Open Access

HIV-1 and recombinant gp120 affect the survival and differentiation of human vessel wall-derived mesenchymal stem cells

  • Davide Gibellini1Email author,
  • Francesco Alviano2,
  • Anna Miserocchi1,
  • Pier Luigi Tazzari3,
  • Francesca Ricci3,
  • Alberto Clò1,
  • Silvia Morini1,
  • Marco Borderi4,
  • Pierluigi Viale4,
  • Gianandrea Pasquinelli5,
  • Pasqualepaolo Pagliaro3,
  • Gian Paolo Bagnara2 and
  • Maria Carla Re1, 6
Contributed equally
Retrovirology20118:40

https://doi.org/10.1186/1742-4690-8-40

Received: 20 December 2010

Accepted: 25 May 2011

Published: 25 May 2011

Abstract

Background

HIV infection elicits the onset of a progressive immunodeficiency and also damages several other organs and tissues such as the CNS, kidney, heart, blood vessels, adipose tissue and bone. In particular, HIV infection has been related to an increased incidence of cardiovascular diseases and derangement in the structure of blood vessels in the absence of classical risk factors. The recent characterization of multipotent mesenchymal cells in the vascular wall, involved in regulating cellular homeostasis, suggests that these cells may be considered a target of HIV pathogenesis. This paper investigated the interaction between HIV-1 and vascular wall resident human mesenchymal stem cells (MSCs).

Results

MSCs were challenged with classical R5 and X4 HIV-1 laboratory strains demonstrating that these strains are able to enter and integrate their retro-transcribed proviral DNA in the host cell genome. Subsequent experiments indicated that HIV-1 strains and recombinant gp120 elicited a reliable increase in apoptosis in sub-confluent MSCs. Since vascular wall MSCs are multipotent cells that may be differentiated towards several cell lineages, we challenged HIV-1 strains and gp120 on MSCs differentiated to adipogenesis and endotheliogenesis. Our experiments showed that the adipogenesis is increased especially by upregulated PPARγ activity whereas the endothelial differentiation induced by VEGF treatment was impaired with a downregulation of endothelial markers such as vWF, Flt-1 and KDR expression. These viral effects in MSC survival and adipogenic or endothelial differentiation were tackled by CD4 blockade suggesting an important role of CD4/gp120 interaction in this context.

Conclusions

The HIV-related derangement of MSC survival and differentiation may suggest a direct role of HIV infection and gp120 in impaired vessel homeostasis and in genesis of vessel damage observed in HIV-infected patients.

Keywords

HIV-1 gp120 mesenchymal stem cells cell differentiaton apoptosis

Background

Although the main targets of HIV infection pathogenesis are the CD4+ cells of the immune system, several studies have clearly shown that HIV infection directly and/or indirectly targets other cell lineages and organs [1]. In particular, HIV progressively hampered the homeostasis and functionality of the CNS, bone, kidney and cardiovascular system. These organ-specific lesions have gained a growing importance in the monitoring of HIV infected patients [24], especially since the advent of highly active anti-retroviral therapy (HAART) that has increased the patients' life expectancy thereby determining a chronic disease evolution [5].

Clinical and epidemiological studies have shown a consistent connection between HIV infection and a significantly increased incidence of cardiovascular events [69], atherosclerosis, coronary arterial disease and pulmonary hypertension [10]. Some reports have clearly demonstrated that HIV infection represents an independent risk factor for atherosclerosis and coronary arterial disease, and atherosclerotic lesions have been observed in coronary, peripheral and cerebral arteries of HIV positive subjects in the absence of classical risk factors [6, 11, 12]. Carotid artery thickening was up to 24% higher in HIV patients compared with uninfected sex- and age-matched individuals [1315] and large retrospective studies have proved that HIV positive subjects have a higher incidence of cardiovascular events than uninfected individuals [7, 16, 17]. These cardiovascular diseases are mainly related to impaired vessel wall homeostasis [18]. In particular, atherosclerosis is linked to severe endothelial dysfunction with arterial wall injury due to factors that trigger a chronic inflammatory response with subsequent atheromatous plaque formation [19, 20]. The mechanisms involved in the genesis of atherosclerosis and subsequent cardiovascular damage in HIV positive patients have still not been elucidated, even though some putative indications were recently reported [10].

HIV infection is associated with systemic inflammation and chronic immune activation determining a dysregulation of several cytokines such as IL-6, TNF alpha, M-CSF, IL-10 and IL-1 [2124]. These cytokines may be involved in the atherosclerosis to different extents, activating and inducing the migration of monocytes in the vessel structures and eliciting the evolution to macrophages [25, 26]. Monocytes are known to be the precursors of lipid-laden foam cells within the atherosclerotic plaque [27] producing high levels of pro-inflammatory cytokines thereby determining an inflammatory positive feed-back [10]. Moreover, HIV infection affects cholesterol metabolism especially by viral Nef protein, impairing cholesterol metabolism and cholesterol transport in macrophages and probably hastening the development of vessel structure damage [28, 29]. Besides the inflammatory pathway, HIV directly affects endothelial cell layer homeostasis: gp120 and Tat elicit apoptosis in endothelial cells [3032] through caspase activation. HIV-1 gp120 induces a direct release of endothelin-1, IL-6 and TNFα in endothelial cells leading to direct vessel injury by continuous endothelial damage. Recent observations showed that the homeostasis of the endothelial layer structure does not depend exclusively on circulating endothelial progenitors but can also be regulated by multipotent MSCs [3336]. MSCs were isolated in the adventitia and in the subendothelial region of vessels and can be differentiated towards several cell lineages such as endothelial cells, osteoblasts, adipocytes and smooth muscle cells [37, 38]. Hence, these cells may be the targets of HIV and/or viral proteins inducing direct or indirect vessel damage. To our knowledge, no study has been performed on the interplay between HIV infection and MSCs derived from vascular wall structures to investigate its possible role in the induction of cardiovascular disease and atherosclerosis. The specific studies performed on MSCs and HIV interaction were focused on MSCs or stromal cells isolated from bone marrow [3943]. These reports described HIV-related bone marrow derangement mechanisms demonstrating that some strains of HIV are able to infect these cells albeit to a low extent [39, 40, 43] impairing their clonogenic potential with a strong effect on bone marrow cell regulation [40]. In addition, the bone marrow-derived MSCs were affected by viral proteins such as Tat, gp120, Rev and p55 in the specific differentiation to different cellular lineages [41, 42]. The aim of our study was to determine the biological effects of HIV infection and gp120 treatment on vascular wall-derived mesenchymal cells to elucidate a possible additional mechanism underlying the vessel dysfunctions observed in HIV-infected patients.

