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Serum extracellular vesicles expressing bone activity markers associate with bone loss after HIV antiretroviral therapy

Marques de Menezes, Erika G.a,b; Ramallho, Janainac; Bucovsky, Marianad; Shane, Elizabethd; Yin, Michael T.d; Norris, Philip J.a,b,e

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doi: 10.1097/QAD.0000000000002430
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Abstract

Introduction

Most studies report that BMD decreases by 2--6% in adults with HIV within 12 months after initiating antiretroviral therapy (ART) [1–3] and may be associated with higher risk of fracture during the first 2 years after ART initiation [4]. As bone loss is consistently observed across different ART regimens, one theory is that the inflammatory state-associated immune reconstitution with ART leads to an imbalance in bone remodeling, favoring osteoclastogenesis and bone resorption [5–9]. Ofotokun et al.[10] found that levels of the bone resorption marker, C-telopeptide (CTx) increased 200% within 12 weeks after ART initiation, and was accompanied by increases in plasma levels of receptor activator of NF-kB ligand (RANKL) and tumor necrosis factor-α (TNF-α); furthermore, CTx levels correlated with the magnitude of CD4+ T-cell repopulation. However, specific antiretrovirals, such as tenofovir disoproxil fumarate (TDF) and ritonavir-boosted protease inhibitors, are associated with greater bone loss in individuals with HIV [3,11] and those without HIV receiving TDF combined with emtricitabine for preexposure prophylaxis [12], suggesting that direct effects of antiretrovirals may also impact bone cells or signaling between osteoblasts and osteoclasts.

Extracellular vesicles represent a heterogeneous population of nano and micro-sized vesicles, described as exosomes and microvesicles, and are released by most cell types, such as immune cells, osteoblasts, osteoclasts, osteocytes and bone marrow stem cells [13–16]. Extracellular vesicles have been isolated from numerous biological fluids including plasma [17], serum [18], urine [19], and cell culture medium [20]. They can transfer their cargo through endocytosis or fusion to recipient target cells, signaling via membrane proteins, microRNAs, mRNAs, and other growth factors that have emerged as novel mediators in bone metabolism and in the bone microenvironment [14,16,21–24]. The biodistribution of extracellular vesicles reflects the parent cell source, and circulating extracellular vesicles are efficiently internalized into different target cell types [25]. In addition, it is known that osteocalcin [26], CD34 [27], and M-CSF are expressed by osteoblast lineage cells [28], and that RANKL is expressed preferentially by immature osteoblasts [29]. Other studies also demonstrated the expression of RANKL by human B cells [9,30] and T cells [31]. RANK is expressed in fewer tissues than RANKL, but is also expressed by mature osteoclasts [32], dendritic cells, T cells [33], and some cancer cells [34]. Prior work has revealed that bone-derived extracellular vesicles contain specific osteogenic proteins, such as osteocalcin [35,36]. EVs also contain proteins related to osteoclast differentiation, such as RANK and RANKL [13,16]. Extracellular vesicles may provide a novel mechanism for intercellular communication in the bone remodeling microenvironment and may reflect the state of cells in the bone under healthy and pathologic conditions [21,37,38].

A recent study reported that osteoblast-derived extracellular vesicles contain RANKL and can stimulate osteoclast formation by signaling through the RANK-RANKL pathway [16]. Osteoprotegerin was also shown to inhibit extracellular vesicle-derived RANKL binding to RANK, preventing the RANK--RANKL interaction to regulate osteoclast activity [16]. Interestingly, another study performed by Li et al. [21] showed that in ovariectomized mice, miR-214-3p from osteoclast-derived exosomes inhibited osteoblast bone formation. Although the evidence supports bone-derived extracellular vesicles having the potential to influence osteoblast and osteoclast activity [22,24,38], the role of extracellular vesicles in osteoporosis and other bone metabolic disorders is not well defined.

Despite the interest in extracellular vesicles across many fields, little is known about the relationship of circulating extracellular vesicle cargo and their function in the bone-remodeling microenvironment. To investigate the relevance of extracellular vesicles both in communication between bone cells and as a potential biomarker of bone remodeling in HIV, we tested whether bone-related extracellular vesicle phenotypes changed after ART initiation and determined whether changes in levels of extracellular vesicles correlated with changes in BMD at 12 months.

