Authors: Tiago O. Ribeiro aff001; Brysa M. Silveira aff001; Mercia C. Meira aff001; Ana C. O. Carreira aff002; Mari Cleide Sogayar aff002; Roberto Meyer aff001; Vitor Fortuna aff001 Authors place of work: Health Science Institute, Federal University of Bahia, Salvador, BA, Brazil aff001; Cell and Molecular Therapy Center NUCEL-NETCEM, School of Medicine, Internal Medicine Department, University of São Paulo, São Paulo, SP, Brazil aff002; Chemistry Institute, Biochemistry Department, University of São Paulo, São Paulo, SP, Brazil aff003 Published in the journal: PLoS ONE 14(10) Category: Research Article doi: https://doi.org/10.1371/journal.pone.0222093
Sickle cell disease (SCD) is a monogenic red cell disorder associated with multiple vascular complications, microvessel injury and wound-healing deficiency. Although stem cell transplantation with bone marrow-derived mesenchymal stem cells (BMSC) can promote wound healing and tissue repair in SCD patients, therapeutic efficacy is largely dependent on the paracrine activity of the implanted BM stromal cells. Since in vitro expansion and culture conditions are known to modulate the innate characteristics of BMSCs, the present study investigated the effects of normoxic and hypoxic cell-culture preconditioning on the BMSC secretome, in addition to the expression of paracrine molecules that induce angiogenesis and skin regeneration. BMSCs derived from SCD patients were submitted to culturing under normoxic (norCM) and hypoxic (hypoCM) conditions. We found that hypoxically conditioned cells presented increased expression and secretion of several well-characterized trophic growth factors (VEGF, IL8, MCP-1, ANG) directly linked to angiogenesis and tissue repair. The hypoCM secretome presented stronger angiogenic potential than norCM, both in vitro and in vivo, as evidenced by HUVEC proliferation, survival, migration, sprouting formation and in vivo angiogenesis. After local application in a murine wound-healing model, HypoCM showed significantly improved wound closure, as well as enhanced neovascularization in comparison to untreated controls. In sum, the secretome of hypoxia-preconditioned BMSC has increased expression of trophic factors involved in angiogenesis and skin regeneration. Considering that these preconditioned media are easily obtainable, this strategy represents an alternative to stem cell transplantation and could form the basis of novel therapies for vascular regeneration and wound healing in individuals with sickle cell disease.
Tissue repair – Hypoxia – Endothelial cells – Wound healing – Medical hypoxia – Angiogenesis – Neurobiology of disease and regeneration – Sickle cell disease
Sickle cell disease (SCD), the most common inherited hemoglobinopathy worldwide, is characterized by repeated vaso-occlusion crises secondary to sickled red blood cells [1]. It is associated with significant microvessel injury, as well as impairments in neovascularization, wound healing and tissue repair [2,3]. SCD patients are at high risk of a wide range of complex and multifactorial vasculopathic complications, including pulmonary hypertension, retinopathy, priapism, osteonecrosis and leg ulcers [4,5]. Consequently, these complications often cause significant functional, emotional, and economic burdens for the afflicted patients and result in considerable cost to the healthcare system [6, 7].
The transplantation of bone marrow-derived mesenchymal stem cells (BMSC) has been extensively investigated as source of promising proangiogenic stem cell therapy for diseases with vascular complications, such as peripheral artery disease, acute kidney injury, myocardial infarction and skin ulcers [8]. A growing number of studies have reported that BMSC secrete a wide range of bioactive factors that enhance in vitro the proliferation and migration of endothelial cells [9, 10] and promote tissue healing and formation of new blood vessels [11]. Recently, Kim and colleagues identified important bioactive factors in the BMSC secretome that correlate with vascular regenerative efficacy in the treatment of ischemic disease [10]. These biofactors were then validated and can now be used as efficient biomarkers to predict response to proangiogenic MSC-based cell therapies. Furthermore, significant variation in the MSC secretome and the functional capacity of its biomarkers has been observed among differing donor sources and diseases. However, in SCD, the key factors secreted by BMSCs that possess the potential to promote angiogenesis and tissue repair have not been identified to date.
As cell therapy efficacy is dependent on the number of implanted BMSCs, culture expansion can overcome this limitation to improve the treatment of diseases with vascular complications [12]. However, in vitro expansion and culture conditions modulate the innate characteristics of BMSCs and hinder the clinical applications of BMSCs [13, 14]. To optimize the culturing conditions of stem cells, various in vitro pretreatment strategies (“preconditioning”) have recently been evaluated to enhance the regenerative capacity of BMSCs, including cell culture expansion in an hypoxic (Hyp) environment [15]. Preconditioning by hypoxia increases the secretion of regenerative factors and enhances stem cell survival [16, 17]. The paracrine factors secreted by cells can accumulate in the conditioned medium (CM). The conditioned medium derived from the BMSC culture has been reported to serve multiple positive functions in tissue regeneration [11, 12, 16, 18]. Furthermore, findings by Elabd and colleagues suggest that hypoxic preincubation positively impacted the BMSC secretome and transcriptome, improving the vasculogenic and angiogenic properties critical for the development of successful cellular therapies [19]. Although numerous studies using BMSCs and their conditioned mediums as potential therapeutic agents have been published [18, 20–22], how hypoxic preincubation affects the BMSC secretion of bioactive factors with vascular regenerative potential remains poorly understood.
Here, we attempted to investigate the potential of BMSCs from SCD patients as an innovative source for proangiogenic therapies. We first evaluated the effects of hypoxic preconditioning on the ability of these BMSCs to secrete bioactive angiogenic factors in culture medium (CM). We then used this hypoxic preconditioned CM for subsequent in vitro and in vivo studies in a mouse model of angiogenesis and wound healing. In summary, preconditioning by hypoxia was shown to enhance the secretion of trophic paracrine factors involved in angiogenesis and tissue regeneration. Therefore, hypoxic BMSCs secretome represent a promising alternative for stem cell transplantation and can provide a novel proangiogenic and tissue regeneration option for sickle cell disease patients.
