Vascular calcification (VC) is the process of deposition of calcium phosphate crystals in the blood vessel wall, with a central role for vascular smooth muscle cells (VSMCs). VC is highly prevalent in chronic kidney disease (CKD) patients and thought, in part, to be induced by phosphate imbalance. The molecular mechanisms that regulate VC are not fully known. Here we propose a novel role for the mineralisation regulator Ucma/GRP (Upper zone of growth plate and Cartilage Matrix Associated protein/Gla Rich Protein) in phosphate-induced VSMC calcification. We show that Ucma/GRP is present in calcified atherosclerotic plaques and highly expressed in calcifying VSMCs in vitro. VSMCs from Ucma/GRP−/− mice showed increased mineralisation and expression of osteo/chondrogenic markers (BMP-2, Runx2, β-catenin, p-SMAD1/5/8, ALP, OCN), and decreased expression of mineralisation inhibitor MGP, suggesting that Ucma/GRP is an inhibitor of mineralisation. Using BMP signalling inhibitor noggin and SMAD1/5/8 signalling inhibitor dorsomorphin we showed that Ucma/GRP is involved in inhibiting the BMP-2-SMAD1/5/8 osteo/chondrogenic signalling pathway in VSMCs treated with elevated phosphate concentrations. Additionally, we showed for the first time evidence of a direct interaction between Ucma/GRP and BMP-2. These results demonstrate an important role of Ucma/GRP in regulating osteo/chondrogenic differentiation and phosphate-induced mineralisation of VSMCs.
Vascular calcification (VC) is a process of deposition of calcium phosphate crystals in the form of hydroxyapatite in the intima and media of the vessel wall1,2. The presence of VC reduces arterial wall elasticity and alters the hemodynamic profile, increasing the risk of cardiovascular events. VC is an independent risk factor predicting cardiovascular mortality and frequently measured as marker of atherosclerotic burden3. Nearly all patients suffering from cardiovascular disease have some degree of calcification, and in asymptomatic patients prevalence of coronary calcification corresponds with age. Amongst cardiovascular disease patients, approximately 60% of over 60-year-olds suffer from VC3,4. Chronic kidney disease (CKD) patients are known to be especially prone to VC. Mineral homeostasis dysregulation, uremic toxins and warfarin treatment are known to contribute to VC in dialysis patients5,6. Elevated phosphate in blood is thought to be one of the main inducers of VC in CKD7,8.
VC is an active process regulated by vascular smooth muscle cells (VSMCs). In response to cellular stress VSMCs undergo VC via several mechanisms: apoptosis, release of extracellular vesicles, loss of calcification inhibitors such as matrix Gla protein MGP; reviewed in Schurgers et al.9, ageing-related DNA damage and osteo/chondrogenic differentiation10,11.
In physiological conditions VSMCs exist in the vessel wall as contractile cells and regulate vascular tone. However, VSMCs are known to have a high degree of phenotypic plasticity12. In response to stress and injury, VSMCs lose expression of contractility-related genes such as SM22α, calponin (CNN1), and myosin light chain (MLC)13,14,15,16. When vascular injury is persistent, the phenotypic transition is dysregulated and VSMCs can undergo an unfavourable transdifferentiation into cells with characteristics of osteoblasts or chondrocytes4,12,17,18,19,20. This is termed osteo/chondrogenic differentiation. Many bone mineralisation-regulating proteins were found to be expressed in the calcifying blood vessel, such as BMP-2 Runx2, MGP, osteocalcin (OCN), osteopontin (OPN)18,21,22 amongst others and have been shown to play an active part in regulating VC. Additionally, calcifying VSMCs have been shown to release extracellular vesicles in a mechanism similar to release of matrix vesicles from chondrocytes23. However, the exact molecular mechanisms regulating VSMC osteo/chondrogenic transdifferentiation are unknown.
Ucma (Upper zone of growth plate and Cartilage Matrix Associated protein; also known as Gla Rich Protein - GRP) is a novel mineralisation inhibitor, which was first reported in cartilage24,25 and later in the vasculature26,27. Ucma/GRP-deficient mice did not develop a clear phenotype28, however in vitro studies revealed that Ucma/GRP regulates differentiation of chondrocytes and osteoblasts29,30,31. Using immunohistochemistry, Ucma/GRP was shown to be present at sites of VC. Moreover, when added exogenously, Ucma/GRP inhibited calcification of aortic rings in vitro26,27,29.
Based on the involvement of Ucma/GRP in differentiation of osteoblasts and its role in VC, we hypothesized that Ucma/GRP is involved in osteo/chondrogenic differentiation of VSMCs. To test our hypothesis we examined expression of Ucma/GRP during phosphate-induced calcification of VSMCs. We also examined osteo/chondrogenic gene expression and calcification of Ucma/GRP−/− VSMCs exposed to elevated levels of inorganic phosphate. Our findings indicate that Ucma/GRP reduces VC by inhibiting osteo/chondrogenic VSMC transdifferentiation through a BMP-2-regulated pathway.
