associated with cell death were observed. In addition, it was shown that the structures obtained have an “organized morphology”. Compared to the controls, the OMS shows a strong expression of vimentin (Fig. 5K, L). The expression of Ki67 was evaluated after 10 and 15 days and a greater tendency of expression was observed in the sphere with Flt3L, although the difference was not significant (Fig. 6).
 | Fig. 6Ki67 expression. OMS were cultivated with (A) Flt3L (+) and (B) without the cytokine Flt3L (cells expressing Ki67 antigen are indicated with the arrows). Cuts of the spheres were imaged with laser scanning confocal microscope FV1000 (Olympus) using an UPLSAPO 20×, 1.35 NA oil immersion objective. A 405 nm diode laser was used for DAPI (nuclei), 488 nm argon laser line for Alexa-Fluor 488 nm (α-tubulin) and Argon 515 nm laser for alexa-fluor 514 nm (Ki67). Data analysis was performed with the FlowView and ImageJ software (green: α-tubulin, blue: DAPI, magenta: Ki67) (Scale bar: 10 μm). (C) Percentage of Ki67 expression after 10 and 15 d.
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Functional evaluation of HSC after cultivation in multicellular spheres
To establish whether the spheres obtained can mimic the microenvironment of the bone marrow, it is essential to evaluate the function of the HSC after a long period of culture within the spheres. To determine this, HSC multipotency tests were performed to evaluate the ability of these cells to generate CFU-GEMM (multipotent progenitors), CFU-GM (granulocyte-monocyte progenitors) and CFU-E (erythroid progenitors) after 10 and 15 days in culture inside the OMS and we observed that in comparison to CFU obtained from freshly purified HSC (basal) and HSC cultivated in the spheres with cytokine, the cultured HSC in the OMS without cytokine have a great capacity to generate more primitive hematopoietic colonies (CFU-GEMM) (Fig. 7).
 | Fig. 7Multipotent capacity of HSC after cultivation in OMS. (A) Dot plot representative of the recovery percentages of CD34+ cells after the disintegration of the multicellular spheres. The ability of HSC to generate (B) CFU-GM (colony forming unit - granulocyte/monocyte progenitor. ×10, inverted microscope. Scale bar: 5 mm) (C) Immature granulocytic and monocytic cells: promyelocytes, myelocytes, promonocytes and bands cells (×100, hematoxylin & eosin. Scale bar: 20 μm), (D) CFU-E (colony forming unit - erythroid progenitor. ×10, inverted microscope. Scale bar: 5 mm), (E) Immature erythroid cells: orthochromatic normoblasts are indicated (×100, hematoxylin & eosin. Scale bar: 20 μm), (F) CFU-GEMM (colony forming unit – granulocyte, erythrocyte, monocyte, megakaryocyte. ×10, inverted microscope. Scale bar: 5 mm) and (G) Immature cells of myeloid lineage: myeloblasts, promyelocytes, normoblasts, promonocytes (×100, hematoxylin & eosin. Scale bar: 20 μm) was evaluated after 10 d (H) and 15d (I) (n=1) (p>0.05).
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Discussion
From the work of Moscona and Moscona (29), during recent years, it has been demonstrated that the organotypic multicellular spheres (OMS) developed in vitro can exhibit physiological characteristics similar to tissues in vivo, such as myocardium, hepatic and vascular tissue (30, 31). The formation of OMS involves the participation of different adhesion molecules, such as E-cadherin, N-cadherin, connexins and pannexins, as well as extracellular matrix (ECM) proteins, such as type I collagen and the activation of cytoskeletal proteins as actin filaments (32, 33), which generates in the cells morphological changes that promote their aggregation and compaction with a decrease in their volume compared to the initial phase (34, 35). The OMS developed in our work have a similar behavior. We observed cellular aggregates that progressively compact in a structure with a sphericity that increases, while the volume decreases after 15 days of culture (Fig. 5A, B), which could demonstrate that in our system, there is possibly a dynamic between different adhesion molecules, ECM and structural changes in the cells.