Human umbilical vein endothelial cells (HUVEC) were isolated as described previously [23]. The institutional review board of the Climério de Oliveira Maternity Hospital (Federal University of Bahia, approval no 625.059) approved the human umbilical cord sampling and bone marrow aspiration procedures after obtaining written informed patient consent. Briefly, the umbilical vein was cannulated with a 20G needle and perfused with 0.05% collagenase I at 37° C for 15 min. HUVECs were then collected with PBS, centrifuged at 200 g for 10 min and resuspended in EGM2/ BulletKit medium (Lonza Group Ltd.). HUVECs were cultured on 0.1% gelatin (Sigma, St. Louis, MO) in EGM2/BulletKit supplemented with 100 U/mL penicillin/streptomycin (Life Technologies) at 37°C in 5% CO2 and 95% air. The medium was replaced every 2–3 days and cells were subcultured when confluent. The HUVECs were then maintained in EGM2 and used for experiments for a maximum of five passages.
BM was aspirated from the posterior iliac crest of nine patients with SCD. BMSC were cultured as previously described [24]. Briefly, BM aspirates were diluted with PBS, layered onto a Ficoll density gradient and centrifuged at 400 g for 20 minutes. Mononuclear cells were plated in complete Dulbecco’s modified Eagle’s complete medium (low glucose, 10% fetal calf serum, 100 U/mL penicillin/streptomycin) at 100,000 to 300,000 cell/cm2. After four days of culturing, the medium was replaced and BMSCs were allowed to expand for 7–12 days. BMSCs were passaged weekly, and passages 3–6 were used in experimentation.
BMSCs were harvested after the third passage and cell surface antigen expression was analyzed using a fluorescence-activated cell sorter (FACScalibur, BD Biosciences). The following monoclonal antibodies were used: CD29-FITC (clone TS2/16), CD90-FITC (clone eBIO5E10), CD105-PE (clone SN6), CD14-PE (clone 61D3) (all from eBioscience, San Diego, CA, USA), CD31-FITC (clone WM59), CD34-FITC (clone 8G12) (both from BD Biosciences, San Jose, CA, USA) and CD73-PE (clone AD2, EXBio Praha). All samples were run using the appropriate isotype control antibody in accordance with the manufacturer’s protocol.
BMSCs were expanded to subconfluency in standard culture medium at 37°C under 5% CO2 and humidity (standard conditions). To generate normoxic (nor) or hypoxic (hypo) conditions, confluent cells in 6-well plates (average of 20,000 cells/cm2) were washed twice and cultured for 48h with 3ml/well of serum-free EBM-2 medium. For hypoxic preconditioning, BMSC were placed in an Anaerobac Jar (Probac, São Paulo, Brazil) at 0.5% oxygen, as described [17, 25]. After 48hs, the procedures for conditioned medium collection and storage were performed as previously described [26]. Briefly, the cell-cultured supernatant was aspirated, pooled, centrifuged at 2000g for 20 min at 4o C, and stored at -70o C. This total BMSC secretome hereafter is referred to as ‘‘BMSC secretome”. Total protein was determined by the Lowry method before use.
Human angiogenesis antibody arrays were purchased from R&D Systems (cat. no ARY007) and used according to the manufacturer’s instructions. Briefly, protein contents in the CM were determined by Lowry assay and equal amounts of protein were used for each condition. After overnight incubation, retained protein signals were revealed by an enhanced luminol-based detection reaction and quantified by densitometry using ImageJ (NIH, USA) software.
After normoxic or hypoxic conditions, BMSC monolayers were briefly rinsed with ice-cold PBS and total RNA was extracted using a commercial kit (RNeasy Qiagen) according to the manufacturer’s instructions. All RNA samples were checked for purity using Thermo Scientific NanoDrop spectrophotometer. 1 μg RNA was taken for cDNA synthesis with the Omniscript RT-PCR kit from Qiagen as recommended by the manufacturer. Relative mRNA expression of the target genes was detected using Maxima SYBR Green/ROX qPCR Master Mix (Thermo Scientific) (final volume: 12 μL) in a GeneAmp 7300 Sequence Detection System (Applied Biosystems) in accordance with the manufacturer’s instructions. All primer sequences are listed in a S1 Table. Differential mRNA expression levels were considered when relative expression (R.E.) was ≥2.0 and ≤0.5 and statistical significance was determined if P < 0.05 (Wilcoxon’s test). Relative mRNA expression levels were estimated using the method described by [27], which generates normalized values in geNorm Software using RN18S1, GAPDH and HPRT for housekeeping.
HUVECs were seeded (2.0 x 104 cells/well) on 0.1% gelatin-coated 24-well plates and serum starved for 4 hours in EBM-2 medium, followed by stimulation with norCM, hypoCM or a vehicle control for 24 hours. Cultured HUVECs were incubated with 10 μM BrdU (5-bromo-2′-deoxy-uridine) for 4 h before fixation. BrdU detection and incorporation were performed with a cell proliferation kit (Thermo Fisher Scientific).
Fluorescent terminal deoxynucleotidyl transferase deoxyuridine triphosphate (dUTP) nick end labeling (TUNEL) was performed using an in situ cell death detection kit (Roche) in accordance with the manufacturer protocol. Cell death in HUVEC was induced with serum starvation for 4 h. Only apoptotic cells were stained by TUNEL, while DAPI labeled the nuclei of all cells. The number of HUVECs that underwent apoptosis was determined by counting TUNEL/DAPI double‐stained cells in five different fields under a fluorescence microscope.
A 3-dimensional in vitro model of angiogenesis was utilized, as previously described [28, 29]. Briefly, collagen-cytodex microcarrier beads (Sigma-Aldrich Co) were coated with HUVECs (#3) and embedded in fibrin gel. After the gels were allowed to clot on 24-well plates, vehicle control, nor - or hypo-BMSC-derived conditioned medium (500 μL) was added to each well and replaced every two days. The number of endothelial sprouts/beads, branches and tubule length was quantified in at least 30 beads per condition after four days. Only sprouts larger than the bead diameter were considered.