Treatment of VSMCs in vitro with phosphate induces calcification
We first set out to examine calcification of primary mouse VSMCs in vitro. WT VSMCs were cultured in medium with elevated phosphate as described before8,32 (osteogenic medium, OM), which induced mineralisation in vitro, as observed by quantification of deposited calcium phosphate crystals (Fig. 1A). To control for spontaneous mineral precipitation on collagen, collagen-coated wells were incubated with OM in the absence of VSMCs. Under these a-cellular conditions, no calcification was observed (data not shown). To examine osteo/chondrogenic differentiation in mineralisation of VSMCs in vitro, Runx2 and Osteocalcin expression was measured using qPCR after 12 days of incubation with osteogenic medium (Fig. 1B and C). Expression of both markers was significantly increased, suggesting that the observed mineralisation is an active process involving osteo/chondrogenic differentiation. Moreover, treatment of human VSMC with osteogenic medium increased secretion of extracellular vesicles (Fig. 1D), which have recently been shown to mediate VC23.
Ucma/GRP is expressed in atherosclerotic plaques of ApoE−/− mice
Ucma/GRP has previously been shown to be expressed in calcified human aortas and aortic valves27. Here we demonstrated that Ucma/GRP is expressed in advanced atherosclerotic lesions of ApoE−/− mice. UcmaGRP was expressed specifically in atherosclerotic plaques (Fig. 2A and B) in cells which show similarities to chondrocyte morphology. As shown in Fig. 2C and D, these cells also expressed osteo/chondrogenic markers BMP-2 and Runx2. This suggests that Ucma/GRP is involved in osteo/chondrogenic differentiation and calcification of VSMCs in atherosclerotic plaques. Interestingly, not all cells with chondrocyte-like morphology visibly expressed Ucma/GRP.
Ucma/GRP expression in VSMCs in vitro increases in response to osteogenic medium
The presence of Ucma/GRP in murine VSMCs (mVSMCs) in vitro was confirmed using RT-PCR (Fig. 3A). Additionally, immunocytochemistry (Fig. 3B) has shown expression of Ucma/GRP in scattered cytoplasmic foci, which is consistent with its subcellular localization in other cell types31. Next, in order to examine whether Ucma/GRP has a role in mineralisation of VSMCs in vitro, expression was measured in response to treatment with osteogenic medium (Fig. 3C). Ucma/GRP expression, measured by qPCR, increased in a time-dependent manner with a 20-fold increase after 12 days of culture. Immunocytochemistry analysis confirmed this result and showed that control medium does not induce a similar increase (Fig. 3D).
Ucma/GRP-deficient VSMCs are more prone to calcification in response to osteogenic medium
Aortas were harvested from Ucma/GRP−/− mice (KO) and wild type (WT) counterparts generated as previously described28. The knock-out of Ucma/GRP was confirmed by immunohistochemical staining of the epiphyseal plate (Supplemental Fig. 1A). VSMCs were isolated and their identity was verified by immmunocytochemical staining for VSMC markers (αSMA, CNN1, p-MLC) (Supplemental Fig. 1B). We and others26,27 have shown that Ucma/GRP is upregulated in response to calcification and that its expression is confined to osteo/chondrogenic cells in atherosclerotic plaques (Figs 2A and 3A,B). Therefore, we hypothesized that Ucma/GRP is involved in controlling osteo/chondrogenic differentiation of VSMCs and consequently calcification. To test this, WT and Ucma/GRP−/− VSMCs were incubated in osteogenic medium over a time span of 15 days (Fig. 4A and B). Both WT and Ucma/GRP−/− VSMCs calcified in response to osteogenic medium, with calcification becoming detectable after 6 days. However, Ucma/GRP−/− VSMCs calcified approximately twice as much as WT cells after 9, 12 and 15 days. Neither Ucma/GRP−/− nor WT VSMCs calcified in control medium (Supplemental Fig. 1C). Ucma/GRP knock-down in WT cells using siRNA resulted in significantly increased calcification compared to cells transfected with a scramble control (Supplemental Fig. 1D), confirming that the observed effects are specific to Ucma/GRP. In response to osteogenic medium alkaline phosphatase (ALP) activity was increased in Ucma/GRP−/− cells but not in WT cells, suggesting increased osteo/chondrogenic potential of Ucma/GRP−/− cells (Fig. 4C).
Ucma/GRP deficiency results in increased osteo/chondrogenic gene expression
Since osteo/chondrogenic differentiation is an important mechanism regulating VC and expression of osteo/chondrogenic markers is found in atherosclerotic plaques, we set out to examine whether there were any differences in osteo/chondrogenic marker expression between WT and Ucma/GRP−/− VSMCs. We observed that Ucma/GRP−/− cells expressed increased levels of BMP-2 mRNA in baseline conditions (CM, Fig. 5A). Additionally, when challenged with osteogenic medium, Ucma/GRP−/− VSMCs expressed higher levels of OPN, Osteocalcin and BMP-2, compared to WT VSMCs (Fig. 5A,B and C). MGP mRNA expression was significantly downregulated in Ucma/GRP−/− compared to WT VSMCs, both in baseline and osteogenic conditions, in line with the increased calcification potential of these cells (Fig. 5D). Upon treatment with osteogenic medium MGP expression increased, both in WT and Ucma/GRP−/− VSMCs. Western blot analysis demonstrated an increase in β-catenin and phosphorylated SMAD1/5/8 expression, suggesting the involvement of SMAD signalling pathways (Fig. 5E,F,G) known to be involved in osteoblast mineralization and VC. Additionally, expression of Runx2 and ALP was higher in Ucma/GRP−/− cells compared to WT (Fig. 5E,H and I). Importantly, we also observed that Ucma/GRP−/− VSMCs displayed reduced expression levels of contractile phenotype marker αSMA compared to WT VSMCs (Supplemental Fig. 1E). Taken together these results show that Ucma/GRP−/− VSMCs undergo increased osteo/chondrogenic differentiation, compared to WT VSMCs, both at baseline as well as in osteogenic conditions.
