Impact of heart failure on the behavior of human neonatal stem cells in vitro
© Klose et al.; licensee BioMed Central Ltd. 2013
Received: 22 March 2013
Accepted: 20 September 2013
Published: 27 September 2013
Clinical cardiac cell therapy using autologous somatic stem cells is restricted by age and disease-associated impairment of stem cell function. Juvenile cells possibly represent a more potent alternative, but the impact of patient-related variables on such cell products is unknown. We therefore evaluated the behavior of neonatal cord blood mesenchymal stem cells (CB-MSC) in the presence of serum from patients with advanced heart failure (HF).
Human serum was obtained from patients with severe HF (n = 21) and from healthy volunteers (n = 12). To confirm the systemic quality of HF in the sera, TNF-α and IL-6 were quantified. CB-MSC from healthy neonates were cultivated for up to 14 days in medium supplemented with 10% protein-normalized human HF or control serum or fetal calf serum (FCS).
All HF sera contained increased cytokine concentrations (IL-6, TNF-α). When exposed to HF serum, CB-MSC maintained basic MSC properties as confirmed by immunophenotyping and differentiation assays, but clonogenic cells were reduced in number and gave rise to substantially smaller colonies in the CFU-F assay. Cell cycle analysis pointed towards G1 arrest. CB-MSC metabolic activity and proliferation were significantly impaired for up to 3 days as measured by MTS turnover, BrdU incorporation and DAPI + nuclei counting. On day 5, however, CB-MSC growth kinetics approached control serum levels, though protein expression of cell cycle inhibitors (p21, p27), and apoptosis marker Caspase 3 remained elevated. Signal transduction included the stress and cytokine-induced JNK and ERK1/2 MAP kinase pathways.
Heart failure temporarily inhibits clonality and proliferation of “healthy” juvenile MSC in vitro. Further studies should address the in vivo and clinical relevance of this finding.
Cardiac cell therapy is currently being evaluated as a treatment option for patients with severe heart failure (HF) (reviewed in ). In contrast to experimental models of heart disease, cell-based therapy in humans has brought about only moderate improvements in heart function and there is very little evidence of de novo formation of cardiomyocytes. This mismatch between animal experiments and human clinical trials may be explained by age and disease-related impairment of stem cell function in HF patients [2, 3]. To circumvent the limited regenerative capacity of autologous stem cells from elderly and chronically sick patients, neonatal cell products from healthy donors have been suggested as a superior alternative. However, it has not yet been investigated whether these juvenile cells would withstand the harsh environment upon transplantation into a failing heart. Apart from ischemia and pathologic extracellular matrix architecture, HF may affect stem cell function through circulating disease-related humoral factors. An abnormal molecular milieu is present in HF , and several publications have pointed to a role for HF-associated circulating factors in the modulation of adult stem cell function: Yamahara et al., for instance, identified Angiostatin as an inhibitor of human bone-marrow-derived mesenchymal stem cell (hBM-MSC) proliferation and migration; and Gatta et al. showed that serum composition determines growth of colony-forming endothelial progenitor cells (CFU-EC) [5, 6]. The influence of humoral factors on neonatal stem cell function, however, is still unknown. We therefore sought to test the hypothesis that, in vitro, HF serum factors impair the functionality of neonatal cord blood mesenchymal stem cells (CB-MSC). We chose neonatal CB-MSC from healthy donors because this cell type is characterized by young chronological age and absent disease-associated functional impairment, and possesses a marked proliferation capacity and a broad differentiation potential (reviewed in ). In summary, we found that heart disease does have an impact on CB-MSC biology as evident from impaired proliferation characteristics, stimulation of apoptosis and activation of stress signaling pathways.