Materials and methods

Cell cultures and MSC isolation and differentiation

Human arterial segments of femoral arteries from three male multi-organ heart-beating donors (mean age 39 years) were harvested and used for cell isolation as previously described [38, 44]. These vascular artery segments did not have the requirements of length and calibre for clinical use. Isolated MSCs were characterized by flow cytometry and their multi-differentiation potential was determined as previously described [38]. The flow cytometry characterization was carried out on cells taken at passages 3-5 detached by trypsin and washed twice with phosphate-buffered saline (PBS) containing 2% fetal calf serum (FCS; Gibco, Paisley, UK). The cells were stained for 20 minutes at room temperature using the following monoclonal antibodies (mAbs): fluorescein isothiocyanate (FITC) anti-CD29, phycoerythrin (PE)-anti-CD34, FITC-anti-CD44, FITC-anti-CD45, FITC-anti-CD73, PE-anti-CD90, PE-anti-CD105, PE-anti-CD146, PE-anti-CD166 and FITC-anti-KDR, (all from Beckman-Coulter, Fullerton, CA, USA). vWF expression was revealed after permeabilization with the Intraprep Kit (Beckman-Coulter), then incubated with vWFmAb (1/20 in PBS; DakoCytomation, Glostrup, Denmark) for 1 hour at room temperature and subsequently incubated with secondary anti-mouse IgG FITC (1/40 in PBS; DakoCytomation) for 30 minutes at room temperature. PE- or FITC- irrelevant isotype matched mAb served as negative controls. The cells were extensively washed in PBS and then analyzed by Cytomics FC500 Flow Cytometer (Beckman-Coulter). Isolated MSCs were cultured in D-MEM (Lonza, Basel, Switzerland) plus 10% FCS and split every 3-4 days at about 70% density. MSCs were usually seeded at a density of 5 × 103 cells/cm2. For culture expansion, 75 cm2 and 25 cm2 flasks (Becton Dickinson, Palo Alto, CA) treated with collagen (Sigma, St Louis, MO, USA) were used as previously described [44], while for the experiments, the MSCs were seeded in untreated 6-well or 24-well plates (Nunc, Rochester, NY, USA) and employed between passages 4 and 8. To induce adipogenic differentiation, confluent cells were cultured as follows: three cycles of 3 days induction medium and 3 days maintenance medium of hMSC Mesenchymal Stem Cell Adipogenic Differentiation Medium kit (Lonza) were carried out. After a few days the cells containing neutral lipids in fat vacuoles were stained with fresh red oil solution (Sigma) as previously described [45]. MSCs cultured only with adipogenic maintenance medium were taken as the negative control for differentiation. Angiogenic differentiation was assessed on confluent cells, cultured in DMEM (Lonza) with 2% FCS and 50 ng/ml Vascular Endothelial Growth Factor (VEGF; Invitrogen, Carlsbad, CA, USA) for 7 days, changing the medium every 2 days. MSCs cultured in medium without VEGF throughout the induction period were considered the negative control for differentiation [45, 46]. NK-92 cells were kept in α-MEM (Gibco) plus 15% FCS, 15% horse serum (Gibco) and 20 U/ml of recombinant human IL-2 (Peprotech, London, UK). Peripheral blood mononuclear cells (PBMCs) were obtained from healthy donors who gave their informed consent following the Helsinki declaration. PBMCs were kept in RPMI 1640 plus 10% FCS or activated by PHA (5 μg/ml; Sigma) plus IL-2 (10 U/ml).

Viral stocks and infection procedures

HIV-1IIIB and HIV-1Ada stocks were achieved as previously described [40] and titrated by ELISA HIV-1 p24 antigen kit (Biomerieux, Marcy L'Etoile, France). The heat-inactivated HIV-1IIIB (hiHIV-1IIIb) and HIV-1ada (hiHIV-1ada) viruses were obtained after a cycle of inactivation at 65°C for 30 minutes [47]. HIV-1 infection of MSCs was carried out at 50-60% of confluence with HIV-1IIIB or HIV-1Ada (5 ng/ml of HIV-1 p24) in 6-well or 24-well plates for 2 hours at 37°C. The MSC cultures were extensively washed with PBS, kept in medium and cells and supernatants were harvested at specific times. The HIV-1 p24 content in the infection experiments was assayed by ELISA HIV-1 p24 antigen kit (Biomerieux). In some experiments on sub-confluent MSCs the cell cultures were treated with hiHIV-1 strains (5 ng/ml of HIV-1 p24) or recombinant gp120 (1 μg/ml; NIBSC) for 2 hours at 37°C. As controls, the MSCs were treated with p24 (1 μg/ml; NIBSC) or with HIV-1 strains, hiHIV-1 or gp120 pre-treated for 30 minutes at 37°C with 20 μl of rabbit anti-gp120 pAb (NIBSC, Potters Bar, UK) or, alternatively with 20 μl of rabbit anti-p24 pAb (NIBSC). When confluent MSCs were differentiated to endothelial cells, the same treatment by HIV-1 strains or viral proteins was performed before VEGF stimulation. In the experiments on MSCs differentiated to adipogenesis, HIV-1IIIB or HIV-1Ada (5 ng/ml of HIV-1 p24), hiHIV-1 strains (5 ng/ml of HIV-1 p24) or recombinant gp120 (1 μg/ml; NIBSC) were added to cell cultures for 2 hours at 37°C before every differentiating medium replacement. At specific times post-treatment, the cells were collected for appropriate molecular and flow cytometry analysis the procedures described below. The CD4 receptor blockade was performed by p5p (Sigma) treatment as described previously [42, 48].