The osteo/chondrogenic phenotype in Ucma/GRP−/− VSMCs is induced by lack of inhibition of a BMP-2/4-p-SMAD1/5/8-β-catenin dependent-pathway
BMP-2 is a key modulator in the development of VC19,21. Since we observed an increase in BMP-2 expression and its downstream targets p-SMAD1/5/8, we investigated the involvement of BMP signalling in calcification of Ucma/GRP−/− VSMCs. We blocked BMP-2 and BMP-4 signalling using noggin and treated VSMCs with osteogenic medium (Fig. 6A). Noggin treatment decreased calcification of both WT and Ucma/GRP−/− VSMCs. Additionally, to investigate whether there is an interaction between BMP-2/4 and Ucma/GRP we carried out co-immunoprecipitation using media from hVSMCs treated with BMP-2. BMP-2/4-containing protein complexes were captured with a BMP-2/4 antibody and analysed using western blotting for Ucma/GRP. The results show clearly the presence of Ucma/GRP (Fig. 6B), strongly pointing to a functional BMP-2/4-Ucma/GRP interaction. To examine whether there is a direct interaction with BMP-2, we carried out solid phase binding assays by coating ELISA plates with carboxylated Ucma/GRP (cUcma), uncarboxylated (ucUcma), BMP-2 and MGP (positive control) and incubating with BMP-2 in the liquid phase. Detection of BMP-2 with an anti-BMP-2/4 antibody showed that BMP-2 bound to Ucma/GRP, specifically to the carboxylated Ucma/GRP form (Supplemental Fig. 2A).
Further to that, to investigate the involvement of specific downstream targets of BMP-2 we treated cells with dorsomorphin, an inhibitor of SMAD1/5/8 activation (AMPK inhibitor). Dorsomorphin decreased calcification of WT VSMCS and restored levels of calcification in Ucma/GRP−/− cells to the levels observed in WT VSMCs (Fig. 6C). The reduction in calcification was reflected by a decrease in p-SMAD1/5/8 and ALP expression (Fig. 6D,E,F). Taken together, these results suggest that increased osteo/chondrogenic and calcification potential of Ucma/GRP−/− VSMCs is due to impaired inhibition of SMAD-dependent BMP signalling.
As Erk signalling has been known to also activate SMAD signalling33, we investigated whether inhibiting Erk phosphorylation has an effect on calcification of Ucma/GRP−/− VSMCs. Treatment of WT and Ucma/GRP−/− VSMCs with Erk phosphorylation inhibitor U0126 did not change calcification levels of cells of either genotype, suggesting that Erk phosphorylation and Ucma/GRP are not interacting to inhibit calcification of VSMC cultures (Supplemental Fig. 2B).
VC is an important predictor of cardiovascular mortality. In particular, CKD patients have been shown to be at an increased risk of VC5,34. However, the mechanisms through which VC develops remain incompletely understood. In the present study we demonstrate that Ucma/GRP plays a role in the attenuation of osteo/chondrogenic differentiation of VSMCs through a pathway involving SMAD-dependent BMP signalling. Osteo/chondrogenic switching is accelerated in the absence of Ucma/GRP and this results in enhanced calcification. We also provide evidence that high phosphate concentrations, which is a common finding in CKD patients7, induce upregulation of Ucma/GRP in VSMCs. Our findings reveal a novel pathway through which Ucma/GRP inhibits phosphate-induced SMAD signalling and osteo/chondrogenic differentiation, thereby reducing the propensity for calcification of the vessel wall.
Ucma/GRP was previously shown to inhibit maturation of chondrocytes towards hypertrophic cells and osteogenic differentiation of osteoblasts29. Ucma/GRP is known to be present in low levels in calcified aortic valves and in the media. Ucma/GRP inhibits calcification of aortic rings cultured in calcifying medium, when added exogenously to cultures, this was accompanied by an increase in αSMA expression and a decrease of osteopontin expression27. In our study we confirmed the presence of Ucma/GRP in the vasculature and for the first time reveal that Ucma/GRP expression is markedly increased in osteo/chondrogenic cells in atherosclerotic plaques of ApoE−/− mice, which implicates its role in this vascular pathology. CKD patients show accelerated atherosclerosis, which suggests that our in vivo findings are relevant for calcification in CKD-related atherosclerosis35,36.