Material and methods
Study population: heart failure patients and healthy control subjects
Characteristics of healthy controls and HF patients
Healthy control subjects (n = 12)
Heart failure patients (n = 21)
Demographic data and medical history
40 (3, 24–71)
60 (12, 31–82)
HF duration [month]
13 (4.6, 0.3-48)
Time since most recent MI [month]
2.7 (1.8, 0.1-36)
Extent of CAD
NYHA functional class
Heart rate [bpm]
Systolic blood pressure [mmHg]
118 (26, 82–167)
Diastolic blood pressure [mmHg]
76 (19, 54–104)
153 (38, 93–232)
73 (26, 58–149)
24.7 (13.4, 15–38)
Ventricular assist device
Diabetes type II
Chronic obstructive pulmonary disease
Human serum preparation
Blood was drawn by venipuncture into S-Monovettes® (Sarstedt, Nümbrecht, Germany) using the BD Vacutainer Safety-Lok™ blood collection set (BD Medical, Heidelberg, Germany). Serum off the clot was obtained from whole blood which underwent the natural clotting process. Since HF patients routinely receive anticoagulants, blood samples were subjected to a prolonged clotting period (3 h as compared to 30 min: 20 min at room temperature (RT) to initiate the clotting process followed by 2 h 40 min on ice to prevent degradation of serum constituents). After centrifugation for 15 min at 3500 g and 4°C, serum supernatants were sterile filtered. Aliquots were flash frozen and stored in liquid nitrogen, because it took several weeks to recruit enough patients so that experiments with multiple sera could begin. Hemolytic tubes were excluded.
Protein normalization of human serum
The protein content of human blood varies with a number of parameters at the time of blood sampling, such as liquid intake, physical activities, drugs, disease status, and previous infusions . To account for this, serum protein concentration was determined by Bradford assay (Carl Roth, Karlsruhe, Germany) including interpolation from a standard curve established with bovine serum albumin (BSA), and normalized to the lowest concentration (~37 mg/ml, which corresponds to ~10% FCS supplementation) by respective dilution in Gibco® D-PBS with Ca2+ and Mg2+ (PBS++) (Life Technologies, Darmstadt, Germany).
To make sure that sera were indeed typical for patients with chronic HF, selected cytokines were determined using high sensitivity colorimetric assays: Human IL-6 Quantikine HS ELISA Kit (RnD Systems, Wiesbaden-Nordenstadt, Germany) and Human TNF-α Quantikine HS ELISA (RnD Systems). All immunoassays were performed according to the manufacturer’s instructions. Human serum samples were thawed and protein normalized immediately before the assay.
Standard cell culture of human CB-MSC
Cryopreserved human CB-MSC were provided by K.B., who isolated and expanded CB-MSC according to a previously published protocol . Cord blood was obtained with informed consent of the mother, according to the principles outlined in the Declaration of Helsinki and with approval of the local ethical committees in Mannheim and Heidelberg (Ref. 48/05 reconfirmed in 2009). Passage (P) 2 cells were expanded in low glucose Gibco® DMEM (DMEM-LG) (Life Technologies) supplemented with 10% FCS (Life Technologies, pre-tested batch 41F6495K) and 1% penicillin/streptomycin (P/S) (Lonza, Basel, Switzerland). Cells were seeded at a density of ~1000 cells/cm2 in T175 flasks; partial medium change was given every 3 days. At subconfluency, cells were subcultured using Gibco® TrypLE™ Express (Life Technologies), or cryopreserved in FCS supplemented with 10% DMSO (Carl Roth) and stored in liquid nitrogen. Cells used for experiments originated from the umbilical cord of a single healthy donor and had undergone 2–3 freeze-thaw cycles and ~20 population doublings, referred to as P4 cells. Cell culture vessels employed throughout the study were either CELLSTAR® (Greiner Bio-One, Frickenhausen, Germany) or Nunclon™∆ Surface (Nunc, New York, NY, USA) products.
In vitro system establishment and study design
Several criteria (CB-MSC initial seeding density, human serum concentration, exposure time, means and interval of serum supplementation, necessity for dual supplementation using FCS and human serum) were examined for the design of a suitable in vitro system. Unless otherwise stated, final conditions were as follows: Cryopreserved CB-MSC were thawed and plated at a density of 4000 cells/cm2 in medium supplemented with 10% FCS. After cell attachment, on day 0, FCS was replaced by 10% protein-normalized human serum. Complete medium change was performed every 2 days. Total exposure time was 5–14 days. Individual sera were not pooled, but tested separately. Human serum from healthy donors served as experimental control. In parallel, all experiments were also performed with cells maintained under standard culture conditions (FCS supplementation).