It is important to consider that several models for the formation of OMS use cells isolated from solid tumors (for example, mammospheres), which spontaneously form spheroids in non-adherent culture conditions (36, 37), but the generation of OMS from human normal cells with a profile of adhesion molecules different from tumor cells to mimic the microenvironment of a “semi-solid” tissue, such as bone marrow, is a different challenge. The use of the magnetic levitation system allowed us to generate a sphere with adherent cellular populations, such as MSC and Ec, and non-adherent cells, such as HSC, which interact in an OMS that retains its viability for 15 days (Fig. 5C–F). Besides that the magnetic levitation system allowed us to develop a multicellular sphere from normal cell populations with different profiles of adhesion molecules, previous studies have shown that this system does not require the use of exogenous proteins or synthetic scaffolds that modify the cellular physiology but promotes the production of proteins of the extracellular matrix recreating cellular microenvironments similar to those that exist in vivo (38, 39). Since our interest was to develop a 3D culture system that mimics the conditions of the HSC microenvironment, we selected this system for the advantages described above.
In relation to the histological evaluation of the spheres, we showed that they have an organization defined by a cell population that is organized around the perimeter of the structure (Fig. 3G) and other cell populations distributed in the center of the structure that do not have pyknotic nuclei associated with a necrotic center, as described in spheres obtained with tumor cells (40); this is an important result because it indirectly demonstrates the maintenance of cell viability within the 3D structure and the non-toxicity of the nanoparticles used in the magnetic levitation system. We also evaluated the global expression of vimentin in OMS. This is a protein that is used in histological studies to demonstrate the maintenance of cell integrity because it has been shown that its decrease is related to apoptosis (41, 42); therefore, in our study we used the detection of vimentin as an indicator of the quality of the structure rather than a protein associated with mesenchymal cells where it is abundantly expressed. We observed that there is a correlation between the morphological findings observed inside the sphere (Fig. 3G) without apoptotic cells and a high expression of vimentin in the structures (Fig. 5K, L) demonstrated the formation of spheres with histological quality.
Our goal was to develop an in vitro system that would allow us to imitate the microenvironment of human HSC (vascular-stromal niche) without the exogenous use of proteins or scaffolds. It has been demonstrated that the exogenous addition only of the FLt3-L can synergize with the SCF (Stem Cell Factor) and TPO (thrombopoietin) secreted by the mesenchymal cells, stimulating the proliferation and maintenance of the HSC (27); therefore, to evaluate whether the obtained OMS can autonomously maintain the CD34+ cells or require the addition of exogenous hematopoietic cytokines, we use the Flt3L cytokine. Additionally, we evaluated the effect of Flt3L on the formation of the structure (percentage of aggregation), viability and expression of Ki67.
We did not observe differences in the percentage of aggregation (Fig. 4G) and viability (Fig. 5C–F) between the OMS cultivated with Flt3L and without the cytokine. We observed a greater tendency in the expression of Ki67 in the sphere with Flt3L (Fig. 6C) although the difference was not significant. After isolating the cultured HSC from OMS (10 and 15 days), we could determine that our structures maintain viable and multipotent HSC without the exogenous addition of cytokine. The multipotency test showed that from HSC cultivated in the OMS with Flt3-L, a greater number of committed progenitors colonies (CFU-GM and CFU-E) is obtained, while cultivating HSC in the cytokine-free makes them capable of generating a greater number of myeloid progenitors (CFU-GEMM) (Fig. 7). This shows that the OMS cultivated without the addition of exogenous cytokines is autonomous in the maintenance of HSC and that the survival and functionality of these cells depend only on their interaction with MSC and Ec and the soluble factors secreted by these cells as they occur in vivo. This is particularly interesting in HSCs isolated from umbilical cord blood because this source has a very low number of HSCs compared to BM or peripheral blood mobilized (25), and although no significant increase in the number of HSCs is observed through the OMS, an important increase in the number of myeloid progenitors after culture was observed (Fig. 7, basal vs. Flt3L−), which could contribute to the efficiency in the repopulation capacity of this cellular population in adult recipient patients despite the number of available cells.
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Conclusions
In summary, our results demonstrate the development of an OMS from normal human cells as a model for the study of the microenvironment of human HSC. This type of development will allow for the generation of more complex spheroids that imitate the microenvironment of human stem cells and the proposal of new protocols in regenerative medicine.
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