BMP-2 is a potent inducer of calcification and regulator of osteo/chondrogenic differentiation of VSMCs, known to cause phosphate influx into cells21. BMP-2 acts by binding its cell surface receptors which transduce the signal to the cytoplasm by phosphorylating pathway-restricted SMADs (SMAD1 and SMAD5) for BMPs37. This leads to heterodimerization of pathway-restricted SMADs with SMAD4, a common-mediator SMAD, and translocation of the complex to the nucleus, where it binds directly to DNA38. As a result, changes in gene expression occur, such as upregulation of Runx2, OCN and ALP. Additionally, BMP-2 has been shown to induce accumulation of β-catenin39. β-catenin has been demonstrated to activate Runx2 expression in the context of phosphate-induced VSMC calcification40. BMP and Wnt pathways have been shown to be co-activated in calcifying VSMCs41, where SMAD1 and β-catenin interacted and regulated gene expression together. Additionally, dorsomorphin homologue 1 has been recently shown to inhibit phosphate-induced osteogenic differentiation of hVSMCs by inhibiting BMP-242. Our data are in line with these findings, as we demonstrate increased SMAD1/5/8 phosphorylation and expression of β-catenin, Runx2 and their downstream targets ALP, OCN and OPN in phosphate-treated Ucma/GRP−/− VSMCs. Here we demonstrate for the first time that Ucma/GRP interacts with this BMP-SMAD signalling pathway by binding BMP-2 and that inhibiting BMP-2/-4 signalling with noggin and SMAD1/5/8 phosphorylation with dorsomorphin decreased calcification of VSMCs and osteo/chondrogenic gene expression. Interestingly, previous reports show that externally added BMP-2 decreased Ucma/GRP expression in chondrocytes29, suggesting an interaction between BMP-2 signalling and Ucma/GRP. In addition to that, in osteoblasts Ucma/GRP is under direct transcriptional control of Runx2 and Osterix30, however this has not been investigated in VSMCs.
In our study we confirm that high levels of phosphate induce hallmarks of osteogenic differentiation in VSMCs, such as osteo/chondrogenic gene expression and extracellular vesicle release, and that Ucma/GRP expression is increased in VSMCs treated with osteogenic medium in vitro. This, together with the presence of Ucma/GRP in advanced atherosclerotic lesions, suggests that calcifying cells increase the expression of this inhibitor in a bid to protect themselves from adverse phenotype changes. This has been shown to happen with MGP, another vitamin K-dependent calcification inhibitor, by us in the present study and others43. Additionally, insufficient carboxylation of MGP due to warfarin administration is one of the factors contributing to VC in CKD44. Uncarboxylated Ucma/GRP, similar to uncarboxylated MGP, could contribute to these processes. Ucma/GRP is a vitamin K-dependent protein, as it undergoes posttranslational carboxylation45. It has been previously shown that uncarboxylated Ucma/GRP accumulates at sites of pathological calcification in human aortic valves and media and only the carboxylated form of Ucma/GRP was able to inhibit calcification27. Our results are in line with this, as we show that carboxylated Ucma/GRP has high affinity to BMP-2, whereas uncarboxylated Ucma/GRP binds BMP-2 only weakly. However, we have not investigated the carboxylation status of Ucma/GRP in the atherosclerotic plaques which we examined and this warrants further investigation.
MGP is known to inhibit VC by binding mineral and interacting with BMP-2, preventing it from binding its receptor7,9,23. It is therefore tempting to speculate that vitamin K-dependent inhibitors complement each other with respect to regulating VC: calcium-induced calcification is regulated by MGP and whereas phosphate-induced calcification is regulated by Ucma/GRP. This is further supported by previous studies showing that phosphate increases osteo/chondrogenic differentiation of VSMC in vitro, whereas this was not demonstrated for calcium yet8,12,46.
Based on our observations, we propose a model of how Ucma/GRP inhibits VC (Fig. 7). When VSMCs are exposed to elevated phosphate concentrations in the extracellular environment, as is the case in CKD patients, osteo/chondrogenic differentiation (as evidenced by increased Runx2, β-catenin, osteocalcin, osteopontin and ALP expression) is initiated via increased BMP-2-SMAD signalling. We propose that Ucma/GRP can ameliorate the effect of increased phosphate by inhibiting this signalling pathway and thus reduce calcification of the vessel wall.
Taken together, we demonstrate that Ucma/GRP, a member of a range of inherent calcification inhibitors present in the vasculature47, plays an important role in regulating osteo/chondrogenic differentiation of VSMCs. Our findings have implications for vascular pathologies which lead to VC and represent an advancement in our knowledge about the steps resulting in VC. One of the main goals in the treatment of patients with CKD is to reduce the substantially increased risk of cardiovascular comorbidity and mortality, improving both quality and length of life. The increase in CKD stage and cardiovascular risk is accompanied by increased phosphate levels. As shown by our results, the phosphate-Ucma/GRP-BMP axis holds promise for novel interventions. Pharmacological manipulation of Ucma/GRP levels could represent a novel therapeutic strategy to prevent VC.
Ucma/GRP−/− C57BL\6 mice were generated and kindly provided by Dr. M. Stock, University of Erlangen, Germany, with the approval of the local ethics authorities (University of Erlangen-Nuremberg and the Government of Mittelfranken, Ansbach, Germany) and according to the regulations of the animal facilities in Germany28. Mice were maintained in a specific pathogen-free environment with free access to water and western type diet (Arie Block, Woerden, the Netherlands) and sacrificed by portal vein puncture after 12 weeks. Aortas were harvested for immunohistochemistry and VSMC isolation.