MTS metabolic activity assay and BrdU proliferation assay
The CellTiter 96® Aqueous Non-Radioactive Cell Proliferation Assay (Promega, Mannheim, Germany) and the colorimetric BrdU Cell Proliferation ELISA (Roche, Mannheim, Germany) were performed according to the manufacturer’s instructions on days 1, 3 and 5 on triplicate wells of 96-well plates.
DAPI-based direct cell counting
Subsequent to MTS assay, cells were fixed in 4% paraformaldehyde (PFA) (Carl Roth) and stained with Molecular Probes® DAPI (Life Technologies). The Operetta high content screener (PerkinElmer, Rodgau, Germany) was used to capture 23 10X-images per well that covered the whole culture surface. Harmony® software (PerkinElmer) was used for image analysis, which was performed to quantify CB-MSC numbers based on DAPI-stained CB-MSC nuclei. Since CB-MSC are single nucleated cells, nuclei counts served as direct cell counts to validate indirect proliferation readings acquired from colorimetric assays (MTS, BrdU).
Phase contrast microscopy of cell morphology
Morphology of live unstained cells was examined by phase contrast microscopy on days 1, 3, 4 and 5 of human serum treatment.
Flow cytometric immunophenotyping
Cell harvests were washed in PBS and blocked in FACS buffer (1% BSA, 0.05% sodium azide in PBS) for 15 min at 4°C. Triple combinations of antibodies were employed to stain 50,000 cells in 100 μl volume for 30 min at 4°C. Propidium iodide (PI) (BD Biosciences, Heidelberg, Germany) was added after 15 min to a final concentration of 5 μg/ml. Excess antibodies were washed off and cells were resuspended in FACS buffer and analyzed in a BD FACSCalibur flow cytometer (Becton Dickinson, NJ, USA). Fifteen thousand events were acquired and analyzed using FlowJo software (Tree Star, Ashland, OR, USA). The following mouse antibodies were used: Biozol (Eching, Germany): CD14-FITC, CD73-PE; Miltenyi Biotec (Bergisch Gladbach, Germany): CD34-PE, CD45-FITC; eBioscience (Frankfurt, Germany): CD90-APC; antibodies-online (Aachen, Germany): CD105-FITC, HLA-DR-FITC .
Tripotential mesodermal differentiation
For osteogenic and adipogenic differentiation, CB-MSC were grown to subconfluency in the presence of 10% human HF or control serum or FCS in 6-well plates (for q-RT-PCR analysis) or 12-well plates (for stainings). After 7 days, osteogenic or adipogenic induction medium (StemPro® Osteocyte/Adipocyte Differentiation Basal Medium supplemented with StemPro® Osteogenesis/Adipogenesis Supplement, Life Technologies) was added and changed twice per week. After 21 days, cells were fixed and stained with Alizarin Red S or Oil Red O (Sigma-Aldrich, St. Louis, MO, USA) to confirm osteogenic (calcium deposits) or adipogenic differentiation (intracellular lipid granules). For chrondrogenic differentiation a 3-D culture system was used: After 7 days of treatment with 10% human HF or control serum or FCS, CB-MSC were subcultured. Approx. 3.5×105 cells were pelleted in 15 ml tubes (for q-RT-PCR analysis), droplets containing 0.8×105 cells were seeded into 12-well plates to generate micromass cultures (for stainings). Induction medium (StemPro® Chondrocyte Differentiation Basal Medium supplemented with StemPro® Chondrogenesis Supplement, Life Technologies) was added and changed twice per week. After 21 days, micromass cultures were fixed and stained with Alcian Blue (Carl Roth) to visualize proteoglycan deposits. Undifferentiated cells served as negative controls.