All procedures were approved by the institutional review board for animal experimentation (CEUA-2018-131). In vivo angiogenesis experiments were performed as previously described [30]. Briefly, a mixture of basement membrane matrix (Geltrex reduced growth factor, Gibco) and conditioned medium (9 : 1 proportion) was prepared in the 20-mm sterile surgical silicone tubes (angioreactors) from a DIVAA kit (R&D system). A mixture containing basement membrane matrix and buffered saline was included as a control during the assay. After a 1-hour incubation period at 37o C, the angioreactors were subcutaneously implanted into the dorsal flanks of 8-week-old female C57/BL6 mice. Up to 2 angioreactors were implanted on each side for a total of 4 angioreactors per mouse (n = 4 animals per group, for each independent experiment). After 11 days, the animals were euthanized and the angioreactors were removed. For quantitation of functional vessels formed, the contents were removed from angioreactors and homogenized in distilled water. The relative hemoglobin content was measured at 540 nm according to [10]. Differences between the conditions were compared using the Student’s t-test.
HUVEC monolayers cultured on 24-well plates were scratched with a pipette tip to create a straight gap. After debris removal via extensive washing, cells were allowed to migrate in the presence of norCM, hypoCM or a vehicle control medium for 24 hours. In order to evaluate the same field during image acquisition using a phase-contrast microscope, reference points were marked close to the scratches. The plates were kept in an incubator at 37°C and examined periodically (0, 6, 12 and 24 h). The open wound area visible in each image was quantitatively measured at each time point using ImageJ program software.
HUVECs were washed with PBS and lysed in sodium dodecyl sulfate (SDS) buffer containing Complete Mini Proteinase Inhibitor Cocktail Tablets (Sigma, St. Louis, MO, USA). Protein concentration was determined by Lowry protein assay (Sigma, St. Louis, MO, USA). The protein lysates (30 μg) were loaded onto 12% polyacrylamide SDS gel and and then, the separated proteins were transferred to polyvinylidene difluoride (PVDF) membranes, blocked, and incubated overnight at 4°C with primary antibodies against β-Actin, AKT and phospho-AKT (Ser473) (Cell Signaling Technology). The membranes were washed and then incubated with a secondary antibody for 1 hour at room temperature using an orbital shaker. After washing, the bands were detected using an enhanced chemiluminescence reagent (Western Chemiluminescent HRP Subtract, Merck Millipore).
Eight-week-old female C57/BL6 mice were anesthetized and, after shaving the dorsum, two punctures, one on each side of the midline, were made along the dorsal flank with 4-mm disposable punch biopsy instruments. Full-thickness excisional wounds extending through the panniculus carnosus were created and the wounded areas were left uncovered. The animals were randomly divided into three groups (4 in every group), depending on the type of medium (BMSC norCM, hypoCM or vehicle control) injected into the injury site. A total of 100 uL of conditioned medium (3.0–3.3 mg/mL) was injected into four diametrically opposed points around the puncture site at 0 and 2 days after procedures. Control mice were similarly treated with PBS. The puncture sites were subsequently photographed at selected time points using a Nikon Coolpix B700 digital camera. Wound surface size was estimated at each time point, expressed as the percentage of original wound size (day 0). After wound closure, mice were euthanized and the wound areas, along with surrounding tissue, were harvested and processed for immunohistochemical (IHC) or immunofluorescence (IF) analysis.
BMSCs (2.0 x 104 cell/well) cultured on 13-mm diameter glass coverslips were fixed in 4% paraformaldehyde (PFA) for 15 min at room temperature. Cells were incubated overnight at 4o C with the following primary antibodies diluted in 10% normal goat serum: goat anti-PDGFR (1 : 50, R&D System), rabbit anti-NG2 (1 : 200, Millipore) and rabbit anti-Collagen IV (1 : 200, Abcam). After washing with PBS, samples were incubated with the secondary antibodies (Alexa Fluor-555 anti-goat; Alexa Fluor-488 anti-rabbit, Invitrogen) for 30 min at room temperature.
The skin wound specimens were fixed in 4% PFA for 12 hours at 4o C and then prepared for histological processing according to [31]. Briefly, tissue samples were incubated in 30% sucrose for 24 hours, embedded in OCT, snap-frozen and cryosectioned (50-μm-thick sections). All frozen sections were washed in PBS (pH 7.4) three times, and then blocked using 5% calf serum in PBS to eliminate nonspecific protein binding. The primary antibody (goat anti-CD31; R&D system) was diluted and incubated overnight at 4o C. After removing any unbound antibodies by washing, the secondary antibody (Alexa Fluor-488 donkey anti-goat; Invitrogen) was added at a concentration of 1 : 300, and samples were then incubated for 30 min at room temperature. Any unbound antibodies were again removed with PBS. Slides were prepared using mounting medium (Dako) on glass coverslips for fluorescence microscopy analysis (Leika SP8). For histochemical staining, tissue samples were embedded in paraffin, sectioned (5 μm thickness) and stained with hematoxylin and eosin (H&E) in accordance with standard protocols.
Values are expressed as mean +/ - standard deviation for at least three independent experiments. The statistical analysis was performed using the Student’s t-test or a one way analysis of variance (ANOVA) test with the GraphPad Prism software (Version 6.0). A P value of less than 0.05 was considered statistically significant.
All experiments were conducted using BMSCs from nine different donors, which were characterized for surface markers and differentiation multipotential, as previously described [24]. Freshly isolated BMSCs from SCD patients showed classic MSC characteristics and displayed spindle-shaped fibroblastic-like morphology when adhered to plastic at P0. Once MSC reached confluence, these were maintained for 48hs in normoxic or hypoxic conditions. Although total cell number increased, no differences were observed between the normoxic and hypoxic cultured cells (Fig 1A). Live-dead staining showed no changes in viability following normoxic or hypoxic preconditioning (Fig 1B).