Aortic sections of atherosclerotic ApoE−/− mice from a previous study were used48. Sequential 4 µm paraffin sections were cut from the aortic arch and used for immunohistochemical staining as previously described48. The following antibodies were used: anti- BMP-2 (Santa Cruz, sc-6895), anti-Runx2 (M70, Santa Cruz, sc-10758) anti-total Ucma/GRP antibody (Cterm-GRP, GenoGla Diagnostics, Faro, Portugal), HRP conjugated secondary antibodies and DAB or Nova-RED substrate (Vector Labs, Amsterdam, the Netherlands). Sections were counterstained with haematoxylin (Klinipath, Duiven, the Netherlands) and mounted in entellan (Merck, Amsterdam, the Netherlands).
VSMC isolation and culture
Endothelium and adventitia were removed from aortas of Ucma/GRP−/− and WT littermates. Tissue was dissected into ± 5 mm² pieces and digested with 3 mg/ml collagenase (Sigma, Zwijndrecht, the Netherlands) and 1 mg/ml elastase (Sigma) for 4 hours at 37 °C in DMEM (Gibco, Bleiswijk, the Netherlands). The cells were washed, resuspended in growth medium (DMEM with 10% FCS, Gibco, 100 U/ml penicillin and 100 mg/ml streptomycin, Gibco) and transferred to culture dishes. Success of the isolation was determined by immunofluorescent staining for αSMA, SM22α, phosphorylated myosin light chain 2 (method below) and western blotting for αSMA. Cells at passage 4–12 were used for experiments. Cells were maintained in culture medium and passaged when 90% confluent. Cell cultures were not supplemented with additional vitamin K. The following inhibitors were added to media for treatments: 2 µM of U0126 (Merck, Amsterdam, the Netherlands), 100 ng/ml noggin (R&D systems, Abingdon, United Kingdom), 2 µM dorsomorphin dihydrochloride (sc-361173, Santa Cruz). All inhibitors were added to cells for the full duration of the experiment, as indicated in figure legends. Medium was refreshed every 2–3 days.
Human primary VSMCs (hVSMCs) were used for exosome quantification assay and co-immunoprecipitation. They were maintained in M199 with 20% FCS, 100 U/ml penicillin and 100 mg/ml streptomycin (Gibco).
Cells were fixed with 4% PFA, permeablilised with 0.1% Triton X-100, blocked in 1% BSA/PBS and incubated with primary antibodies (Calponin, Abcam, ab46794; αSMA,Sigma; phosphorylated myosin light chain 2, Cell Signalling, 3675S and anti-total Ucma/GRP antibody (Cterm-GRP, GenoGla Diagnostics, Faro, Portugal). The following secondary antibodies were used: anti-rabbit-FITC (Dako, F0205) and anti-mouse-FITC (Dako, F0232). Nuclei were stained with DAPI (Sigma–Aldrich). Cells were mounted in a glycerol DABCO mounting medium. Pictures were taken with a Leica DM2000 widefield microscope (Leica Microsystems).
4 × 104 cells were seeded per well of a 12-well plate. After 24 hours medium was changed to osteogenic medium (growth medium +2.6 mM PO43−, OM) or growth medium (control medium, CM). Quantification of deposited calcium was carried out using a calcium determination kit (Randox, London, United Kingdom) according to the manufacturer’s instruction, after solubilising mineral deposits in 0.1 M HCl. Calcium measurements were normalised to protein content using micro BCA assay (Thermo Scientific, Bleiswijk, the Netherlands). Calcification was additionally visualised using Alizarin Red S staining adapted from Gregory et al.49.
RNA isolation and quantitative real-time PCR
Total RNA was isolated using TRI Reagent (Sigma). RNA concentration and quality were determined using a Nanodrop 2000 spectrophotometer (Thermo Scientific, Bleiswijk, the Netherlands) and agarose-denaturing gel electrophoresis. 1 µg of total RNA was treated with DNAse I (Promega, Leiden, the Netherlands) and reverse transcribed using M-MLV reverse transcriptase (Invitrogen, Bleiswijk, the Netherlands), an oligo dT adapter (Eurogentec, Maastricht, the Netherlands) and RNAse Out (Invitrogen, Bleiswijk, the Netherlands). Real-time qPCR was performed using the Quantitect SYBR green PCR kit (Qiagen, Venlo, the Netherlands) in a LightCycler 480 II (Roche, Woerden, the Netherlands) with 50 ng of cDNA and 0.5 µM of each primer. The following primers were used BMP-2 (F) GTG-CTT-CTT-AGA-CGG-ACT-GCG-GTC-TCC-TA, BMP-2 (R) GCC-TGA-GTG-CCT-GCG-GTA-CAG-ATC-TAG, Runx2 (F) GAC-GAG-GCA-AGA-GTT-TCA-CC, Runx2 (R) GGA-CCG-TCC-ACT-GTC-ACT-TT, HPRT1 (F) AGC-CAA-ATA-CAA-AGC-CTA-AGA-TGA-GCG, HPRT1 (R) GAA-ATG-TCA-GTT-GCT-GCG-TCC-CCA-GA, MGP (F) ACA-CAG-AGG-CAG-ACT-CAC-AGG-ACA-CCC, MGP (R) CTG-AGG-GGA-CAT-AAA-GGT-GTT-GGC-AT, OCN (F) AAG-CAG-GAG-GGC-AAT-AAG-GT, OCN (R) TTT-GTA-GGC-GGT-CTT-CAA-GC, OPN (F) TGA-CCA-CAT-GGA-CGA-CGA-TGA-TGA-CGA-TGA, OPN (R) GGG-ACG-ATT-GGA-GTG-AAA-GTG-TCT-GCT-TGT. Fluorescence curves were analyzed with LightCycler 480 Software (Version 1.5) and relative quantification was performed with the 2−ΔΔCt method. Ucma/GRP was detected as described previously45. All samples were assayed in triplicate.