Proviral and integrated DNA detection

Cellular and proviral DNAs were extracted from samples by DNAeasy kit (Qiagen, Hilden, Germany). Purified DNA (0.5 μg) was amplified by PCR using SK431 and SK462 HIV-1 gag gene oligos as previously described [49]. A specific amplicon of 142 bp was detectable by 2% agarose gel electrophoresis. As a control, parallel amplification of globin gene was carried out as previously described [50]. The integrated HIV-1 proviral DNA was analyzed after gel purification of cell genomic DNA [51] followed by nested Alu-PCR assay as assessed by O'Doherty and coworkers [52]. The first nested PCR amplification was performed on cell genomic DNA (0.5 μg) with primers specific for Alu and gag sequences whereas the second amplification was carried out with HIV-1 LTR oligonucleotide pair. A specific amplicon of 100 bp was detectable by 3% agarose gel electrophoresis.

Qualitative and quantitative RT-PCR amplification

Total mRNA was extracted either from MSCs, PBMCs, NK-92 or from E. coli Dh5α bacteria by High Pure RNA isolation kit (Roche) following the manufacturer's instructions. Total RNA (100 ng) was retro-transcribed and amplified using Quantitect SYBR Green RT-PCR kit (Qiagen) using 400 nM of each β-actin, CD4, CCR5 and CXCR4 specific oligos (for sequences see [49]) in a LightCycler instrument (Roche). The amplification was performed with RT step (1 cycle at 50°C for 20 min) followed by initial activation of HotStar Taq DNA Polymerase at 94°C for 15 min and 40 cycles in three steps: 94°C for 10 s, 60°C for 30 s, 72°C for 60 s. β-actin real time RT-PCR amplification was carried out with an annealing step at 60°C for 15 s and an extension time at 72°C for 25 s. The amplicons were also analyzed in 1.5% agarose gel electrophoresis. The amplification of c-kit, BCRP-1, Oct-4, Notch-1, Sox-2, BMI-1 and β2-microglobulin was assessed following the method described by Pasquinelli and coworkers [38].

To quantify the mRNA expression of several cellular genes involved in the endothelial and adipogenic differentiation, total cellular RNA (100 ng) was retro-transcribed and amplified using Quantitect SYBR Green RT-PCR kit (Qiagen) and 400 nM of each specific oligonucleotide. The amplification was performed with RT step (1 cycle at 50°C for 20 min) followed by initial activation of HotStar Taq DNA Polymerase at 95°C for 15 min and 40 cycles in three steps: 94°C for 10 s, 60°C for 15 s, 72°C for 30 s for C/EBP β, C/EBP δ, adipsin, PPARγ, UCP-1, vWF, KDR whereas for Flt-1 an additional step was added at 78°C for 2 s to analyze the fluorescence. The relative quantifications were performed by specific standard external curves as described [53] and the normalization was performed by parallel amplification of ribosomial 18S as described previously [54]. The specific oligo pairs for adipsin, PPARγ, UCP-1 and ribosomal 18S genes were already published [52], whereas the sequences of C/EBP β, C/EBP δ, vWF, Flt-1 and KDR were:

C/EBPβ: 5' TTCAAGCAGCTGCCCGAGCC 3' and 5' GCCAAGTGCCCCAGTGCCAA 3'

C/EBPδ: 5'-GTGCGCACAGACCGTGGTGA-3' and 5' CGGCGATGTTGTTGCGCTCG 3'

vWF: 5' TAGCCCGCCTCCGCCAGAAT 3' and 5' GTGGGCTGGAGGCCACGTTC 3'

Flt-1: 5'GCCCTGCAGCCCAAAACCCA 3' and 5' CGTGCCCACATGGTGCGTC 3'

KDR: 5'GCGAAAGAGCCGGCCTGTGA 3' and 5' TCCCTGCTTTTGCTGGGCACC 3'

Apoptosis analysis

The apoptotic cells were analyzed on primary sub-confluent MSCs challenged with HIV-1 strains, hiHIV-1 strains or gp120. The cell cultures were washed with PBS and detached by trypsin at specific times after the treatment start. Apoptotic cells were evaluated as previously described [49]. In brief, the cells were fixed in cold ethanol 70% for 15 minutes at 4°C and after washes in PBS the samples were treated with RNase (0.5 mg/ml; Sigma) and then stained with propidium iodide (50 μg/ml; Sigma). The samples were analyzed by FACScan cytometry (Becton-Dickinson) equipped with an argon laser (488 nm) using Lysis II software (Becton-Dickinson).

Flow cytometry analysis of cell surface and intracellular markers

Flow cytometry analysis of cell surface CD4, CXCR4 and CCR5 was carried out by FITC-anti-CD4mAb (Becton-Dickinson), FITC-anti-CXCR4mAb (R&D System, Minneapolis, MI) and FITC-anti-CCR5mAb (R& D System) respectively, whereas FITC- irrelevant isotype-matched mAb served as negative controls. These antibodies were used diluted 1/20 in PBS on 1 × 105 cells for 20 minutes at room temperature. The cells were extensively washed in PBS and then analyzed by Cytomics FC500 Flow Cytometer (Beckman-Coulter). Analysis of intracellular CD4 was performed by staining with the FITC anti-CD4 mAb for 20 minutes at room temperature, after cell fixation with 2% paraformaldehyde and permeabilization with 0.1% saponin. To assay the expression of endothelial specific markers (e.g. Flt-1, KDR, and vWF) by flow cytometry, 1 × 105 MSCs were analyzed at day 7 after detachment with trypsin. FITC-Flt-1mAb (1/20 in PBS; Santa Cruz Biotechnology, Santa Cruz, CA, USA) and FITC-KDRmAb (R&D System) were used at 1/20 in PBS for 20 minutes whereas to reveal vWF, MSCs were permeabilized with the Intraprep Kit (Beckman-Coulter), incubated with vWFmAb (1/20 in PBS; DakoCytomation) for 1 hour at room temperature and subsequently incubated with secondary anti-mouse IgG FITC (1/40 in PBS; DakoCytomation) for 30 minutes at room temperature. Fluorescence intensity data of intracellular and surface proteins were acquired using a Cytomics FC500 Flow Cytometer (Beckman-Coulter). Results were analyzed using the CXP Software (Beckman-Coulter).

PPARγ activity assay

PPARγ transcription factor activity was detected by TransAM PPARγ kit (Active Motif, Carlsbad, CA, USA) as indicated by the manufacturer. This approach is a highly sensitive ELISA assay that provides, after the extraction of nuclear proteins, the determination of PPARγ binding on specific consensus sequence fixed on plate wells. This binding was targeted by specific anti-PPARγ mAb revealed by means of an HRP-conjugated secondary pAb and a colorimetric substrate. The assay was read by spectrophotometer at 450 nm and compared with reference curve after protein concentration normalization.