Quantitative real-time PCR
Total RNA was extracted from undifferentiated (after 7 days of human serum treatment) and differentiated cells (after 7 days of human serum treatment and 21 days of differentiation) using the Qiagen RNeasy Mini Kit (Qiagen GmbH, Hilden, Germany). Contaminating genomic DNA was removed with DNAse I (Sigma-Aldrich). Subsequently, 100 ng of each RNA sample were random hexamer primed and reverse transcribed into cDNA using the Invitrogen™ SuperScript® III First-Strand Synthesis System (Life Technologies). Real-Time PCR was performed using the Applied Biosystems® Power SYBR® Green PCR Master Mix (Life Technologies) and the Eppendorf Mastercycler ep gradient S realplex2 (Eppendorf AG, Hamburg, Germany) by combining 12.5 μl SYBR Green master mix, 2 μl primer mix (forward:reverse 1:1, final concentration 800nM), 5.5 μl sterile ddH2O and 5 μl cDNA (1.25 ng template per reaction) per well in an Applied Biosystems® MicroAmp® Optical 96-Well Reaction Plate (Life Technologies). Each PCR reaction was performed in triplicates. The following PCR program was applied: initial denaturation: 95°C 10 min; 45 cycles: 95°C 15 s, 60°C 30 s, 72°C 30 s; final step: melting curve program. PCR primers were designed using Primer3 software : (5′-3′): Tissue non-specific alkaline phosphatase, ALP (F: GGAAATCTGTGGGCATTGTG, R: CCCTGATGTTATGCATGAGC); Peroxisome proliferator-activated receptor gamma, PPARγ (F: TGCAGTGGGGATGTCTCATA, R: CAGCGGGAAGGACTTTATGT); Trancription factor SOX-9, SOX9 (F: GAGGAAGTCGGTGAAGAACG, R: AAGTCGATAGGGGGCTGTCT); Ribosomal protein L13, RPL13 (F: CCTGGAGGAGAAGAGGAAAGAGA, R: TTGAGGACCTCTGTGTATTTGTCAA). PCR primers were purchased from Life Technologies. Relative gene expression levels of lineage-specific markers in differentiated and undifferentiated cells were quantified by the following alogorithm: E-Δct. RPL13 served as reference gene.
Flow cytometric cell cycle analysis
Cell harvests were resuspended in PBS++ at a concentration of 106 cells/ml and fixed in ice cold (−20°C) 70% ethanol for at least 2 h at 4°C. Next, cells were washed in PBS++ and stained with PI solution (0.1% TritonX100, 10 μg/mL PI (Sigma-Aldrich), 100 μg/mL RNase A (Carl Roth) in PBS++) for 30 min at RT in the dark. Cellular DNA content was assessed through PI fluorescence, which was determined in a BD FACSCalibur flow cytometer. Fifteen thousand events were acquired in a pre-set “single cell” gate that excluded cell aggregates, and were analyzed using FlowJo software.
CFU-F clonal assay
CB-MSC were subcultured, suspended in DMEM supplemented with 20% FCS (to ensure efficient attachment) and seeded at a density of 2 cells/cm2 into 6-well plates. Subsequent to visual inspection of seeding success, FCS was replaced by 10% human HF or control serum. After 14 days of treatment, cells were washed with PBS++, fixed with cold (4°C) 4% PFA for 30 min at RT, and were stained with 0.5% crystal violet solution (Carl Roth) for 30 min at RT on a rocking shaker. Afterwards excess stain was washed off and plates were air dried. Quantitative (number) and qualitative (size) CFU-F data was obtained from triplicate wells. All events seen in the plates (single cells, clusters comprised of 2, 4, 8, >10, >20, >50, >100, >200 or >500 cells) were counted.
AnnexinV flow cytometric apoptosis detection
Cell harvests and supernatants were used to determine apoptosis by AnnexinV FITC Apoptosis Detection Kit I (BD Biosciences) according to the manufacturer’s instructions. Necrotic cells were discriminated by PI counterstaining. Fifteen thousand events were acquired in a BD FACSCalibur flow cytometer and analyzed using FlowJo software.