Quantification of exosome release
Exosomes were quantified using a bead-capture assay as described before23. Briefly, anti-human CD63 antibody (556019, BD Bioscience) was immobilized on aldehyde-sulfate functionalized beads (Invitrogen). Human primary VSMC culture media was incubated with anti-CD63-coated beads on a shaker overnight at 4 °C. VSMCs were stained with Hoechst 33342 (Thermo Fisher) and counted using a Cytation 3 live-cell imager. Beads were washed and incubated with anti-CD81-PE antibodies for 1 h at room temperature. Then beads were washed with PBS with 2% BSA and analyzed by flow cytometry (Accuri C6, BD). Arbitrary units (AU) were calculated as mean fluorescence units times percentage of positive beads and normalized to the number of cells.
VSMCs were lysed in 0.1 M Tris pH 8.1, 0.15 M NaCl, 1% triton x-100 0.2 mM NaVO3 and 1:50 protease inhibitor cocktail (Sigma). Protein concentrations were determined using DC protein assay (Bio-Rad, Veenendaal, the Netherlands) and lysates were separated on Any kD Mini-PROTEAN TGX Precast Protein Gels (BioRad). Samples were transferred to a PVDF or nitrocellulose membrane (BioRad) and incubated overnight with anti-αSMA (A2547, Sigma), anti-calponin (ab46794, Abcam), anti-ALP (R&D Systems, AF290), anti-Runx2 (MBL, D130-3), anti-β-catenin (BD, 610153), anti-p-SMAD1/5/8 (Cell Signalling, 12820P) and α-tubulin (Sigma, T6074) antibodies. Protein was then detected using HRP-conjugated secondary antibodies (anti-mouse: p0447, Dako; anti-rabbit: 7074S, Cell Signalling, anti-goat: P0449, Dako) and visualized by enhanced chemiluminescence (Pierce ECL Western Blotting Substrate, ThermoFisher Scientific).
Co-IP assays were performed using conditioned media from hVSMCs cultured in the presence of 500 ng/ml of recombinant BMP-2 (Preprotech) for 24 h in M199 with 10% FBS, and the Dynabeads Co-immunoprecipitation Kit (Novex, Life Technologies), according to manufacturer’s recommendations. The BMP-2/4 monoclonal (Santa Cruz Biotechnology, sc-137087) and negative IgG antibodies were used as capture antibodies in the Co-IP reactions, and Western blot analysis of the eluted proteins were performed using CTerm-Ucma/GRP (GenoGla Diagnostics, Faro, Portugal) and BMP-2/4 antibodies as described above.
Alkaline phosphatase activity
Cells were lysed in 1% Triton X-100 in PBS, subjected to 2 freeze-thaw cycles and centrifuged at 13000 g for 5 minutes. ALP activity in the supernatants was measured at 405 nm using 4-Nitrophenyl phosphate disodium salt hexahydrate (Sigma) as substrate. Enzyme activity (U) was normalised to protein concentrations.
Data shown are mean ± SD. All data were verified in ≥3 independent experiments. Statistical analysis was performed by 1-way ANOVA with Bonferroni post hoc test or Student’s t-test, as stated in figure legends, using PRISM software (GraphPad). Values of P < 0.05 were considered statistically significant.
The datasets generated during and/or analysed during the current study are available from the corresponding author on reasonable request.
Cees Vermeer is the CSO of VitaK BV, a spin-off company fully owned by Maastricht University. Dina C. Simes and Carla S. B. Viegas are cofounders of GenoGla Diagnostics.
Hunt, J. L. et al. Bone formation in carotid plaques: a clinicopathological study. Stroke 33, 1214–1219 (2002).
Duer, M. J. et al. Mineral surface in calcified plaque is like that of bone: further evidence for regulated mineralization. Arterioscler Thromb Vasc Biol 28, 2030–2034, https://doi.org/10.1161/atvbaha.108.172387 (2008).
Rennenberg, R. J. et al. Vascular calcifications as a marker of increased cardiovascular risk: a meta-analysis. Vasc Health Risk Manag 5, 185–197 (2009).
Sage, A. P., Tintut, Y. & Demer, L. L. Regulatory mechanisms in vascular calcification. Nat Rev Cardiol 7, 528–536, https://doi.org/10.1038/nrcardio.2010.115 (2010).
Shroff, R., Long, D. A. & Shanahan, C. Mechanistic insights into vascular calcification in CKD. J Am Soc Nephrol 24, 179–189, https://doi.org/10.1681/asn.2011121191 (2013).
Chatrou, M. L., Winckers, K., Hackeng, T. M., Reutelingsperger, C. P. & Schurgers, L. J. Vascular calcification: the price to pay for anticoagulation therapy with vitamin K-antagonists. Blood reviews 26, 155–166 (2012).
Shanahan, C. M., Crouthamel, M. H., Kapustin, A. & Giachelli, C. M. Arterial calcification in chronic kidney disease: key roles for calcium and phosphate. Circ Res 109, 697–711, https://doi.org/10.1161/circresaha.110.234914 (2011).