Statistical analysis

The data are expressed as means ± standard deviation (±SD) of three separate experiments performed in duplicate. Statistical analysis was performed using Student's two-tailed t-test.

Results

Human MSCs can be isolated and purified from peripheral artery vascular wall

Human vascular wall-derived MSCs were characterized by cellular and molecular approaches. Flow cytometry analysis showed that these cells expressed a reliable cell marker phenotype with CD29+, CD44+, CD73+, CD90+, CD105+, CD166+, KDRlow, CD34-, CD45-, CD146- and vWF- (Figure 1). Parallel molecular analysis showed that in the early culture passages these cells exhibited RT-PCR positive detection of embryonic stem cell marker Oct-4 as well as some molecules known to play a role in critical regulatory pathways of stem cells, such as c-kit, BCRP-1, Notch-1, Sox-2 and BMI-1 (data not shown). To determine whether these cells also expressed the mRNAs of classical HIV receptor CD4 and co-receptor CXCR4 and CCR5, total RNA was extracted from MSCs and analyzed with the RT-PCR technique. The CD4, CXCR4 and CCR5 mRNAs were currently detectable as shown in Figure 2A. In parallel, the expression of CD4, CXCR4 and CCR5 proteins was analyzed on the cell membrane using a flow cytometry procedure. CXCR4 and CCR5 were clearly detected on the cell membrane. Staining with FITC-conjugated anti-CD4mAb failed to disclose CD4 protein expression on the cell surface, but when the MSCs were fixed and permeabilized with saponin an intracellular positivity was clearly displayed in about 20% of the cells (Figure 2B). This finding may suggest a complex pattern of CD4 protein regulation expression in these cells that did not rule out the possible presence of a very low level of CD4 protein on the cell membrane below the sensitivity level of flow cytometry.
Figure 1

Analysis of typical MSC markers by flow cytometry. Shadowed areas represent MSCs treated with fluorochrome-conjugated irrelevant isotype matched mAb, whereas unshadowed areas are the MSCs stained with specific fluorochrome-conjugate mAb. A typical pattern of CD29, 34, 44, 45, 73, 90, 105, 146, 166, vWF, KDR is shown.

Figure 2

Analysis of CD4, CXCR4 and CCR5 expression in MSCs. Analysis of CD4, CXCR4, CCR5 and β-actin mRNA expression by qualitative real time RT-PCR in MSCs (A). A typical gel electrophoresis of qualitative real time RT-PCR is shown. As positive controls, total RNAs extracted from PBMC were employed. The total RNAs extracted from NK-92 cells (for CD4) and E. coli total RNA (for CXCR4 and CCR5) served as negative control. Panel B displays a typical flow cytometry analysis of CCR5, CXCR4 and CD4 staining in MSCs. Unshadowed areas represent MSCs treated with FITC-conjugated specific mAb, whereas the negative control (MSCs stained by FITC-conjugated irrelevant isotype matched mAb) is represented by shadowed areas. Three experiments were performed in duplicate.

HIV-1ada and HIV-1 IIIbintegrate their retrotranscribed proviral DNA in host MSC genome

To determine whether MSCs can be considered targets of HIV-1 infection, subconfluent MSCs were challenged with two classical HIV-1 X4 and R5 laboratory strains represented by HIV-1IIIb and HIV-1ada respectively. Total DNA, collected and purified at days 3 and 7 post-infection, was analyzed by PCR, and both HIV-1IIIb and HIV-1ada proviral DNAs were disclosed (Figure 3A). In parallel experiments, the integrated viral DNA in the MSC genome was analyzed by a nested-Alu PCR where the first oligo pair amplifies regions of different length between Alu regions and HIV-1 gag gene whereas the second amplification was performed with internal HIV-1 specific oligos to obtain a specific 100 bp amplicon. Whole DNA was extracted from MSCs at days 7 and 10 post-infection, and HIV-1 specific 100 bp product was detected (Figure 3B). Hence, these results indicate that both HIV-1 strains enter MSC cells and retrotranscribe their RNA genome to proviral DNA integrating it in the host cell genome. To establish whether HIV infection of MSCs determines the production of new viral progeny, we analyzed the p24 protein burden by ELISA in MSC supernatants. The p24 protein was barely detected and progressively decreased over time suggesting that the MSCs showed a very low permissivity to HIV infection in these experimental conditions (Figure 3C).
Figure 3

HIV-­‐1 proviral DNA and p24 protein detection in MSCs infected by HIV-­‐1 strains. Analysis of HIV-1 proviral DNA by qualitative real time PCR (A): agarose gel electrophoresis of MSC infected by HIV-1IIIb and HIV-1ada at days 3 and 7 post-infection. Positive control was activated PBMC at day 3 and negative control was mock-infected MSCs. All experiments were performed using 5 × 105 MSC or activated PBMCs infected or not with HIV-1IIIb and HIV-1ada (5 ng/ml p24). Panel B shows DNA integrated proviral HIV-1. The total DNA extracted from 5 × 105 MSC or activated PBMC cells was run in agarose gel electrophoresis and, after the purification of cellular DNA as previously described (51), a nested Alu-PCR was performed. The MSCs challenged by HIV-1 strains were analyzed at day 7. Activated PBMCs infected with the two HIV-1 strains served as positive controls. A specific LTR 100 bp band is detectable in HIV-1 infected MSCs and positive controls. Panel C displays the cell supernatant p24 analysis. ELISA p24 kit was employed to analyze the p24 content in cell supernatant. This assay exhibits a sensitive limit at 3 pg/ml. The amount of p24 in MSCs challenged with HIV-1 strains was very low and, in these experimental conditions, slowly declined at later tested times. The positive controls were performed by activated PBMC infected with HIV-1 strains.

