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Cell Death and Differentiation logoLink to Cell Death and Differentiation
. 2017 Sep 22;25(2):268–281. doi: 10.1038/cdd.2017.153

A vitronectin-derived peptide reverses ovariectomy-induced bone loss via regulation of osteoblast and osteoclast differentiation

Seung-Ki Min 1,3, Hyun Ki Kang 2,3, Sung Youn Jung 2,3, Da Hyun Jang 2, Byung-Moo Min 2,*
PMCID: PMC5762842  PMID: 28937683

Abstract

Osteoporosis affects millions of people worldwide by promoting bone resorption and impairing bone formation. Bisphosphonates, commonly used agents to treat osteoporosis, cannot reverse the substantial bone loss that has already occurred by the time of diagnosis. Moreover, their undesirable side-effects, including osteonecrosis of the jaw, have been reported. Here, we demonstrated that a new bioactive core vitronectin-derived peptide (VnP-16) promoted bone formation by accelerating osteoblast differentiation and activity through direct interaction with β1 integrin followed by FAK activation. Concomitantly, VnP-16 inhibited bone resorption by restraining JNK-c-Fos-NFATc1-induced osteoclast differentiation and αvβ3 integrin-c-Src-PYK2-mediated resorptive function. Moreover, VnP-16 decreased the bone resorbing activity of pre-existing mature osteoclasts without changing their survival rate. Furthermore, VnP-16 had a strong anabolic effect on bone regeneration by stimulating osteoblast differentiation and increasing osteoblast number, and significantly alleviated proinflammatory cytokine-induced bone resorption by restraining osteoclast differentiation and function in murine models. Moreover, VnP-16 could reverse ovariectomy-induced bone loss by both inhibiting bone resorption and promoting bone formation. Given its dual role in promoting bone formation and inhibiting bone resorption, our results suggest that VnP-16 could be an attractive therapeutic agent for treating osteoporosis.

Bone defects that result from fractures, accidents, cancer, or other diseases pose a serious risk of loss of function and can significantly impair quality of life.1 Current grafting methods have limitations such as donor site morbidity and graft rejection.2, 3 Osteoporosis is a systematic skeletal disorder characterized by low bone mass, microarchitectural deterioration of bone tissue, and susceptibility to fracture.4, 5, 6 Furthermore, the incidence of osteoporosis is very high and has increased due to ageing of populations worldwide, which is responsible for a growing number of postmenopausal women with osteoporosis.7, 8 More improved bone formation method such as new therapeutic agents is highly in demand because many patients with osteoporosis followed by fractures still end up with poor clinical outcomes after the current surgery and techniques for bone healing.9

Proteins are of major concern in the field of tissue engineering because of their exquisite potency and selectivity for their molecular targets.10 Although the functions and potential applications of several proteins in bone engineering have been described,11 the use of proteins for therapeutics is associated with high cost and a number of other disadvantages.12 Because of their flexibility in adopting and mimicking the local structural features of proteins,13 peptides are a valid alternative.14 Furthermore, the use of peptides in regenerative medicine has several advantages over the use of entire proteins in terms of immunogenicity, susceptibility to degradation, and tumor-related side effects.15, 16, 17 To date, local application of numerous peptides has been used to repair bone defects in the clinic; however, very few peptides have the ability to form bone themselves.13 On the other hand, a few peptide drugs derived from protein hormones such as calcitonin gene-related peptide (α-CGRP; 37-mer) and parathyroid hormone 1–34 peptide (teriparatide) have shown clinical usefulness for treating osteopenia/osteoporosis and calcium homeostasis disorders.13 Among their functions, α-CGRP inhibits bone resorption by inhibiting nuclear factor kappa B (NF-κB) activity whereas teriparatide increases bone mass by stimulating bone formation via promoting osteoblast proliferation and differentiation and preventing its apoptosis.13, 18 However, a concern has been raised about the potential risk of osteosarcoma in patients who have used teriparatide as high percentage of the rats treated with high dose of it shows osteosarcoma.19