The expression of characteristic BMSC markers was performed by flow cytometry and immunostaining after normoxic and hypoxic preconditioning. As shown in Fig 2, BMSCs were highly positive for surface markers typical of MSCs, such as CD90, CD105, CD73 and CD29, and were negative for hematopoietic or endothelial markers, such as CD34, CD45 and CD31. Surface marker expression in BMSC cultures after normoxic or hypoxic culturing is shown on S2 Table. Representative markers, such as collagen IV, NG2 and PDGFR-beta, were also detected in the BMSCs (Fig 2B). No significant differences in the expression of any of these markers were observed between the normoxically or hypoxically cultured BMSCs (Fig 2). In sum, hypoxic preconditioning for 48h did not result in any detectable changes with respect to the surface and intracellular markers evaluated.
In order to compare the proangiogenic factor profiles of normoxically and hypoxically cultured BMSCs from SCD patients, the secretome contents were estimated using a human proteome profiler array. Experiments were performed on normoxic (nor) or hypoxic (hypo) conditioned medium (CM) generated after 48 h of serum deprivation, since FBS contains high levels of growth factors. Under normoxic conditions, we observed that classic trophic molecules, such as VEGF-A, MCP-1, IL8, IGFBP-2/3, PTX3 and THBS1, were secreted at relatively high concentrations (Fig 3A). However, the hypoxic secretome was rich in molecules related to angiogenesis and tissue repair processes when compared to the normoxic BMSC secretome (Fig 3B).
Direct analysis of BMSC-CM contents showed that, of all the 55 trophic factors examined, 21 secreted growth factors/cytokines were consistently more abundant in hypoCM than in norCM. The hypoCM molecules with no less than three times higher expression than norCM were grouped into distinct categories: pro-angiogenic factors (angiogenin, angiopoietin-1/2, EG-VEGF, endothelin-1, endostatin, FGF-b, TGF-b1, PIGF and prolactin), tissue repair-related factors (HGF and TIMP-4) and anti-angiogenic factors (platelet factor 4, IGFBP-1 and serpin F1).
The relative expression of transcripts between the normoxic and hypoxic preconditioned BMSCs was evaluated by real time PCR. Of all the 11 genes examined, the transcriptional levels of six genes showed more than a three-fold difference between normoxic (upregulation of THBS) and hypoxic (upregulation of Col-4, FGF-1, HGF, SDF-1a, Il-8) (Fig 3C) conditions. These data indicate that hypoxic preconditioning modulated and enhanced the expression of trophic factors in the secretome of BMSCs from SCD patients.
HUVEC tube formation and migration induced by norCM or hypoCM were assessed to determine the ability of the secretome of BMSCs from SCD patients to support in vitro angiogenesis. In this assay, HUVECs seeded on collagen-coated cytodex beads were embedded in a 3-dimensional fibrin matrix. NorCM or hypoCM were added on top of gel. Fig 4A demonstrates that numbers of sprouts/beads (3.7 ± 1.5 vs. 1.9 ± 0.8 sprout/bead, p<0.01) and sprout lengths (189 ± 120.6 vs. 122.3 ± 88 μm, p<0.05) were significantly increased in the presence of hypoCM as compared to norCM. By contrast, minimal sprouting was observed in the vehicle control medium (Fig 4A). Furthermore, the migration of HUVECs, measured by a monolayer wound assay, was significantly greater in the presence of hypoCM (Fig 4B). HypoCM and norCM conditions significantly facilitated monolayer wound closure in comparison to the vehicle control medium (96.0 ± 7.4, 74.7 ± 11.1 vs 16.3 ± 3.1, p<0.01). These data indicate that hypoxic preconditioning was highly correlated with in vitro EC migration and proangiogenic activities in BMSCs from SCD patients.
The effects on angiogenesis of HypoCM and norCM were also examined using an in vivo assay in C57Bl6 mice. The induction of new blood vessel formation was not evident in the angioreactor containing PBS alone. By contrast, the inclusion of either CM significantly induced the development of new blood vessels. HypoCM was shown to induce greater angiogenesis than norCM, which had less pronounced effect (Fig 4C). These results clearly indicate that hypoxic preconditioning results in in vivo pro-angiogenic activity.
To examine the effects of normoxic and hypoxic BMSC secretomes on endothelial cell proliferation, HUVECs were serum-starved for four hours, then stimulated with CM or vehicle control medium for 24 hours. BrdU incorporation in HUVECs was consistently higher in the presence of hypoCM compared to norCM (p< 0.05) (Fig 5A). In addition, following serum starvation, hypoCM significantly reduced the number of HUVECs undergoing apoptosis (Fig 5B). Furthermore, phosphorylation of the pro-survival kinase AKT was enhanced under hypoCM (p < 0.05), indicating that culturing hypoxic conditions activate survival mechanisms in HUVECs.
The therapeutic efficacy of hypoCM and norCM was evaluated in a murine excisional wound healing model. Both hypoCM and norCM significantly accelerated wound healing in comparison to controls (Fig 6A). At day 7, a smaller wound area was observed in mice injected with either hypoCM or norCM compared with the vehicle control group. Immunofluorescence analysis showed similar increases in CD31+ (endothelial cell density) and a-SMA (smooth muscle cells) expression in the norCM and hypoCM wounds as compared to controls (Fig 6B). Taken together, these results indicate that norCM and hypoCM wound treatment increased the vascularization of newly formed tissue, an essential component of the wound healing process.
BMSCs are considered to hold strong potential for the development of cell-based therapies designed to enhance angiogenesis during the wound-healing process, and also have beneficial effects on skin regeneration. However, the dysfunction of BMSCs in different bone marrow disorders and pathological conditions has narrowed treatment possibilities [32–34], making the evaluation of these cells’ biological functioning crucial prior to therapeutic applications in sickle cell disease patients. The present study provides evidence that the secretome of BMSCs from SCD patients demonstrates pro-angiogenic properties and promotes wound healing. Conditioned media from hypoxic BMSC cultures promoted greater increases in both the proliferation and migration of HUVECs in comparison to cells cultured normoxically or with vehicle control medium. In addition, the introduction of preconditioned medium into skin wounds resulted in a significant improvement in wound closure and the formation of a mature vascular network, confirming that hypoxically preconditioned BMSC media from SCD patients presents considerable proangiogenic and reparative potential.