After 5 days of human serum treatment total protein from CB-MSC was isolated and quantified using Pro-Prep Protein Extraction solution (Intron Biotechnology, South Korea) and DC Protein Assay (Bio-Rad, Hercules, CA, USA) or BCA Protein Assay Kit (Pierce/Thermo Scientific, Rockford, IL, USA). Protein (15–20 μg) was separated by discontinuous SDS-PAGE and blotted to 0.45 μm nitrocellulose membranes (Bio-Rad, Carl Roth) by o/n wet tank or 40 min semidry transfer. Membranes were blocked for 1.5 h at RT in 5% skim milk prepared in TBS-T (10 mM TrisHcl pH 7.4, 100 mM NaCl, 0.1% Tween20 in ddH2O), washed with TBS-T and incubated with primary antibody o/n at 4°C, washed with TBS-T again and were stained with HRP- or IRDye-labeled secondary antibodies for 1 h at RT. Chemiluminescent protein detection was performed using the Amersham™ ECL Western Blotting Detection Reagents (GE HEALTHCARE, Little Chalfont, UK) and the FluorChem® HD2 Imaging System (Alpha Innotech, Santa Clara, CA, USA). Infrared protein detection was performed using the Odyssey Infrared Imaging System (LI-COR Biosciences, Lincoln, NE, USA). Primary mouse or rabbit antibodies were: Upstate/Millipore (Billerica, MA, USA): Bax; Abcam (Cambridge, UK): alpha Tubulin, p21, p16, p38, Caspase 3; Millipore: GAPDH, pp38; Cell Signaling (Danvers, MA, USA): CDK1, Cyclin E2, Cyclin D1, Cyclin B1, p27, JNK, pJNK, ERK1/2, pERK1/2, GAPDH; Santa Cruz Biotechnology (Santa Cruz, USA): CDK4, CDK2, pp53. Secondary goat antibodies were: anti-rabbit or anti-mouse IgG-HRP (Zymed/Life Technologies) and IRDye®680LT anti-mouse IgG or IRDye®800CW anti-rabbit IgG (LI-COR Biosciences). Band quantification was performed by ImageJ (NIH, Bethesda, MD, USA) as described elsewhere  (FCS treated cells served as standard).
Unless otherwise stated, medians (IQR) given were obtained from results of experiments performed with group sizes of at least four separate control or HF sera. Normal distribution provided, ANOVA with Bonferroni’s post-hoc test was done, otherwise the Kruskal-Wallis-Test or Mann–Whitney U-Test were applied to test for differences between groups. A general linear model was constructed to test the impact of several clinical variables on CB-MSC behavior within the HF patient cohort (see below). Statistical analyses were performed in SPSS 20 (IBM Corporation, Somers, NY, USA).
HF serum cytokines
HF serum treatment does not affect basic MSC characteristics
HF alters clonogenicity and colony formation pattern of CB-MSC
Impaired proliferation of CB-MSC upon HF serum treatment
Cell cycle progression in CB-MSC is inhibited in the presence of HF serum
Insights into the molecular cell cycle machinery of HF serum treated CB-MSC
By immunoblotting, we monitored the expression of stage specific proteins that drive cell cycle progression and act in its regulation. We studied the expression of cyclin dependent kinases (CDK), their activating cyclins and their inhibitors (CDKI) contributing to G1 phase progression (CDK4, Cyclin D1, CDKI p16INK4A), G1-S phase transition (CDK2, Cyclin E2, CDKI p21CIP1 and p27KIP1) and M phase entry (CDK1, Cyclin B1, CDKI p21CIP1). The data are summarized in Figure 5B. While Cyclin D1 expression was elevated and p16 unchanged in response to HF serum (adjusted band densities: Cyclin D1: human control, 0.83 (0.71-1.2) vs. HF, 2.49 (1.81-3.17), p < 0.05; p16: human control, 0.55 (0.43-0.72) vs. HF, 0.39 (0.32-0.5), p = 0.2), completion of G1-S phase transition as well as the G2 and M phase of the cell cycle were clearly inhibited as evidenced by upregulation of p21 and p27, and a trend toward downregulation of Cyclin B1 (p21: human control, 1.23 (0.91-1.4) vs. HF, 2.35 (2.06-2.44), p = 0.03; p27: human control, 1.12 (0.94-2.09) vs. HF, 6.86 (5.59-8.77), p = 0.03; Cyclin B1: human control, 2.32 (1.70-2.79) vs. HF, 1.65 (1.31-1.78), p = 0.2). This pattern indicates that, in response to HF serum, most CB-MSC rest in the G1 phase of the cell cycle, and are not able to progress despite a certain pro-mitotic stimulation (Cyclin D1 upregulation).