Methods

Study population characteristics

The study population consisted of 15 ART-naïve male and female adults living with HIV who were about to start ART. Participants were recruited from the Comprehensive Health Program at Columbia University Irving Medical Center (CUIMC) for a prospective observational study of change in BMD and bone turnover markers with initiation of ART. Stored sera from this study were utilized for this extracellular vesicle substudy. Participants were considered ineligible if they had previously been diagnosed with an opportunistic infection, chronic kidney disease, malabsorption syndrome, neoplasia, hepatic impairment, or had history of treatment with bisphosphonates, glucocorticoids, or antiresorptive drugs. At enrollment, demographic information and clinical laboratory data including CD4+ T-cell count, HIV-1 RNA levels, medical history, osteoporosis risk factors, and current and past medication history were obtained.

Blood samples were collected at study entry before ART initiation and after 1, 3, 6 and 12 months on treatment. Of the 15 participants, 6 did not have serum samples available at every time point, so we averaged early time points (TP1, 1–3 months) and late time points (TP2, 6–12 months). BMD was assessed at baseline and month 12 by dual-energy X-ray absorptiometry (DXA). This study was approved by the Institutional Review Board of CUIMC, and all participants gave written informed consent.

Serum extracellular vesicle processing

At baseline and at 1, 3, 6, and 12 months after ART initiation, fasting morning blood samples were collected into marble-top tubes with clot activator and gel separator, processed, and the obtained serum stored at −80 °C until batch analyses. Fractionation of serum-extracellular vesicles was performed with 0.22 μm Ultrafree MC-GV Centrifugal Filter Units (Millipore) for 5 min at 860 g. Extracellular vesicles were recovered from the top of the filter by resuspension with phosphate-buffered saline as previously reported [39], and their relative size, absolute count, and markers from their cell of origin were determined.

Characterization of extracellular vesicle surface markers by flow cytometry

To determine extracellular vesicle quantity and expression of phenotypic markers, blinded serum samples were stained using pretitrated volumes of the following fluorochrome-conjugated monoclonal antibodies: osteocalcin (OC)-Alexa/488 (R&D Systems, Minneapolis, Minnesota, USA), RANK [(CD265) receptor activator of nuclear factor-kappa B-Alexa/700 (Novus Biologicals, Centennial, Colorado, USA)], RANKL [(CD254) RANK ligand-APC (BioLegend, San Diego, California, USA), M-CSF [(macrophage colony stimulating factor) – PE (R&D Systems)], and CD34-PE-Dazzle/594 (BioLegend). When panels were optimized, appropriate isotype-matched antibodies for each specific antibody were used as a negative control to assist with setting parameter gates. Prior to testing extracellular vesicle samples, each antibody was filtered using a 0.22 μm centrifugal filter, and the filtrate was used for staining. One to 5 μl of titrated monoclonal antibodies was added to 20 μl of extracellular vesicles and incubated at 4 °C for 30 min. To reduce background staining extracellular vesicles were centrifuged for 5 min at 860 g using 0.22 μm filters, and extracellular vesicles remaining on the filter surface were resuspended in 300 μl-buffered of 0.22 μm-filtered PBS containing 2.8% formaldehyde (BD stabilizing fixative).

Acquisition was performed on an LSRII flow cytometer (Becton Dickinson, Franklin Lakes, New Jersey, USA). Forward scatter (FSC) and side scatter (SSC) were set to the maximum voltages around of 500–600 and 300–400, respectively, to exclude the majority of the background instrument noise. Samples were acquired for 1 min at low sample pressure and flow rate (8–12 μl/min), and the collection of 10 000 events was attempted for each sample. The sensitivity of the flow cytometer to set a counting window was based on polystyrene beads. Gates were established using a blend of size-calibrated fluorescent beads sized from 0.1 μm (Invitrogen, Carlsbad, California, USA) to 1 μm (Megamix beads: 0.16, 0.2, 0.24 and 0.5 μm; and Spherotech 1 μm size) and used to set up SSC and FSC voltages for Extracellular vesicle analysis. TruCount tubes (BD Biosciences) containing a lyophilized pellet, which releases a known number of fluorescent beads, were used to measure the absolute counts of extracellular vesicles. Analysis was performed using FlowJo 10 software (Tree Star, Ashland, Oregon, USA).