Hypoxic preconditioning (i.e., short-term exposure to hypoxia) represents a promising strategy for increasing cellular survival in and the self-renewing capacity of human BMSCs, as well as improving the immunomodulatory and regenerative potential of these cells. However, the effects on BMSCs produced by hypoxic preconditioning are highly dependent on the culture conditions, cell source and composition of growth medium [15, 35, 36]. Some studies reported that short-term hypoxia preconditioning significantly increased cell viability and induced stem cell properties [17], while others have reported either negative or no effects on BMSCs [37–39]. While hypoxia induces cell cycle arrest in mammalian cells, mesenchymal stem cells are highly resistant to stress conditions [40]. The present study demonstrated that although short-term hypoxic preconditioning had no effect on cell expansion efficacy or viability, the expression and secretion of trophic factors was found to be upregulated in comparison to normoxic culture conditions. Nonetheless, BMSCs subjected to short-term hypoxia exhibited similar cellular marker expression as those cultured under normoxic conditions. These results indicate that the short-term hypoxic preconditioning employed herein did not deleteriously affect cell viability and was capable of inducing a secretory phenotype.
Recent studies have demonstrated the brief survival of BMSCs following implantation, and that the benefits of BMSC therapy could arise from the vast variety of factors secreted by these cells [41–43]. The cell secretome is a collective term defined as the set of secreted trophic factors/soluble molecules (proteins, free nucleic acids, lipids) and extracellular vesicles (exosomes, microvesicles, membrane particles). To date, it has been shown that both of these components may be capable of independently trigger angiogenesis, tissue regeneration and repair [44–46]. Discrimination of which of these components is more effective in producing therapeutic effects is still matter of debate [40, 41, 43]. Here, we were particularly interested in the effects of the whole cell secretome, without fractionation of its sub-component. Preparation of the whole cell-secretome is more economical, more practical, and less time-consuming for clinical application [42]. Recent reports have also described that processing methods to separate soluble components from the microvesicles are labor-intensive, may influence paracrine factor concentration and add several disadvantages that complicate further analysis [47, 48].
The present report found alterations in the secreted factors present in culture medium after hypoxic preconditioning, which may account for the enhanced wound healing and microvascular recovery observed herein. Therefore, we compared the compositions of the secretomes produced in response to normoxic and hypoxic preconditioning using a proteome antibody array. Our results indicated that hypoxic preconditioning led to the increased expression of 17 trophic factors, including four important biomarkers previously implicated in vascular regeneration: angiogenin, interleukin-8, monocyte chemoattractant protein-1 and vascular endothelial growth factor [10]. Some studies have additionally shown that the trophic factors HGF, IGF-1, ang1/2 and bFGF, in addition to promoting angiogenesis, also present anti-inflammatory and neurogenic properties that may either directly or indirectly enhance healing after microvascular or skin injury [42, 49, 50]. In addition, Kim and colleagues described that hypoxia-preconditioning induced BMSCs to express higher levels of HIF-1α and growth factors GDNF, BDNF, VEGF, Ang-1 and SDF-1, as well as its receptor CXCR4, all of which have been linked to neovascularization [51]. These authors additionally found increased expression of EPO and its receptor EPOR, a neuroprotective and pro-angiogenic molecule [51].
The proteome antibody array technique employed herein is limited by the number of specific proteins that can be detected using this approach. Using LC-MS/MS for a more systematic analysis of the human BMSC secretome, Jiang and colleagues identified a diverse range of secretory products associated with microvascular recovery as a result of hypoxic preconditioning [11]. Moreover, an extensive proteomic analysis of the secretome derived from hypoxia-conditioned BMSCs showed that many bioactive factors induced angiogenesis in endothelial cells via the activation of the NFκB pathway [44], while another study implicated the Wnt signaling pathway in the attenuation of vessel injury [45]. While hypoxia seems to be linked to increased secretion of trophic factors in general [52], further research must be carried out to better understand the contributions made by these pathways in the context of SCD. In addition, many potential molecular mechanisms underlying hypoxic CM-mediated functional recovery, which may act as treatment targets in future clinical applications, require additional investigation.
The formation of new blood vessels is a critical step in normal wound healing. Delayed wound healing and chronic wound formation is observed in conditions associated with impaired angiogenesis, such as diabetes and sickle cell disease [2]. The present study demonstrated that the secretome of BMSCs from SCD patients regulates endothelial cell migration, proliferation and survival. These findings were associated with the activation of the PI3k-AKT pathway and the expression of phosphorylated AKT in HUVECs. These data are consistent with previous reports which showed that the conditioned medium derived from hypoxic BMSCs significantly increased endothelial cell proliferation and migration, thereby promoting early events of angiogenesis [17; 35]. In addition, some authors have described, in vivo, the recruitment of fibroblasts and keratinocytes after wound treatment with a hypoxic BMSC secretome [53]. The PI3k-AKT pathway, a classical regulator of cell cycle and survival, has been implicated in ischemic conditions [11]. Moreover, activation of the AKT signaling pathway in endothelial-progenitor cells has been linked to wound healing and microvascular regeneration [54]. These findings suggest that the injection of BMSC secretomes from SCD patients could positively affect the local microenvironment, thusly facilitating the proliferation, recruitment and migration of resident endothelial cells in response to chemoattractants, which may reinforce skin regeneration and repair in conditions associated with impaired angiogenesis, e.g. sickle cell disease.
The therapeutic benefits of the BMSC secretome have been well demonstrated in numerous experimental, pre-clinical and clinical models [41, 42]. Secretome-based approaches may present considerable therapeutic advantages over living cells in terms of facilitating manufacturing, storage, biocompatibility, non-immunogenicity, and non-tumorigenicity. Moreover, secretomes are more physiologically stable than cells, and constitute an efficient biological therapeutic agent. Since the secretome profile varies significantly among BMSC populations derived from different donors and anatomical locations [10, 19, 55], it is important that an appropriate secretome signature be chosen in accordance with a specific therapeutic end point. In this context, additional studies focusing on optimal protein concentrations, administration frequency and optimum injection volume could contribute to the therapeutic success of the BMSC secretome in promoting vascular regeneration and wound healing in individuals with sickle cell disease.