HF serum treatment triggers apoptosis in CB-MSC
ERK1/2 and JNK transduce the HF serum cytokine stimulus into CB-MSC response
Heart failure subgroup analysis
Since the regenerative capacity of HF-patient derived stem cells is limited through age and disease [13, 14], the use of neonatal cell products for cardiac cell therapy may represent a better alternative. It is, however, unknown whether the performance of these juvenile cells would be affected by the various stresses imposed by the diseased organism. We therefore investigated the behavior of CB-MSC in response to serum from patients with severe HF. CB-MSC maintained their principal MSC characteristics including surface marker phenotype, osteogenic, chondrogenic and limited adipogenic differentiation capacity. This robustness of the minimal MSC criteria has also been shown for adult hBM-MSC in autologous and allogeneic human serum from healthy individuals , as well as in the presence of autologous human serum from patients with heart disease . Only under more forceful manipulation of MSC in vitro, such as exposure of MSC to local anesthetics or replicative senescence in high passages do MSC display detectable changes in morphology and differentiation capacity [17, 18]. While the minimal MSC properties withstand most external factors, clonality and proliferative capacity are more susceptible. In our experiments, clonal efficiency was reduced in the presence of HF serum, and the colonies that did develop were predominantly small. Thus, within a CB-MSC population some cells are inhibited to divide at all, whereas others are significantly slowed down in doing so. Similar phenomena have been described for cells of endothelial and hematopoietic lineage, where therapeutic interventions in patients partially reversed the inhibitory serum effects [6, 19]. Interestingly, the colony-forming ability of endogenous hBM-MSC seems to be activated in patients with cardiovascular risk factors, but the majority of the patients in that study had coronary artery disease but not HF .
Similar to the results obtained from the CFU-F assay, CB-MSC proliferation as measured by BrdU incorporation, direct cell counting and MTS test was initially inhibited by HF serum. This was associated with strong upregulation of cell cycle inhibitors p21 and p27 that block progression to the S, G2 and M phase. Accordingly, the majority of CB-MSC rested in the G1 phase. Our finding of concomitant Cyclin D1 upregulation indicates attempted or beginning mitosis and may reflect the reversal of the proliferation block at day 5. Overall, the HF induced CB-MSC depression is in line with observations made by Yamahara et al., who used adult hBM-MSC and identified Angiostatin as one mediator of HF induced MSC depression. In our experiments, however, MSC proliferation kinetics caught up with and metabolic activity even exceeded those observed in human control serum around day 5. The most straightforward explanation for this phenomenon is that MSC adapt to the presence of HF serum factors and compensate for the initial proliferation inhibition. Possible mechanisms include downregulation of surface receptors involved, as in agonist-induced desensitization of, for instance, adrenergic receptors. In addition to attenuation of inhibitory signaling, activation of stimulatory intracellular mechanisms may also play a role. It may be argued that methodological factors such as degradation of serum factors in the culture medium also played a role, but the medium was completely replaced every 48 hours.
HF serum treatment also triggered MSC apoptosis, as evidenced by increased phosphatidyl serine exposure and Caspase 3 activation. Such a pro-apoptotic effect of HF serum has also been noted by Mammi et al., who used endothelial cells from healthy donors as a model . Expression of Bax (Bcl-2-associated X protein), which is involved in mitochondrial membrane permeabilization, was not upregulated in our model. One explanation for this contradictory finding is that upon activation Bax changes its conformation, translocated to the outer mitochondrial membrane, and induced cytochrome C release, so that transcriptional activation is not required to induce or accelerate apoptotic cell death (reviewed in ).