Measurement of markers of bone turnover, inflammation and calciotropic hormones

Fasting morning serum samples were collected at baseline, and at 1, 3, 6, and 12 months after ART initiation, aliquoted, stored at −80 °C and batch-analyzed at the Irving Institute Biomarkers Core at CUIMC. Bone turnover markers were analyzed, including bone formation markers osteocalcin (OC; RIA, Immutopics, San Clemente, California, USA) and procollagen type I N-terminal propeptide (P1NP; RIA, Immunodiagnostic Systems, Gaithersburg, Maryland, USA), and the resorption marker C-telopeptide (CTx, ELISA; IDS). Additionally, we measured inflammatory markers interleukin (IL)-6 and tumor necrosis factor (TNF)-α by ELISA (ELISA; R&D Systems), and calciotropic markers, parathyroid hormone (PTH; RIA, Corning-Nichols Laboratory), total 25-hydroxyvitamin D (25-OHD, liquid chromatography tandem mass spectrometry), and 1,25-dihydroxyvitamin D (1,25-OHD; RIA, Diasorin). Except for 25-OHD, biomarkers were measured in duplicate and values averaged for analysis. CD4+ cell counts were measured by flow cytometry. HIV-1 RNA was quantified by a PCR using the Amplicor HIV-1 Monitor Ultrasensitive Test with a linear range of 50–100 000 copies/ml (Roche Diagnostics, Indianapolis, Indiana, USA).

Bone densitometry and body composition by dual energy X-ray absorptiometry

Areal BMD of the lumbar spine (L1--4), total hip, and femoral neck were measured at baseline and at 12 months on 14 participants by DXA utilizing a QDR 4500 bone densitometer (Discovery; Hologic Inc., Marlborough, Massachusetts, USA). BMD values are reported as g/cm2, Z-score and T-scores, and analyzed per the criteria established by the WHO. BMI was calculated as weight (kg) divided by height (m) squared. Total body and trunk fat were measured on a QDR 4500 bone densitometer.

Statistical analysis

Statistical analyses were performed using Prism 7.0 (GraphPad Software, San Diego, California, USA). Data were log10 transformed to address rightward skewing. The Shapiro--Wilk test was used to determine normality. Longitudinal data were analyzed by repeated measure analysis of variance (ANOVA) with the Greenhouse--Geisser correction and using Dunnett's Multiple Comparison post hoc test. Friedman repeated measures ANOVA with Dunn's Multiple Comparison post hoc test was used whenever variables were not normally distributed. Baseline and 12-month BMD data were compared using paired Student t tests. Spearman correlations were used to test associations between extracellular vesicle phenotypes in serum at each time point separately (baseline, early and late time points). All data are expressed as means ± standard deviation (SD), unless otherwise indicated. Values of P 0.05 or less were considered statistically significant. All P values are two-sided.

Results

Demographics and clinical course

Of 15 enrolled participants, 40% were men, 54% Hispanic and 40% Caucasian, with a mean age of 42.7 ± 11.4 years. The mean entry CD4+ T-cell count and HIV-1 RNA were 345 ± 168 cells/μl and 177 000 ± 234 000 copies/ml, respectively. Average duration from HIV diagnosis to enrollment into study and initiation of ART was 88.8 months. Of the 15 participants, nine initiated ART with a fixed dose of tenofovir disoproxil fumarate (TDF)/emtricitabine (FTC) in combination with efavirenz, four with TDF/FTC/rilpivirine, one with TDF/FTC/ ritonavir/darunavir, and one with TDF/FTC/raltegravir. Detailed demographic and baseline clinical characteristics are shown in Table 1. BMD declined significantly from baseline to 12 months in the lumbar spine (−2.6% ± 1.9), total hip (−4.3% ± 2.9) and femoral neck (−3.7% ± 3.6) after ART initiation (Fig. 1).