In conclusion, BMSCs subjected to hypoxic preconditioning demonstrated an increased ability to secrete bioactive trophic factors in culture medium, thereby providing paracrine effects to endothelial cells. This finding indicates that the hypoxic secretome of BMSCs from SCD patients presents promising potential to develop regenerative medicine strategies to enhance tissue repair after skin injury.
S1 Table [pdf] List of primer sequences used for RT-PCR.
S2 Table [pdf] Flow cytometry analysis of BMSC cultures isolated from SCD patients.
S3 Table [pdf] Raw data (Hematological characteristics of SCD patients).
1. Kato GJ. Sickle cell vasculopathy: Vascular phenotype on fire!. J Physiol. 2019 Feb; 597(4):993–994. doi: 10.1113/JP276705 30007009
2. Nguyen VT, Nassar D, Batteux F, Raymond K, Tharaux PL, Aractingi S. Delayed Healing of Sickle Cell Ulcers Is due to Impaired Angiogenesis and CXCL12 Secretion in Skin Wounds. J Invest Dermatol. 2016 Feb. 136(2):497–506. doi: 10.1016/j.jid.2015.11.005 26967481
3. Okwan-Duodu D, Hansen L, Joseph G, Lyle AN, Weiss D, Archer DR, et al. Impaired Collateral Vessel Formation in Sickle Cell Disease. Arterioscler Thromb Vasc Biol. 2018 May;38(5):1125–1133. doi: 10.1161/ATVBAHA.118.310771 29545241
4. Minniti CP, Delaney KM, Gorbach AM, Xu D, Lee CC, Malik N, et al. Vasculopathy, inflammation, and blood flow in leg ulcers of patients with sickle cell anemia. Am J Hematol. 2014 Jan;89(1):1–6. doi: 10.1002/ajh.23571 23963836
5. Potoka KP, Gladwin MT. Vasculopathy and pulmonary hypertension in sickle cell disease. Am J Physiol Lung Cell Mol Physiol. 2015 Feb 15;308(4):L314–24. doi: 10.1152/ajplung.00252.2014 25398989
6. Azar S, Wong TE. Sickle cell disease: a brief update. Med Clin North Am. 2017 Mar;101(2):375–393. doi: 10.1016/j.mcna.2016.09.009 28189177
7. Bou-Maroun LM, Meta F, Hanba CJ, Campbell AD, Yanik GA. An analysis of inpatient pediatric sickle cell disease: Incidence, costs, and outcomes. Pediatr Blood Cancer. 2018 Jan;65(1). doi: 10.1002/pbc.26758 28801954
8. Bronckaers A, Hilkens P, Martens W, Gervois P, Ratajczak J, Struys T, et al. Mesenchymal stem cells and vascular regeneration. Pharmacol Ther. 2014 Aug; 143(2):181–96. doi: 10.1016/j.pharmthera.2014.02.013 24594234
9. Gu W, Hong X, Potter C, Qu A, Xu Q. Mesenchymal stem/stromal cells as a pharmacological and therapeutic approach to accelerate angiogenesis. Microcirculation. 2017 Jan;24(1). doi: 10.1111/micc.12324 27681821
10. Kim HK, Lee SG, Lee SW, Oh BJ, Kim JH, Kim JA, et al. A Subset of Paracrine Factors as Efficient Biomarkers for Predicting Vascular Regenerative Efficacy of Mesenchymal Stromal/Stem Cells. Stem Cells. 2019 Jan;37(1):77–88. doi: 10.1002/stem.2920 30281870
11. Jiang RH, Wu CJ, Xu XQ, Lu SS, Zu QQ, Zhao LB, et al. Hypoxic conditioned medium derived from bone marrow mesenchymal stromal cells protects against ischemic stroke in rats. J Cell Physiol. 2019 Feb;234(2):1354–1368. doi: 10.1002/jcp.26931 30076722
12. Hoch AI, Leach JK. Concise review: optimizing expansion of bone marrow mesenchymal stem/stromal cells for clinical applications. Stem Cells Transl Med. 2014 May;3(5):643–52. doi: 10.5966/sctm.2013-0196 24682286
13. Zhu W, Chen J, Cong X, Hu S, Chen X. Hypoxia and serum deprivation-induced apoptosis in mesenchymal stem cells. Stem Cells. 2006 Feb;24(2):416–25. doi: 10.1634/stemcells.2005-0121 16253984
14. Dionigi B, Ahmed A, Pennington EC, Zurakowski D, Fauza DO. A comparative analysis of human mesenchymal stem cell response to hypoxia in vitro. J Pediatr Surg. 2014 Jun;49(6):915–8. doi: 10.1016/j.jpedsurg.2014.01.023 24888834
15. Buravkova LB, Andreeva ER, Gogvadze V, Zhivotovsky B. Mesenchymal stem cells and hypoxia: where are we? Mitochondrion. 2014 Nov;19 Pt A:105–12. doi: 10.1016/j.mito.2014.07.005 25034305
16. Bader AM, Klose K, Bieback K, Korinth D, Schneider M, Seifert M, et al. Hypoxic Preconditioning Increases Survival and Pro-Angiogenic Capacity of Human Cord Blood Mesenchymal Stromal Cells In Vitro. PLoS One. 2015 Sep 18;10(9):e0138477. doi: 10.1371/journal.pone.0138477 26380983
17. Antebi B, Rodriguez LA 2nd, Walker KP 3rd, Asher AM, Kamucheka RM, Alvarado L, et al. Short-term physiological hypoxia potentiates the therapeutic function of mesenchymal stem cells. Stem Cell Res Ther. 2018 Oct 11;9(1):265. doi: 10.1186/s13287-018-1007-x 30305185
18. Ferreira JR, Teixeira GQ, Santos SG, Barbosa MA, Almeida-Porada G, Gonçalves RM. Mesenchymal Stromal Cell Secretome: Influencing Therapeutic Potential by Cellular Pre-conditioning. Front Immunol. 2018 Dec 4;9 : 2837. doi: 10.3389/fimmu.2018.02837 eCollection 2018. 30564236