Regarding the intracellular signaling pathways, it is well established that MAP kinases relay stress signals upon extracellular stimulation with, for instance, growth factors and cytokines, and among the targets of MAP kinases are regulators of proliferation and apoptosis . The downstream effector MAP kinases are ERK1/2, JNK and p38, all of which directly activate nuclear transcription factors. We found a substantial downregulation of ERK1/2 phosphorylation, possibly due to lower levels of growth factors in HF sera, which may account for impaired proliferation in CB-MSC. We also found that total expression of JNK as well as the amount of phosphorylated JNK were significantly elevated, so that the ratio of phosphorylated to total JNK remained constant despite clear activation of the pathway. This transcriptional regulation of JNK is unusual and underscores the profound effect of HF serum on CB-MSC. Activation of p38, however, does not seem to play a major role. This finding may surprise because p38 is typically strongly induced by inflammatory cytokines, while JNK mediates cellular response to environmental stresses (oxidative stress and DNA damage for instance). MAP kinase pathways leading to JNK are typically activated by FAS death receptors, but also by inflammatory cytokine receptors including TNF-α and TGF-β. A more detailed analysis of HF induced signaling events in somatic stem cells may be necessary in the future.
It was beyond the scope of this study to identify the components of HF serum that are responsible for the temporary MSC depression. As mentioned above, Yamahara et al. described a prominent role of Angiostatin in the inhibition of hBM-MSC by serum from patients with HF . However, it may be safe to assume the effect of HF serum on CB-MSC biology is the result of concerted cytokine actions within a tremendous protein pool. In addition, drugs used for palliative treatment of HF, neurohormones and reactive oxygen species may also play a role .
Limitations of the study
The in vitro setting we chose for our experiments is clearly a very artificial environment that is far from mimicking the situation in vivo, especially in man. Further studies in long-term in vitro settings as well as in vivo are needed to solidify the evidence. Working with pooled patient sera may have provided more robust data in some experiments, but we chose to test the sera separately in order to be able to test for patient-specific confounding factors. Several groups that have pioneered the isolation and characterization of CB-MSC used higher FCS concentrations in their protocols, so that one may suspect that our cells were suffering from low serum concentrations throughout . We chose to conduct our experiments with 10% serum because, first, the primary CB-MSC cultivation and expansion (K.B.) was done this way, and, second, we had only a limited volume of patient serum available for our experiments. It is not possible, either, to infer from our data what the most important molecular stimuli of the depressive HF effects are. In addition to having heart failure, our patients received a multitude of different pharmaceuticals, of which each may interfere with CB-MSC function. Again, further studies would be needed to dissect these effects. In the univariate analysis we found that serum from patients with previous myocardial infarction may inhibit CB-MSC more than that of HF patients without MI (Figure 8). However, these data must be interpreted with caution, because cohort size is very small after stratification. Finally, we worked with a multitude of sera but all our CB-MSC were from the same batch. We chose this approach to limit possible confounding factors with CB-MSC and feel that this is justified because neonatal cells are very uniform and have not been subjected to age, disease and lifestyle-related changes. However, confirmation of our data in other CB-MSC batches would clearly be necessary if immediately relevant conclusions were to be drawn.
We found that serum from patients with advanced HF temporarily inhibits the proliferative performance of “healthy” neonatal cord blood-derived MSC. This proliferation block seems to be overcome after 5 days in our experimental setting, but reduced number of colony-forming units and upregulation of several molecular cell cycle inhibitors remain detectable beyond that point. These data confirm the inhibitory impact of HF on stem cell populations, and demonstrate that even allogeneic neonatal cells are affected by this phenomenon. Although our experiments were performed in an artificial in vitro setting, this kind of study gives valuable insight into the behavior of exogenous therapeutic cell products in response to the diseased recipient organism. Ultimately, such studies may lead to the development of personalized, patient-specific cell therapies that are adapted to the individual patient’s response.
We thank Julia Stein for her help with the statistical analysis, Karla Weber for finalizing the graphics, and Anne Gale for carefully editing this manuscript.
This work was supported by the Berlin-Brandenburg Center for Regenerative Therapies (BCRT) via Charité Universitätsmedizin (FKZ 1315848A) and Helmholtz-Zentrum Geesthacht (FKZ 1315848B).
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