Table 1
Table 1:
Baseline characteristics of the study population.
Fig. 1
Fig. 1:
Significant change in bone mineral density at 12 months after antiretroviral therapy initiation.

Antiretroviral therapy initiation promotes an increase in serum and extracellular vesicle-derived osteocalcin

Polystyrene beads ranging from 100 to 1000 nm range were used to set extracellular vesicle-sizing gates. The gates were set just below the 100 nm bead signal up to the 1000 nm bead signal on the SSC channel (Fig. 2a). We examined if specific subsets of extracellular vesicles expressed markers that are related to bone metabolism (osteocalcin, RANK, RANKL, M-CSF and CD34) (Fig. 2b). There was minimal RANK--RANKL co-expression on individual extracellular vesicles. Not surprisingly, the lack of co-expression with either CD34 or M-CSF are consistent with extracellular vesicles expressing these markers being generated from separate cell types [40,41].

Fig. 2
Fig. 2:
Antiretroviral therapy initiation drives bone resorption and elicits a compensatory increase in serum and extracellular vesicle-derived bone formation.

Next we examined whether the concentration of total extracellular vesicles and bone related extracellular vesicles changed after ART initiation. There were no significant differences in total extracellular vesicle concentration between baseline, early and late time points (Fig. 2c). Levels of OC+EVs increased 130% from baseline to the early time point and 320% to the late time point (Fig. 2d). RANKL+EVs increased 110% from baseline to the late time point, although this change did not reach statistical significance (P = 0.08). There were no significant changes in levels of extracellular vesicles expressing RANKor CD34.

Serum osteocalcin levels increased 26% from baseline to the early time point and 68% from baseline to the late time point (Fig. 2e). P1NP levels increased 20% from baseline to the early time point and 95% from baseline to the late time point. CTx levels also increased 120% from baseline to the early time point and 175% from baseline to the late time point. The pro-inflammatory cytokine TNF-α decreased 47% after ART initiation, whereas there was no change in IL-6 levels. There was no significant change in serum PTH. These results show that both extracellular vesicle and soluble serum markers of bone metabolism changed after initiation of ART, with the largest fold-change seen in OC+EVs.

Correlation between extracellular vesicle phenotypes and bone turnover markers

We examined correlations between bone-related extracellular vesicle phenotypes and bone turnover markers at baseline and after initiation of ART. At baseline, serum bone formation and resorption markers were highly correlated, reflecting a coupled process of bone formation and resorption: osteocalcin and CTx (r = 0.84, P < 0.001), and P1NP and CTx (r = 0.79, P < 0.001). Bone formation and resorption markers remained highly correlated at the early time points [osteocalcin and CTx (r = 0.71, P = 0.004) and P1NP and CTx (r = 0.93, P < 0.001)] and late time points [osteocalcin and CTx (r = 0.71, P = 0.004), and P1NP and CTx (r = 0.69, P = 0.006)].

At baseline, there were no significant correlations between extracellular vesicle phenotypes, but after ART initiation, the correlations became significant. The correlation between RANKL+EVs and OC+EVs was significant at the early (r = 0.67, P = 0.01) and late time points (r = 0.64, P = 0.01, respectively). RANK+EVs and OC+EVs were also significantly correlated at the late time point (r = 0.58, P = 0.03). A strong relationship was found between M-CSF+EVs and RANKL+EVs at the early time point (r = 0.75, P = 0.002) and between M-CSF+EVs and CD34+EVs at the late time point (r = 0.90, P < 0.0001). Although correlations between extracellular vesicle phenotypes were not significant at every time point, the tightest association was found at the early time point post-ART initiation.

At baseline, OC+EV and RANKL+EV levels did not correlate with either serum osteocalcin or P1NP levels. Similarly, RANK+EV did not correlate with CTx. At the early time point, OC+EV levels did not correlate with any bone turnover markers, in spite of the fact that OC+EV and serum osteocalcin levels both rose after ART initiation. There was a negative correlation between RANKL+EV and serum osteocalcin (r = −0.71, P = 0.004), serum P1NP (−0.55, P = 0.04), and serum CTx (r = −0.71, P = 0.003). At the early time point, RANK+EV still did not correlate with CTx levels.