19. Elabd C, Ichim TE, Miller K, Anneling A, Grinstein V, Vargas V, et al. Comparing atmospheric and hypoxic cultured mesenchymal stem cell transcriptome: implication for stem cell therapies targeting intervertebral discs. J Transl Med. 2018 Aug 10;16(1):222. doi: 10.1186/s12967-018-1601-9 30097061
20. Konala VB, Mamidi MK, Bhonde R, Das AK, Pochampally R, Pal R. The current landscape of the mesenchymal stromal cell secretome: A new paradigm for cell-free regeneration. Cytotherapy. 2016 Jan;18(1):13–24. doi: 10.1016/j.jcyt.2015.10.008 26631828
21. Kusuma GD, Carthew J, Lim R, Frith JE. Effect of the Microenvironment on Mesenchymal Stem Cell Paracrine Signaling: Opportunities to Engineer the Therapeutic Effect. Stem Cells Dev. 2017 May 1;26(9):617–631. doi: 10.1089/scd.2016.0349 28186467
22. Salomon C, Ryan J, Sobrevia L, Kobayashi M, Ashman K, Mitchell M, et al. Exosomal Signaling during Hypoxia Mediates Microvascular Endothelial Cell Migration and Vasculogenesis. PLoS One. 2013 Jul 8;8(7):e68451. doi: 10.1371/journal.pone.0068451 23861904
23. Jaffe EA, Nachman RL, Becker CG, Minick CR. Culture of human endothelial cells derived from umbilical veins. Identification by morphologic and immunologic criteria. J Clin Invest. 1973 Nov;52(11):2745–56. doi: 10.1172/JCI107470 4355998
24. Daltro GC, Fortuna V, de Souza ES, Salles MM, Carreira AC, Meyer R, et al. Efficacy of autologous stem cell-based therapy for osteonecrosis of the femoral head in sickle cell disease: a five-year follow-up study. Stem Cell Res Ther. 2015 May 29;6 : 110. doi: 10.1186/s13287-015-0105-2 26021713
25. Overath JM, Gauer S, Obermüller N, Schubert R, Schäfer R, Geiger H, et al. Short-term preconditioning enhances the therapeutic potential of adipose-derived stromal/stem cell-conditioned medium in cisplatin-induced acute kidney injury. Exp Cell Res. 2016 Mar 15;342(2):175–83. doi: 10.1016/j.yexcr.2016.03.002 26992633
26. Edwards SS, Zavala G, Prieto CP, Elliott M, Martínez S, Egaña JT, et al. Functional analysis reveals angiogenic potential of human mesenchymal stem cells from Wharton's jelly in dermal regeneration. Angiogenesis. 2014;17(4):851–66. doi: 10.1007/s10456-014-9432-7 24728929
27. Pfaffl MW. A new mathematical model for relative quantification in real-time RT-PCR. Nucleic Acids Res. 2001;29:e45. doi: 10.1093/nar/29.9.e45 11328886
28. Nakatsu MN, Hughes CC. An optimized three-dimensional in vitro model for the analysis of angiogenesis. Meth Enzymol. 2008;443 : 65–82. doi: 10.1016/S0076-6879(08)02004-1 18772011
29. Newman AC, Chou W, Welch-Reardon KM, Fong AH, Popson SA, Phan DT, et al. Analysis of stromal cell secretomes reveals a critical role for stromal cell-derived hepatocyte growth factor and fibronectin in angiogenesis. Arterioscler Thromb Vasc Biol. 2013 Mar;33(3):513–22. doi: 10.1161/ATVBAHA.112.300782 23288153
30. Guedez L, Rivera AM, Salloum R, Miller ML, Diegmueller JJ, Bungay PM, et al. Quantitative assessment of angiogenic responses by the directed in vivo angiogenesis assay. Am J Pathol 2003;162 : 1431–1439, doi: 10.1016/S0002-9440(10)64276-9 12707026
31. Salz L, Driskell RR. The Sox2: GFP+/ - knock-in mouse model does not faithfully recapitulate Sox2 expression in skin. Exp Dermatol. 2017 Nov;26(11):1146–1148. doi: 10.1111/exd.13396 28636810
32. Geyh S, Oz S, Cadeddu RP, Fröbel J, Brückner B, Kündgen A, et al. Insufficient stromal support in MDS results from molecular and functional deficits of mesenchymal stromal cells. Leukemia. 2013 Sep;27(9):1841–51. doi: 10.1038/leu.2013.193 23797473
33. Hamzic E, Whiting K, Gordon Smith E, Pettengell R. Characterization of bone marrow mesenchymal stromal cells in aplastic anaemia. Br J Haematol. 2015 Jun;169(6):804–13. doi: 10.1111/bjh.13364 25819548
34. Ribot J, Caliaperoumal G, Paquet J, Boisson-Vidal C, Petite H, Anagnostou F. Type 2 diabetes alters mesenchymal stem cell secretome composition and angiogenic properties. J Cell Mol Med. 2017 Feb;21(2):349–363. doi: 10.1111/jcmm.12969 27641937
35. Hu C, Li L. Preconditioning influences mesenchymal stem cell properties in vitro and in vivo. J Cell Mol Med. 2018 Mar;22(3):1428–1442. doi: 10.1111/jcmm.13492 29392844
36. Tsai CC, Yew TL, Yang DC, Huang WH, Hung SC. Benefits of hypoxic culture on bone marrow multipotent stromal cells. Am J Blood Res. 2012;2(3):148–59. 23119226
37. Moya A, Paquet J, Deschepper M, Larochette N, Oudina K, Denoeud C, et al. Human Mesenchymal Stem Cell Failure to Adapt to Glucose Shortage and Rapidly Use Intracellular Energy Reserves Through Glycolysis Explains Poor Cell Survival After Implantation. Stem Cells. 2018 Mar;36(3):363–376. doi: 10.1002/stem.2763 29266629
38. Nie Y, Han BM, Liu XB, Yang JJ, Wang F, Cong XF, et al. Identification of MicroRNAs involved in hypoxia - and serum deprivation-induced apoptosis in mesenchymal stem cells. Int J Biol Sci. 2011;7(6):762–8. doi: 10.7150/ijbs.7.762 21698002