Jono, S. et al. Phosphate regulation of vascular smooth muscle cell calcification. Circ Res 87, E10–17 (2000).
Schurgers, L. J., Uitto, J. & Reutelingsperger, C. P. Vitamin K-dependent carboxylation of matrix Gla-protein: a crucial switch to control ectopic mineralization. Trends Mol Med 19, 217–226, https://doi.org/10.1016/j.molmed.2012.12.008 (2013).
Liu, Y., Drozdov, I., Shroff, R., Beltran, L. E. & Shanahan, C. M. Prelamin A accelerates vascular calcification via activation of the DNA damage response and senescence-associated secretory phenotype in vascular smooth muscle cells. Circ Res 112, e99–109, https://doi.org/10.1161/circresaha.111.300543 (2013).
Neven, E., Dauwe, S., De Broe, M. E., D’Haese, P. C. & Persy, V. Endochondral bone formation is involved in media calcification in rats and in men. Kidney Int 72, 574–581 (2007).
Iyemere, V. P., Proudfoot, D., Weissberg, P. L. & Shanahan, C. M. Vascular smooth muscle cell phenotypic plasticity and the regulation of vascular calcification. J Intern Med 260, 192–210, https://doi.org/10.1111/j.1365-2796.2006.01692.x (2006).
Frid, M. G., Shekhonin, B. V., Koteliansky, V. E. & Glukhova, M. A. Phenotypic changes of human smooth muscle cells during development: late expression of heavy caldesmon and calponin. Dev Biol 153, 185–193 (1992).
Huang, Q. Q., Fisher, S. A. & Brozovich, F. V. Forced expression of essential myosin light chain isoforms demonstrates their role in smooth muscle force production. J Biol Chem 274, 35095–35098 (1999).
Feil, S., Hofmann, F. & Feil, R. SM22alpha modulates vascular smooth muscle cell phenotype during atherogenesis. Circ Res 94, 863–865, https://doi.org/10.1161/01.res.0000126417.38728.f6 (2004).
Shankman, L. S. et al. KLF4-dependent phenotypic modulation of smooth muscle cells has a key role in atherosclerotic plaque pathogenesis. Nat Med 21, 628–637, https://doi.org/10.1038/nm.3866 (2015).
Alexander, M. R. & Owens, G. K. Epigenetic control of smooth muscle cell differentiation and phenotypic switching in vascular development and disease. Annu Rev Physiol 74, 13–40, https://doi.org/10.1146/annurev-physiol-012110-142315 (2012).
Dhore, C. R. et al. Differential expression of bone matrix regulatory proteins in human atherosclerotic plaques. Arterioscler Thromb Vasc Biol 21, 1998–2003 (2001).
Speer, M. Y. et al. Smooth muscle cells give rise to osteochondrogenic precursors and chondrocytes in calcifying arteries. Circ Res 104, 733–741, https://doi.org/10.1161/circresaha.108.183053 (2009).
Shanahan, C. M. et al. Medial localization of mineralization-regulating proteins in association with Mönckeberg’s sclerosis evidence for smooth muscle cell–mediated vascular calcification. Circulation 100, 2168–2176 (1999).
Li, X., Yang, H. Y. & Giachelli, C. M. BMP-2 promotes phosphate uptake, phenotypic modulation, and calcification of human vascular smooth muscle cells. Atherosclerosis 199, 271–277 (2008).
Giachelli, C. M. et al. Osteopontin is elevated during neointima formation in rat arteries and is a novel component of human atherosclerotic plaques. J Clin Invest 92, 1686–1696, https://doi.org/10.1172/jci116755 (1993).
Kapustin, A. N. et al. Vascular smooth muscle cell calcification is mediated by regulated exosome secretion. Circ Res 116, 1312–1323, https://doi.org/10.1161/circresaha.116.305012 (2015).
Tagariello, A. et al. Ucma–A novel secreted factor represents a highly specific marker for distal chondrocytes. Matrix Biol 27, 3–11, https://doi.org/10.1016/j.matbio.2007.07.004 (2008).
Viegas, C. S. et al. Gla-rich protein (GRP), a new vitamin K-dependent protein identified from sturgeon cartilage and highly conserved in vertebrates. J Biol Chem 283, 36655–36664, https://doi.org/10.1074/jbc.M802761200 (2008).
Viegas, C. S. et al. Gla-rich protein is a novel vitamin K-dependent protein present in serum that accumulates at sites of pathological calcifications. Am J Pathol 175, 2288–2298, https://doi.org/10.2353/ajpath.2009.090474 (2009).
Viegas, C. S. et al. Gla-rich protein acts as a calcification inhibitor in the human cardiovascular system. Arterioscler Thromb Vasc Biol 35, 399–408, https://doi.org/10.1161/atvbaha.114.304823 (2015).
Eitzinger, N. et al. Ucma is not necessary for normal development of the mouse skeleton. Bone 50, 670–680, https://doi.org/10.1016/j.bone.2011.11.017 (2012).
Surmann-Schmitt, C. et al. Ucma, a novel secreted cartilage-specific protein with implications in osteogenesis. J Biol Chem 283, 7082–7093, https://doi.org/10.1074/jbc.M702792200 (2008).