HIV-1 strains and recombinant gp120 induce apoptosis in subconfluent MSCs

Besides the direct infection of specific targets, HIV employs several pathogenetic mechanisms among which apoptosis activation plays a pivotal role in several cell models such as CD34+ hematopoietic progenitor cells and T cells. To investigate whether the interaction between HIV-1 and MSCs induces apoptosis activation, subconfluent MSCs were exposed to both HIV-1 strains, and the apoptotic cell percentage was assessed with propidium iodide flow cytometry technique. The flow cytometry analysis performed at day 1, 3 and 7 post-infection showed a significant increase in apoptotic cells (Figure 4A) in the samples challenged with the two HIV-1 strains at day 3 (13.9 ± 3.2% and 11.2 ± 2.5% in the HIV-1IIIb or HIV-1ada infected samples respectively, in comparison with 4.4 ± 0.5% of apoptotic cells detected in the mock-infected cultures; p < 0.05) and to a lesser extent at day 7 (10.3 ± 1.4% and 10.1 ± 1.2% in the HIV-1IIIb or HIV-1ada infected samples respectively, in comparison with 5.2 ± 0.4% in the mock-infected cultures; p < 0.05). The parallel challenge of MSCs with recombinant viral gp120 (11.8 ± 2% vs 4.4 ± 0.5% at day 3) or heat inactivated (hi)HIV-1 strains displayed a similar apoptosis increase pattern (Figure 4B). The pre-treatment of HIV-1 strains or gp120 with neutralizing rabbit pAb to gp120 elicited a clear inhibition of apoptosis induction (Figure 4B). Since the interaction between gp120 and CD4 was related to programmed cell death in different cell models, MSCs were treated by p5p (a CD4 antagonist) and challenged with HIV-1IIIb, HIV-1ada or gp120. This p5p treatment induces a significant inhibition of HIV related apoptosis induction at days 3 and 7 indicating that CD4 blockade tackled the HIV-1 and gp120 related MSC apoptosis (Figure 4C).
Figure 4

Determination of apoptotic cell percentage by a flow cytometry procedure. Sub-confluent MSCs treated with HIV-1 strains (5 ng/ml p24) and recombinant gp120 (1 μg/ml) were assayed (panel A) with propidium iodide staining after cell fixation at different times (days 1, 3, and 7). Panel B reports the apoptosis induction when hiHIV-1 strains or gp120 were used. Panel C represents the apoptotic cell percentages obtained when CD4 blockade by p5p treatment was performed. Statistical significance was determined using Student's t test with *p < 0.05.

In the next series of experiments, we studied whether HIV-1 strains and/or gp120 elicited apoptosis in MSCs differentiated towards adipogenic and endothelial cell lineages. Interestingly, biologically active or hiHIV-1 strains and gp120 failed to determine a significant apoptosis induction during the adipogenetic or endothelial differentiation (data not shown) suggesting that these differentiation stimuli could prevent the negative survival signal induced by viral treatment.

HIV-1 and recombinant gp120 positively modulate the MSCs differentiation to adipogenesis

MSCs isolated from blood vessels can be differentiated into several lineages such as osteoblast, adipocyte, smooth muscle and endothelial cells. To study the effects of HIV-1 on the differentiation of these cells, the interaction of HIV-1 and recombinant gp120 on MSC differentiation to adipogenic and endothelial lineages was analyzed. The adipogenic differentiation was tested at different times by direct staining of cell cultures with red oil. The microscopic evaluation of the red oil stained cell cultures showed a reliable increase in red oil stained cells in the cell cultures treated with viral agonists at days 7 and 10 (Figure 5), in comparison with control cultures indicating that the HIV-1 and gp120 enhanced a more rapid and massive differentiation of MSC stimulated to adipogenic lineage. Since PPARγ is currently considered the most important regulator of adipogenesis through its transcription factor activity, we assayed with ELISA TransAM assay the PPARγ activity at day 7 in the same experimental conditions. HIV-1IIIb, HIV-1ada and recombinant gp120 induced (Figure 6A) a significant up-regulation of PPARγ activity in comparison with the cell culture control (3.4 ± 0.5 fold increase with HIV-1IIIb (p < 0.05), 3 ± 0.4 fold increase with HIV-1ada (p < 0.05) and 2.7 ± 0.5 fold increase with gp120 (p < 0.05) when the cell cultures were challenged either by HIV-1 strains or gp120. This effect was abolished when HIV-1 strains or gp120 were pre-treated with anti-gp120 pAb. In parallel, the PPARγ mRNA content evaluated by quantitative real time RT-PCR (Figure 6B) showed a slight but significant up-regulation of specific transcripts (2 ± 0.5 fold increase with HIV-1IIIb; p < 0.05, 1.7 ± 0.3 fold increase with HIV-1ada; p < 0.05 and 1,8 ± 0,4 fold increase with gp120; p < 0.05) with respect to induced cell culture controls. Since adipogenesis is regulated by several factors modulating specific gene expression, the mRNA expression of other specific genes involved in adipogenesis regulation was analyzed. The early steps of differentiation are linked to activation of C/EBP β and δ, which, in turn, activate C/EBP α and PPARγ inducing the complete differentiation to mature adipocyte with the expression of late differentiation markers such as adipsin and UCP-1. The analysis of C/EBP β and δ mRNA expression was analysed by quantitative real time RT-PCR (Figure 7A). HIV-1 and gp120 induced a significant up-regulation of C/EBP β (8.2 ± 2.3, p < 0.05 with HIV-1IIIb, 5.8 ± 1.4 p < 0.05 with HIV-1ada and 4.7 ± 1.3 p < 0.05 with gp120) and δ (3.6 ± 1.2, p < 0.05 with HIV-1IIIb, 3.4 ± 1.3 p < 0.05 with HIV-1ada and 3.5 ± 0.9 p < 0.05 with gp120) mRNAs at day 3. As expected, the pre-treatment of HIV-1 strains or gp120 with anti-gp120 pAb inhibited the specific mRNA increase. In parallel, some late adipogenetic markers such as adipsin and UCP-1 mRNAs expression were studied with quantitative real time RT-PCR at day 10. HIV-1 strains and gp120 positively modulated the adipsin mRNA expression whereas UCP-1 is poorly expressed and did not show any significant quantitative mRNA variation related to any treatment (Figure 7B) suggesting that MSCs in these experimental conditions underwent a differentiation toward white fat rather than brown fat. The CD4 blockade by p5p determined a significant decrease of adipogenesis induction (Figure 5) by HIV-1 strains and gp120 as well as PPARγ activity up-regulation (Figure 6C-D). Consistently, the treatment with p5p also decreased the HIV-related activation of C/EBPβ, C/EBPδ and adipsin mRNA expression (Figure 7C-D) indicating a general down-regulation of HIV related proadipogenetic effects.
Figure 5

Red oil staining of MSCs differentiated towards adipogenesis at day 10. MSCs challenged with HIV-1 strains (5 ng p24/ml) or gp120 (1 μg/ml) displayed more abundant multivacuolar adipogenic vescicles in the cytoplasm than untreated differentiated cells. Neutralizing anti-gp120 pAb or p5p treatment in MSC samples challenged with HIV-1 or gp120 inhibited the increase in red oil stained lipid drop amount. Magnification 200X.