39. Pezzi A, Amorin B, Laureano Á, Valim V, Dahmer A, Zambonato B, et al. Effects Of Hypoxia in Long-Term In Vitro Expansion of Human Bone Marrow Derived Mesenchymal Stem Cells. J Cell Biochem. 2017 Oct;118(10):3072–3079. doi: 10.1002/jcb.25953 28240374
40. Ferreira JR, Teixeira GQ, Santos SG, Barbosa MA, Almeida-Porada G, Gonçalves RM. Mesenchymal Stromal Cell Secretome: Influencing Therapeutic Potential by Cellular Pre-conditioning. Front Immunol. 2018 Dec 4; 9 : 2837. doi: 10.3389/fimmu.2018.02837 30564236
41. Vizoso FJ, Eiro N, Cid S, Schneider J, Perez-Fernandez R. Mesenchymal Stem Cell Secretome: Toward Cell-Free Therapeutic Strategies in Regenerative Medicine. Int J Mol Sci. 2017 Aug 25;18(9). pii:E1852. doi: 10.3390/ijms18091852 28841158
42. L PK, Kandoi S, Misra R, S V, K R, Verma RS. The mesenchymal stem cell secretome: A new paradigm towards cell-free therapeutic mode in regenerative medicine. Cytokine Growth Factor Rev. 2019 Apr;49 : 1–9. doi: 10.1016/j.cytogfr.2019.04.002 30954374
43. Todorova D, Simoncini S, Lacroix R, Sabatier F, Dignat-George F. Extracellular Vesicles in Angiogenesis. Circ Res. 2017 May 12;120(10):16581673. doi: 10.1161/CIRCRESAHA.117.309681 28495996
44. Bian S, Zhang L, Duan L, Wang X, Min Y, Yu H. Extracellular vesicles derived from human bone marrow mesenchymal stem cells promote angiogenesis in a rat myocardial infarction model. J Mol Med. 2014 Apr;92(4):387–97. doi: 10.1007/s00109-013-1110-5 24337504
45. Park H, Park H, Mun D, Kang J, Kim H, Kim M, et al. Extracellular vesicles derived from hypoxic human mesenchymal stem cells attenuate GSK3beta expression via mirna-26a in an ischemia-reperfusion injury model. Yonsei Med J. 2018 Aug; 59(6):736–45. doi: 10.3349/ymj.2018.59.6.736 29978610
46. Wysoczynski M, Pathan A, Moore JB 4th, Farid T, Kim J, Nasr M, et al. Pro-Angiogenic Actions of CMC-Derived Extracellular Vesicles Rely on Selective Packaging of Angiopoietin 1 and 2, but Not FGF-2 and VEGF. Stem Cell Rev. 2019 Aug;15(4):530–542. doi: 10.1007/s12015-019-09891-6 31102187
47. Marcus H, Attar-Schneider O, Dabbah M, Zismanov V, Tartakover-Matalon S, Lishner M, et al. Mesenchymal stem cells secretomes' affect multiple myeloma translation initiation. Cell Signal. 2016 Jun;28(6):620–30. doi: 10.1016/j.cellsig.2016.03.003 26976208
48. Konoshenko MY, Lekchnov EA, Vlassov AV, Laktionov PP. Isolation of Extracellular Vesicles: General Methodologies and Latest Trends. Biomed Res Int. 2018 Jan 30;2018 : 8545347. doi: 10.1155/2018/8545347 eCollection 2018. 29662902
49. Chang PY, Zhang BY, Cui S, Qu C, Shao LH, Xu TK, et al. MSC-derived cytokines repair radiation-induced intra-villi microvascular injury. Oncotarget. 2017 Sep 23;8(50):87821–87836. doi: 10.18632/oncotarget.21236 29152123
50. Oskowitz A, McFerrin H, Gutschow M, Carter ML, Pochampally R. Serum-deprived human multipotent mesenchymal stromal cells (MSCs) are highly angiogenic. Stem Cell Res. 2011 May;6(3):215–25. doi: 10.1016/j.scr.2011.01.004 21421339
51. Kim YS, Noh MY, Cho KA, Kim H, Kwon MS, Kim KS, et al. Hypoxia/reoxygenation-preconditioned human bone marrow-derived mesenchymal stromal cells rescue ischemic rat cortical neurons by enhancing trophic factor release Mol Neurobiol. 2015 Aug;52(1):792–803. doi: 10.1007/s12035-014-8912-5 25288154
52. Anderson JD, Johansson HJ, Graham CS, Vesterlund M, Pham MT, Bramlett CS, et al. Comprehensive proteomic analysis of mesenchymal stem cell exosomes reveals modulation of angiogenesis via nuclear factor-kappab signaling. Stem Cells 2016 Mar;34(3):601–13. doi: 10.1002/stem.2298 26782178
53. Chen L, Xu Y, Zhao J, Zhang Z, Yang R, Xie J, et al. Conditioned Medium from Hypoxic Bone Marrow-Derived Mesenchymal Stem Cells Enhances Wound Healing in Mice. PLoS One. 2014 Apr 29;9(4):e96161. doi: 10.1371/journal.pone.0096161 24781370
54. Carolina E, Kato T, Khanh VC, Moriguchi K, Yamashita T, Takeuchi K, et al. Glucocorticoid Impaired the Wound Healing Ability of Endothelial Progenitor Cells by Reducing the Expression of CXCR4 in the PGE2 Pathway. Front Med (Lausanne). 2018 Sep 28;5 : 276. doi: 10.3389/fmed.2018.00276 30324106
55. Assoni A, Coatti G, Valadares MC, Beccari M, Gomes J, Pelatti M, et al. Different Donors Mesenchymal Stromal Cells Secretomes Reveal Heterogeneous Profile of Relevance for Therapeutic Use. Stem Cells Dev. 2017 Feb 1;26(3):206–214. doi: 10.1089/scd.2016.0218 27762666
Zvyšte si kvalifikaci online z pohodlí domova
Nemáte účet? Registrujte se
Zadejte e-mailovou adresu, se kterou jste vytvářel(a) účet, budou Vám na ni zaslány informace k nastavení nového hesla.