Early increases in levels of bone-related extracellular vesicles are associated with decreases in total hip bone mineral density after antiretroviral therapy initiation

We next examined whether changes in levels of bone-related extracellular vesicles correlated with changes in lumbar spine or hip BMD. Changes in level of serum bone turnover marker levels (osteocalcin, P1NP, CTx) did not correlate with changes in BMD after ART initiation. In contrast, decreases in TNF-α from baseline to the early time point correlated with decrease in lumbar spine BMD at 12 months (r = 0.67, P = 0.01).

We found negative correlations between change in OC+EVs, RANKL+EVs, RANK+EVs, and CD34+EVs from baseline to the early time point and change in total hip BMD from baseline to 12 months (Fig. 3a). These data suggest that increases in bone-related extracellular vesicle phenotypes are associated with decreases in total hip BMD. The correlations between bone-related extracellular vesicles and BMD at the lumbar spine and femoral neck did not reach significance, although the direction of association was the same (data not shown). Total hip BMD loss at 12 months was also associated with increase in CD34+EVs from baseline to the late time point, and increases in M-CSF+EV levels from baseline to the late time point were associated with decreases in femoral neck BMD (Fig. 3b). In summary, increases in levels of several different bone-related extracellular vesicle markers were associated with decreases in BMD, whereas none of the classic soluble markers of bone turnover correlated with degree of bone loss.

Fig. 3
Fig. 3:
Early changes in levels of bone-derived extracellular vesicles are associated with the magnitude of change in total hip at 12 months.

Discussion

To the best of our knowledge, this study provides the first evidence that early increases in levels of serum bone-related extracellular vesicles are associated with decreases in BMD associated with ART initiation in people living with HIV (PLWH). The mechanism by which HIV and ART leads to alterations in the immune-skeletal interface remains uncertain, despite well designed studies with bone turnover markers and immune parameters. Future studies including extracellular vesicle phenotypes may help to clarify signaling mechanisms driving bone loss with ART initiation, or find that certain extracellular vesicle phenotypes can be utilized as biomarkers that can help to predict, which individuals are at the highest risk of bone loss or fracture with ART.

Definitive markers for osteoblast-derived extracellular vesicles and osteoclast-derived extracellular vesicles have not been established. In-vitro studies of osteoblast cell lines have shown that extracellular vesicles shed from osteoblasts have RANKL on their surface [13], as well as other proteins, such as bone sialoprotein, osteocalcin, osteopontin, and osteonectin [35]. In-vitro studies of osteoclast cell lines demonstrate that extracellular vesicles released from osteoclasts have RANK [13] as well as other proteins, such as ephirin A2 [22], tartrate-resistant acid phosphatase (TRAcP5), and sema4D [21]. Osteoclast-derived extracellular vesicles also carry various microRNAs (miRNAs), which have been shown to be able to regulate gene expression target cells after the extracellular vesicles fuse with target cellular membranes, allowing miRNAs to be internalized and bind to mRNAs. Several miRNAs have been identified as relevant for osteoclast and osteoblast regulation [21,36,42–45].

Very few studies have characterized extracellular vesicles using clinical specimens. In a study of exosomes from sera of elderly individuals with and without osteoporosis, Xie et al.[24] identified between-group differences in candidate proteins using a proteomic approach, but did not identify RANKL, RANK and osteoclasts in their extracellular vesicle proteomic analyses. Given the lack of extracellular vesicle data from clinical specimens, we characterized RANKL+EV and OC+EVs as osteoblast-derived extracellular vesicles, and RANK+EVs as osteoclast-derived extracellular vesicles based upon existing in-vitro studies. Before ART initiation, there were no significant correlations between extracellular vesicles and bone turnover markers. At the early time point after ART initiation, RANKL+EVs, a putative osteoblast-derived extracellular vesicle, had a negative correlation with both bone formation and resorption markers; whereas, correlations between the other osteoblast-derived extracellular vesicle (OC+EV) and the putative osteoclast-derived EV (RANK+EV) and respective bone formation and resorption markers remained not significant.