Figure 6

Effect of HIV-1 strains and gp120 on PPARγ transcription factor activity and mRNA expression in MSCs differentiated to adipogenesis. In A and C, MSCs were challenged with HIV-1 strains (5 ng/ml) and gp120 (1 μg/ml) in the presence or absence of anti-gp120 pAb, anti p24 pAb and p5p. MSCs were harvested at day 7 and nuclear extracts were processed for PPARγ activity using TransAM PPARγ kit. The PPARγ activity data were expressed by the ratio (±SD) between samples and the control represented by MSC cell cultures differentiated to adipogenesis. The adipogenesis differentiated cell culture PPARγ activity was set at 1. Three experiments performed in duplicate were carried out. In B and D, quantitative real-time RT-PCR was performed at day 7 to analyze PPARγ mRNA expression in cell cultures treated with the viral strains and viral proteins. The mRNA expression data were expressed by the ratio between samples and the control represented by adipogenesis differentiated cell cultures after 18S ribosomial normalization. The adipogenesis differentiated cell culture mRNA was set at 1. Three experiments performed in duplicate were carried out. Statistical significance was determined using Student's t test with *p < 0.05.

Figure 7

Analysis of mRNA expression of specific early and late genes involved in adipogenesis by quantitative real time RT-PCR. MSCs were challenged with HIV-1 strains (5 ng/ml) and gp120 (1 μg/ml) in the presence or absence of anti-gp120 pAb, anti p24 pAb and p5p. Panel A and C show the up-regulation of two transcription factor gene expressions such as C/EBP β and C/EBP δ involved in the early stages of differentiation. The analysis was performed at day 3 post-stimulation and the two mRNA were significantly increased with respect to adipogenesis differentiated cell cultures. In B and D, some late markers of adipogenic differentiation such as adipsin and UCP-1 mRNA expression were analyzed. Adipsin was significantly up-regulated at day 10 whereas UCP-1 a marker of brown fat was barely expressed and without any significant difference with respect to the controls. The results were expressed by the ratio between samples and the control represented by adipogenesis differentiated cell cultures after 18S ribosomial normalization. The adipogenesis differentiated cell culture mRNA was set at 1. The data represent the mean (+SD) of three independent experiments performed in duplicate. Statistical significance was determined using Student's t test with *p < 0.05.

HIV-1 and recombinant gp120 inhibit the MSCs endothelial differentiation

In a next series of experiments, we investigated the effects of HIV-1 and gp120 on endothelial differentiation of MSCs induced by VEGF treatment. When MSCs were treated with VEGF, they differentiated to endothelial cells exhibiting several specific endothelial markers. To assess whether the endothelial differentiation may be positively or negatively affected by viral challenge, the expression of some endothelial markers such as vWF, Flt-1 and KDR was analyzed by a flow cytometry procedure. This approach displayed a clear decrease of all three markers (Figure 8) when MSCs were challenged by gp120 or HIV-1 strains. In parallel, quantitative real time RT-PCR was carried out and the results confirmed a significant decrease of Flt-1, KDR and vWF mRNA expression when HIV-1 strains or gp120 were added to cell cultures (p < 0.05; Figure 9A). Moreover, the treatment of cell cultures with p24 or gp120 and HIV pre-treated with neutralizing anti-gp120 pAb did not show any significant biological effect on mRNA and protein endothelial marker expressions.
Figure 8

HIV-1 strains and gp120 inhibited the protein expression of some specific differentiation markers on MSCs differentiated towards the endothelial lineage. MSCs were differentiated to endothelial cells by VEGF treatment and at day 7 the cell cultures were collected and flow cytometry analysis of vWF, Flt-1 and KDR protein showed an inhibition of these three markers in MSC samples challenged with HIV-1 or gp120. In the histograms, shadowed areas represent the isotype irrelevant FITC-labeled mAb treated samples, the unshadowed areas represent VEGF treated sample challenged with HIV-1 or gp120 with or without neutralizing anti-gp120 pAb. A typical experiment is shown.

Figure 9

Determination of vWF, Flt-1 and KDR mRNA by quantitative real-time RT-PCR. MSCs were differentiated to endothelial cells by VEGF and challenged with HIV-1 strains and gp120 in the presence or absence of anti-gp120 pAb, anti p24 pAb (panel A) and p5p (panel B). Total RNA was extracted and purified at day 7 and vWF, Flt-1 and KDR mRNAs were analysed. The results were expressed by the ratio between samples and the control represented by VEGF-differentiated cell cultures after 18S ribosomial normalization. The VEGF treated control cell culture mRNA was set at 100. The data represent the mean (+SD) of three independent experiments performed in duplicate. Statistical significance was determined using Student's t test with *p < 0.05.

We also analysed whether p5p treatment may affect the HIV-related inhibition of VEGF-driven MSC differentiation. As shown in Figure 9B and 10, CD4 blockade determined a clear recovery of vWF protein and mRNA expression at day 7 as well as for Flt-1 and KDR (Figures 9 and 10 and data not shown) in HIV-1 and gp120 treated samples.
Figure 10

Flow cytometry analysis of vWF intracellular protein in MSC challenged by HIV-1 and gp120 with or without p5p treatment at day 7. CD4 blockade by p5p inhibited the HIV-related negative modulation of intracellular vWF protein in VEGF-differentiated cell cultures. Shadowed areas represent samples treated with irrelevant mAb plus FITC-conjugated secondary antibody, whereas unshadowed areas are the MSCs stained with anti-vWF mAb plus FITC-conjugated secondary antibody. A typical experiment is shown.