Normal bone mass and architecture are maintained by osteoclasts and osteoblasts, and bone is continuously renewed through a dynamic balance between resorption and formation. An imbalance caused by the increased activity and/or number of osteoclasts leads to bone destruction in pathological bone diseases;4 therefore, much focus has been placed on the pharmacological control of osteoclasts for the treatment of osteoclast-related bone disorders such as osteoporosis and arthritis.5, 6 Osteoclastogenesis is cooperatively induced by macrophage-colony stimulating factor (M-CSF), receptor activator of NF-κB ligand (RANKL), and its co-stimulatory factor.20, 21, 22 RANKL induces entire processes that promote the development of osteoclasts.23, 24 Specifically, RANKL activates the three mitogen-activated protein kinases (MAPKs), leading to the activation of downstream regulators of osteoclast formation, including c-Fos and nuclear factor of activated T cells, cytoplasmic 1 (NFATc1), both of which are master regulators of osteoclast differentiation.20, 21, 22, 25 NFATc1 regulates a number of osteoclast-specific genes in cooperation with other transcription factors.26 cAMP-response element-binding protein also cooperates with NFATc1 to activate these genes.27 The roles of NFATc1 in osteoclastogenesis have been demonstrated in vitro and in vivo.25, 28, 29 Furthermore, proline-rich tyrosine kinase 2 (PYK2) forms a complex with c-Src, linking αvβ3 integrin signaling to actin cytoskeletal organization in osteoclasts.30

Vitronectin, an abundant multifunctional glycoprotein found in serum, the extracellular matrix, and bone,31 is involved in various physiological processes and promotes cell attachment, spreading, and migration.32, 33 Here, we developed a new vitronectin-derived therapeutic peptide named VnP-16 (RVYFFKGKQYWE; residues 270–281) that promotes osteoblast differentiation and activity, and concomitantly restrains osteoclast differentiation and resorptive function. We elucidated the mechanism by which VnP-16 exhibits opposite effects on osteoblast and osteoclast differentiation, and its biological potency on bone formation and resorption, in three different, but complementary, animal models.

Results

A human vitronectin-derived peptide promotes osteogenic cell behavior

To identify the biologically active sequences that confer bone-forming activity, three constructs covering the entire human vitronectin protein were generated (rVn-FI, rVn-FII, and rVn-FIII; Figure 1a), expressed separately in Escherichia coli (Figure 1b), and characterized (Figures 1c and d). Characterization of the bacterially expressed rVn truncations showed the presence of intramolecular disulfide bonds in all three recombinant proteins (Figure 1c) and protein rich in β-structure (Figure 1d), suggesting their sufficiency in folding. Furthermore, analyses of rVn truncations showed their ability to perform cell behavior, except rVn-FIII (Figures 1e–h). Even though rVn-FI was the most biologically active of the three recombinant truncations (Figures 1f–h), however, we focused on identifying the bioactive cell binding sequences required for this activity of rVn-FII, because peptides lacking the RGD motif within the rVn-FI region did not show cell attachment and spreading activities (data not shown).

Figure 1.

Figure 1

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Analyses of purified rVn truncations by SDS-PAGE and circular dichroism spectroscopy and their effects on cell behavior. (a) Schematic diagram of the rVn truncations. The amino acid (aa) positions and the domain structure of full-length vitronectin are indicated. The black box and colored bars represent the signal peptide and the positions of the recombinant proteins, respectively. (b) Schematic diagram and SDS-PAGE analyses (10% polyacrylamide gels under reducing conditions) of the purified rVn proteins, expressed as His6-tagged fusions. The bands were visualized by Coomassie staining. (c) Gel mobilities (12.5% SDS-PAGE) of the purified rVn proteins treated with or without dithiothreitol (DTT). (d) Circular dichroism analysis of the rVn fragments in PBS (pH 3.0) at 23 °C. (e) The dose-dependent effects of the truncated rVn proteins on the attachment of human osteogenic cells. The cells were seeded onto rVn-treated plates for 1 h in serum-free medium. (f and g) Cell attachment (f) and spreading (g) of osteogenic cells induced by BSA (1%), vitronectin (0.23 μg/cm2), and the truncated rVn proteins (5.7 μg/cm2) for 1 h (f) or 3 h (g) in serum-free medium. (h) Migration of osteogenic cells induced by vitronectin and the truncated rVn proteins. Osteogenic cells were seeded into the upper chambers of Transwell filters coated with vitronectin or rVn proteins and were incubated for 24 h. ND, not detected. Data in (e–h) represent the mean±SD (n=4). **P<0.01