Lee, Y. J. et al. Ucma, a direct transcriptional target of Runx2 and Osterix, promotes osteoblast differentiation and nodule formation. Osteoarthritis Cartilage 23, 1421–1431, https://doi.org/10.1016/j.joca.2015.03.035 (2015).
Le Jeune, M. et al. Identification of four alternatively spliced transcripts of the Ucma/GRP gene, encoding a new Gla-containing protein. Exp Cell Res 316, 203–215, https://doi.org/10.1016/j.yexcr.2009.10.002 (2010).
Steitz, S. A. et al. Smooth muscle cell phenotypic transition associated with calcification: upregulation of Cbfa1 and downregulation of smooth muscle lineage markers. Circ Res 89, 1147–1154 (2001).
Hough, C., Radu, M. & Doré, J. J. E. TGF-Beta Induced Erk Phosphorylation of Smad Linker Region Regulates Smad Signaling. PLoS One 7, e42513, https://doi.org/10.1371/journal.pone.0042513 (2012).
Mizobuchi, M., Towler, D. & Slatopolsky, E. Vascular calcification: the killer of patients with chronic kidney disease. Journal of the American Society of Nephrology 20, 1453–1464 (2009).
Cheung, A. K. et al. Atherosclerotic cardiovascular disease risks in chronic hemodialysis patients. Kidney international 58, 353–362 (2000).
Olechnowicz-Tietz, S., Gluba, A., Paradowska, A., Banach, M. & Rysz, J. The risk of atherosclerosis in patients with chronic kidney disease. International urology and nephrology 45, 1605–1612 (2013).
Liu, F., Hata, A., Baker, J. C. & Doody, J. A human Mad protein acting as a BMP-regulated transcriptional activator. Nature 381, 620 (1996).
Heldin, C.-H., Miyazono, K. & Ten Dijke, P. TGF-β signalling from cell membrane to nucleus through SMAD proteins. Nature 390, 465–471 (1997).
de Jesus Perez, V. A. et al. Bone morphogenetic protein 2 induces pulmonary angiogenesis via Wnt–β-catenin and Wnt–RhoA–Rac1 pathways. The Journal of Cell Biology 184, 83–99, https://doi.org/10.1083/jcb.200806049 (2009).
Cai, T. et al. WNT/beta-catenin signaling promotes VSMCs to osteogenic transdifferentiation and calcification through directly modulating Runx2 gene expression. Exp Cell Res 345, 206–217, https://doi.org/10.1016/j.yexcr.2016.06.007 (2016).
Guerrero, F. et al. TGF-beta prevents phosphate-induced osteogenesis through inhibition of BMP and Wnt/beta-catenin pathways. PLoS One 9, e89179, https://doi.org/10.1371/journal.pone.0089179 (2014).
Lin, T., Wang, X.-L., Zettervall, S. L., Cai, Y. & Guzman, R. J. Dorsomorphin homologue 1, a highly selective small-molecule bone morphogenetic protein inhibitor, suppresses medial artery calcification. Journal of Vascular Surgery 66, 586–593, https://doi.org/10.1016/j.jvs.2016.03.462 (2017).
Proudfoot, D., Skepper, J. N., Shanahan, C. M. & Weissberg, P. L. Calcification of human vascular cells in vitro is correlated with high levels of matrix Gla protein and low levels of osteopontin expression. Arteriosclerosis, thrombosis, and vascular biology 18, 379–388 (1998).
McCabe, K. M. et al. Dietary vitamin K and therapeutic warfarin alter the susceptibility to vascular calcification in experimental chronic kidney disease. Kidney international 83, 835–844 (2013).
Rafael, M. S. et al. Insights into the association of Gla-rich protein and osteoarthritis, novel splice variants and gamma-carboxylation status. Mol Nutr Food Res 58, 1636–1646, https://doi.org/10.1002/mnfr.201300941 (2014).
Shanahan, C. M., Crouthamel, M. H., Kapustin, A. & Giachelli, C. M. Arterial Calcification in Chronic Kidney Disease: Key Roles for Calcium and Phosphate. Circulation Research 109, 697–711 (2011).
Willems, B. A., Vermeer, C., Reutelingsperger, C. P. & Schurgers, L. J. The realm of vitamin K dependent proteins: shifting from coagulation toward calcification. Mol Nutr Food Res 58, 1620–1635, https://doi.org/10.1002/mnfr.201300743 (2014).
Schurgers, L. J. et al. Vitamin K-antagonists accelerate atherosclerotic calcification and induce a vulnerable plaque phenotype. PLoS One 7, e43229, https://doi.org/10.1371/journal.pone.0043229 (2012).
Gregory, C. A., Gunn, W. G., Peister, A. & Prockop, D. J. An Alizarin red-based assay of mineralization by adherent cells in culture: comparison with cetylpyridinium chloride extraction. Anal Biochem 329, 77–84, https://doi.org/10.1016/j.ab.2004.02.002 (2004).
This work was supported in part by research funding from NWO ZonMw (MKMD 40-42600-98-13007). CSB Viegas is the recipient of the FCT fellowship SFRH/BPD/70277/2010.
The authors declare no competing interests.
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Willems, B.A., Furmanik, M., Caron, M.M.J. et al. Ucma/GRP inhibits phosphate-induced vascular smooth muscle cell calcification via SMAD-dependent BMP signalling. Sci Rep 8, 4961 (2018). https://doi.org/10.1038/s41598-018-23353-y
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