Discussion

Human MSCs are multipotent cells that can be isolated from almost all tissues and organs in the human body [55]. These cells have the potential to differentiate by specific stimuli to different cell lineages and can be involved in tissue repair and homeostasis [56]. Several studies have demonstrated MSCs in the blood vessel wall that can be differentiated to endothelial, adipocyte, osteoblast and smooth muscle cells [38, 5759]. In particular, MSCs isolated from the blood vessel wall are strongly involved in the control of endothelial layer structure and vessel wall homeostasis [60] suggesting that their impairment may play an important role in vessel damage and atherosclerotic evolution. Since cardiovascular lesions, particularly atherosclerosis, represent major clinical manifestations during the evolution of HIV-related disease [1315, 61], we investigated the interaction between HIV-1 and MSCs isolated from the vessel wall to establish whether HIV-1 is able to impair MSC biology. This report focused on two main aspects: the direct effects of HIV-1 challenge and gp120 treatment on primary vessel wall MSCs and the impact of viral action on MSC differentiation towards specific cellular lineages to identify possible mechanisms involved in the derangement of vascular structure observed in HIV-1 positive individuals. Two classical HIV-1 X4 and R5 laboratory strains were able to enter, retro-transcribe and integrate the proviral DNA in the MSC host genome but the very low level of p24 protein content detected in the cell supernatant raised the possibility that the MSCs may be considered barely permissive to HIV-1 infection.

Previous studies [39, 40, 43] disclosed that HIV productively infected bone marrow mesenchymal or stromal cells to different extents. Recent data on bone marrow-derived MSCs demonstrated that HIV-1 proviral DNA integration was detected after HIV-infected sera challenge [42] in the absence of detectable HIV-1 p24 in the cell supernatants. It is conceivable that the relative discordance among the results described in these studies is related to both MSC culture isolation purity and the specific anatomical origins (bone marrow and vessel wall) that may induce different responses to HIV-1 challenge. Interestingly, the indication that vessel wall MSCs were subjected to proviral DNA integration in the DNA host genome may suggest a possible role of MSCs as a potential infection reservoir. However, the importance and the relative possibility of HIV reactivation by this reservoir must be assessed by further studies to discern its true extent and biological impact in vivo. Following these data on the sensitivity of MSCs regarding the HIV infection, we also studied the effects of HIV on the survival of primary MSCs. Apoptosis activation plays a pivotal role in some HIV-1-related pathogenetic aspects related to specific cell lineage progressive loss [62]. Programmed cell death is considered an important pathway involved in the progressive decline of CD4+ T lymphocytes and in the anemia, granulocytopenia and thrombocytopenia, due to impaired CD34+ hematopoietic progenitor survival, occurring in several patients during HIV-related disease development [1, 2, 62]. Moreover, Tat and gp120 are involved in the apoptosis of neuronal and osteoblast cells, respectively, supporting, at least in part, the AIDS dementia complex and the osteopenia/osteoporosis observed in several HIV-positive individuals [3, 4, 49]. The treatment of sub-confluent vessel wall MSCs with both HIV-1 strains lead to significant apoptosis activation. Interestingly, HIV-1 strains and gp120 are able to elicit apoptosis induction that is inhibited in presence of anti gp120pAb or p5p treatment. This suggests that the interaction between gp120 and CD4 plays an important role in the activation of programmed cell death. HIV-1 gp120 recognizes CD4 as its main receptor even though it is well known to bind other cell receptors such as the galactocerebroside molecule (GalC) determining a wide array of biological effects from infection of susceptible cells to induction of signal transduction intracellular pathways [63]. In particular the interaction between gp120 and CD4 determines apoptosis activation in several cell lineages such as CD34+ hematopoietic progenitor cells and CD4+ cells [6466]. The vessel wall MSCs express the CD4 mRNA in the absence of detectable amounts of CD4 protein on the cell membrane by flow cytometry analysis. However, the presence of CD4 protein below the sensitivity limit of the technique cannot be ruled out because flow cytometry showed its detection limit at around 1,000 fluorescent molecules [67]. Moreover, the intracellular detection of a low amount of CD4 in about 20% of MSCs suggests a possible complex regulation of CD4 protein expression in these cells. It is noteworthy that this pattern of CD4 expression (mRNA positivity and protein undetectable on cell membrane by flow cytometry) was previously observed on MSC purified from bone marrow [39] and in other cell lines sensitive to HIV infection that underwent productive infection and/or apoptosis induction [6769]. Interestingly, apoptosis activation was not detected when the MSCs were committed to fat or endothelial cells. The treatment with differentiation inducers and the cell confluence may tackle the HIV-1 strains/gp120-induced negative signals. VEGF, for example, induces a strong activation of cell survival pathways with the phosphorylation of AKT via activation of PI-3-kinase that determines cell survival during the differentiation [70, 71]. In addition, MSCs differentiate when the cells are confluent suggesting a possible role of the cell cycle and then a specific pattern of transcription factors in survival regulation.

Since the vessel wall MSCs exhibited cell differentiation multipotency, we analyzed the HIV-1 impact on MSCs when these cells were differentiated towards specific cell lineages represented by adipocytes and endothelial cells. Adipogenesis is regulated through a sequence of cellular and molecular events well described in pre-adipocye cell models such as the 3T3-L1 cell line and stem cell lines [72, 73]. After the growth arrest in confluence, the cells in these models were subjected to clonal expansion mediated to induction of C/EBP β and C/EBP δ [74, 75] that positively regulate the expression of some adipocyte specific genes. In particular, these transcription factors activate C/EBPα and PPARγ [76], which in turn modulate the further steps of the differentiation programme to adipocytes. PPARγ is a pivotal factor for in vivo adipogenesis: PPARγ deficient mice are characterized by a total absence of white and brown adipose tissue [77]. In vessel wall MSCs, HIV-1 and gp120 are able to enhance adipogenesis and up-regulate PPARγ activity. PPARγ has already been described as a target of gp120. Cotter and coworkers [78] reported increased PPARγ activation in primary osteoblasts with a dysregulation of osteoblastogenesis also associated with RUNX-2 inhibition. In addition, Rev and p55 were able to activate PPARγ in MSCs from bone marrow [41]. These observations suggested that the modulation of PPARγ by HIV proteins during HIV infection may be considered a co-factor in the lipid and bone derangement observed during the HIV infection and in some antiretroviral treatments [79]. Our data also showed that viral infection and gp120 exposure induced an up-regulation of C/EBPβ and δ mRNA expressions demonstrating that adipogenesis positive modulation is determined until the first differentiation molecular steps. Interestingly, C/EBPβ factor modulates HIV-1 expression and replication in monocyte/macrophages and is even activated by the gp120/CD4 interaction through the MAP kinase pathway [80] suggesting a more complex role of this transcription factor in HIV-1 pathogenesis. Of note, CD4 blockade determined a significant decrease of HIV-related adipogenesis in agreement with data described by Cotter and coworkers in bone marrow-derived MSCs (42). Altogether, these observations suggest that these HIV-related pro-adipogenic effects in MSCs purified from different anatomical districts, might be induced, at least in part, by CD4/gp120 binding.