As extracellular vesicles reflect the function of parent cells [16,23], an inverse relationship between RANKL+EV and serum OC and P1NP at the early time point was unexpected. Similarly, if RANKL+EVs were capable of inducing osteoclastogenesis and osteoclastic resorption, we would have expected to find a positive correlation between RANKL+EV and CTx levels. In contrast to bone turnover marker data, increases in the osteoblast-derived EVs (OC+EVs and RANKL+EVs) and osteoclast-derived EVs (RANK+EVs) correlated with decreases in total hip BMD. Our data are consistent with an in-vitro study in which RANKL-containing extracellular vesicles derived from osteoblasts stimulate osteoclast formation [16]. Our data show that OC+EVs and RANKL+ EVs increase after ART initiation, but that RANK+ EVs do not increase. Given that RANK+ EVs secreted by activated osteoclasts can stimulate osteoblast function through inside-out signaling [46], the relative imbalance between RANKL and RANK-expressing extracellular vesicles could cause greater activation of osteoclasts than osteoblasts, resulting in net bone resorption (Fig. 4).

Fig. 4
Fig. 4:
Proposed model for effect of changes in levels of extracellular vesicle-derived bone markers after antiretroviral therapy initiation.

Similar to our study, others have also found that BMD decreases within 12 months after initiating ART [1–3], with significant upregulation in osteoclastic bone resorption measured by serum CTx [10]. We and others found that ART initiation was associated with decreased TNF-α levels [47–49]. Although some studies have found that IL-6 decreases after ART initiation [50,51], these findings are not consistent among different studies [52,53]. However, we observed that decreasing levels of serum TNF-α after ART initiation were associated with decreased lumbar spine BMD.

Although provocative, our current study has several limitations. The relatively small sample size of PLWH reduced our power to detect other potentially relevant associations, and not all samples were available at each time point. Of 15 participants, four were at least 50 years old and postmenopausal. We did not investigate whether extracellular vesicles expressing other markers, such as osteoprotegerin (OPG) or immune activation markers, might be shed into the circulation and also predict the bone loss. We did not measure the concentration of soluble RANK, RANKL and OPG, which might have detected a relationship with changes in BMD when the classical bone turnover markers did not. Of note, we did not measure the phenotype of extracellular vesicles less than 200 nm in size because of technical limitations of flow cytometry. It is possible that exploration of smaller extracellular vesicles using alternative techniques would reveal information that would complement the current study.

Future studies are required to understand the cell of origin for extracellular vesicles expressing markers of bone activity, and the precise mechanism of effect on bone cells in PLWH on ART treatment. It will be of interest to extend our findings with a prospective longitudinal study determining whether the bone extracellular vesicle markers identified as well as other extracellular vesicle phenotypes are predictive of changes in BMD, and to perform in-vitro or in-vivo experiments to determine if ART affects the balance between RANK and RANKL expressing extracellular vesicles. Our observations suggest that extracellular vesicles may serve as novel serum biomarkers for measuring bone remodeling and potentially be a better candidate predictor for HIV-related bone loss than classic bone turnover markers. Elucidating the role of extracellular vesicles in bone metabolism related to HIV infection could lay the foundation for novel strategies to diagnose and treat abnormalities in bone homeostasis in HIV and other disease process.

Acknowledgements

E.G.M.M. designed and performed experiments, analyzed data, and wrote the manuscript, J.R. analyzed data, M.B. provided clinical samples and edited the manuscript, E.S. provided clinical samples and edited the manuscript, M.T.Y. designed experiments, provided clinical samples, and edited the manuscript, P.J.N. designed experiments and edited the manuscript. This work was supported by RO1 AI1065200 (E.S.); K23 AI059884 (M.T.Y.).

E.G.M.M. would like to thank the Sao Paulo Research Foundation (FAPESP) for the support provided for grant #2015/12965-6.

Funding sources: NIH RO1 AI1065200 (E.S.); K23 AI059884 (M.T.Y.); Sao Paulo Research Foundation (FAPESP) for the support provided for grant #2015/12965-6 (E.G.M.M.).

Conflicts of interest

There are no conflicts of interests.

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Keywords:

antiretroviral therapy; bone mineral density; bone remodeling; extracellular vesicles; HIV; osteocalcin; receptor activator of NF-kB ligand

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