Until the study by Asahara and coworkers [33], it was generally postulated that the formation of new vessels in the adult originated from sprouting of pre-existing vessels [81, 82]. More recent studies showed that endothelial cells could also be renewed by other cell types such as mesenchymal cells with a more complex regulation of vessel wall structure homeostasis [36, 37, 83]. In particular, adult human arteries contain multipotent MSCs that reside within specific zones of the vascular wall such as the sub-endothelial space and vascular adventitia [37]. In our model, we analyzed the impact of HIV-1 and gp120 protein on MSCs differentiated by VEGF treatment to endothelial cells studying the mRNA and protein expression of specific endothelial markers such as vWF, Flt-1 and KDR. Unlike adipogenesis, endothelial differentiation was impaired by HIV-1 and gp120 as documented by a decrease of vWF, Flt-1 and KDR mRNA and protein expression that is strongly inhibited by CD4 blockade. This impairment of endothelial differentiation may represent an interesting additional pathogenetic model in HIV-1 infection. The dysfunction of endothelial cells and vascular structure has been proven in HIV patients [9, 10]. In particular, several studies have described how chronic inflammation, platelet activation and hypercoagulability elicit damage to endothelial homeostasis [8486] and may play a role in the linkage between HIV infection and cardiovascular disease [9].

HIV-related chronic inflammation determines the expression of several cytokines especially in mononuclear cells such as IL-6, IL-8 and TNF α [22, 23, 87, 88] which activate endothelial cells and enhance leukocyte adhesion. In addition, gp120 is able to determine direct and indirect injury to endothelial cells. This viral glycoprotein induces apoptosis in endothelial cells especially in the lung, thereby contributing to pulmonary hypertension [30, 89]. HIV-1 gp120 also stimulates the activation of cytokines like IL-6 and TNF α [90] resulting in damage to endothelial vessel structure.

Vascular injury and atherosclerosis have been described in HIV positive patients: autopsy reports demonstrated atherosclerotic lesions in peripheral, coronary and cerebral arteries in the absence of traditional atherosclerosis risk factors [1113]. Several retrospective studies performed on HIV-infected individuals have demonstrated a two-three fold rise in the incidence of cardiovascular disease in comparison with sex and age-matched healthy subjects [7, 16, 61]. In addition, an analysis of surrogate markers of coronary artery disease showed that carotid artery intima-media thickness (IMT) is increased up to 24% in HIV-infected patients with respect to controls [13].

The HIV-related mechanisms of atherosclerosis induction and cardiovascular damage remain unsettled. Some studies have suggested that the atherosclerosis induction observed in HIV-positive patients is linked to the direct effect of HIV infection and/or viral proteins on cholesterol metabolism in monocytes [28, 91, 92]. These cells represent the precursors of the lipid foam cells within the atherosclerotic plaque producing a high level of IL-6, a cytokine positively regulated also by Tat [10, 21, 24]. The foam cells produce proatherogenic factors such as chemokines, cytokines and metalloproteinases, which promote plaque expansion with instability of lesions and vascular cell degeneration and apoptosis [10, 29]. In addition, chronic infection and endothelial damage determine a significant increase in monocyte migration exacerbating vessel damage [25].

Conclusions

Our data suggest an additional HIV-related mechanism of vessel wall and endothelial layer injury, involving MSCs. HIV affects MSC biology acting on both uncommitted and committed MSCs. HIV is able to integrate its genome in vascular wall MSC DNA. Apoptosis activation is mainly activated through the gp120/CD4 interaction that also plays an important role even in differentiation derangement. This shows a direct effect on primary MSCs that decreases the viable MSCs suited for vessel structure homeostasis. Our findings may even suggest the role of reservoir for HIV infection in MSCs although the true clinical and virological impact awaits clarification.

HIV and gp120 negatively influence endotheliogenesis thereby facilitating diffuse vascular damage and the promotion and development of atherosclerosis lesions due to impaired MSC repair control of endothelial and vessel structure. On the other hand, HIV and gp120 induce the differentiation of MSCs to adipocytes through PPARγ activity and C/EBP β expression up-regulation leading to speculate that not all subintimal foam cells originate from monocytes. The HIV-related induction of adipocyte differentiation can determine a derangement of MSC differentiation balance with a possible involvement in atherosclerosis genesis and development. Interestingly, some peculiar lesions are found in atherosclerothic vessel degeneration such as cartilaginous metaplasia with endocondral ossification and fat tissues, especially in inflammatory abdominal aortic aneurysms [93, 94] that have not been well explored and might be related to dysregulated MSC differentiation. Altogether, these results indicate that HIV and gp120 have a strong direct impact on vessel wall MSC biology and differentiation. These observations may help to explain the early and diffuse atherosclerosis and vascular damage observed in HIV-infected patients.

Conflict of interest statement

The authors declare that they have no competing interests.

Notes

Declarations

Acknowledgements

The HIV-1 rgp120 was provided by the EU programme EVA/MRC Centre for AIDS Reagents, NISBC/MRC (Contract QLKZ-CT-1999-00609) Immunodiagnostics, UK Medical Research Council. We thank NIBSC also for p24, anti-gp120 pAb and anti-p24 pAb. This study was supported by following grants: Fondazione Cassa di Risparmio Bologna, Italy, Italian Ministry of Health (AIDS project), University of Bologna (selected topics) and MURST 60%.

Authors’ Affiliations

(1)
Department of Haematology and Oncological Sciences, Microbiology Section, University of Bologna
(2)
Department of Histology, Embryology and Applied Biology, University of Bologna
(3)
Transfusion Medicine Service, St Orsola Hospital
(4)
Department of Internal Medicine, Aging and Nephrology, Infectious Diseases Section, University of Bologna
(5)
Department of Haematology, Oncology and Clinical Pathology, University of Bologna
(6)
Interuniversity Consortium, National Institute Biostructure and Biosystems (INBB) Rome

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