A series of overlapping 12-mer peptides (VnP-11 to VnP-21) covering the rVn-FII truncation (amino acids 230–322), which contained two α-helices and nine β-strands (Supplementary Figure S1), was synthesized (Figure 2a). Human osteogenic cells that were differentiated from skin-derived precursors (SKPs) were used to test the functions and osteoinductive activities of the synthetic peptides. Directed differentiation from SKPs to mesenchymal precursors to osteogenic cells is shown in Supplementary Figure S2. VnP-16 promoted the cell attachment activity of osteogenic cells in a dose-dependent manner, and its activity reached a maximum at a concentration of approximately 9.1 μg/cm2 (Figures 2b and c). VnP-16 also induced cell spreading to an extent that was comparable to that of vitronectin (Figure 2d), but did not affect the viability of the osteogenic cells (Figure 2e). Next, to determine the minimum bioactive sequence, synthetic peptides were prepared from VnP-16, which are N- and C-terminal truncated peptides (Figure 2f). Further deletion in VnP-16 led to significantly lower cell attachment than that of VnP-16 (Figure 2g), demonstrating that VnP-16 is a bioactive core binding sequence for cellular responses. We further investigated whether VnP-16 could also mediate the attachment of other types of cells. Notably, VnP-16 enhanced the attachment of primary fibroblasts, including normal human dermal fibroblasts (NHDFs) and normal human oral fibroblasts (NHOFs), and fibroblast lineages, including MC3T3-E1 and NIH/3T3 cells, but not that of other cell types, including normal human epidermal keratinocytes (NHEKs) and normal human oral keratinocytes (NHOKs; Figure 2h). These results demonstrate that VnP-16 acts via a fibroblast lineage-specific attachment mechanism. In addition, VnP-16 did not affect the viabilities of the fibroblasts (Supplementary Figure S3), indicating that it is cytocompatible. The PSIPRED protein structure prediction server identified two β-strands in the VnP-16 (Figure 2i). Taken together, these data demonstrate that VnP-16 is a bioactive core binding sequence that acts on fibroblast lineage cells, including human osteogenic cells, but not on normal human keratinocytes.

Figure 2.

Figure 2

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VnP-16 promotes cell behavior in fibroblast lineages. (a) The locations of the synthetic peptides (VnP-11 to VnP-21) in the amino acid sequence of the central region of human vitronectin (residues 230–322). (b) Dose-dependent cell attachment to immobilized synthetic peptides. Human osteogenic cells were allowed to adhere to peptide-treated plates for 1 h in serum-free medium. (c and d) Cell attachment (c) and spreading (d) of osteogenic cells induced by treatment with BSA (1%), vitronectin (0.23 μg/cm2), rVn-FII (5.7 μg/cm2), or the synthetic peptides (9.1 μg/cm2) for 1 h (c) or 3 h (d) in serum-free medium. (e) The viabilities of osteogenic cells treated with VnP-16 for 24 or 48 h. (f) The amino acid sequence of N- and C-terminal truncated peptides for VnP-16. (g) Attachment of osteogenic cells induced by vitronectin, rVn-FII, and peptides. (h) Attachment of NHEKs, NHOKs, NHDFs, NHOFs, PC-12 cells, MC3T3-E1 cells, CV-1 cells, and NIH/3T3 cells to VnP-16 (9.1 μg/cm2). The cells were allowed to adhere to VnP-16-treated plates for 1 h in serum-free medium. (i) The predicted structure of the VnP-16 dodecapeptide computed using the PSIPRED protein structure prediction server. The positions of the two β-strands (yellow arrows) on the coil (black line) are indicated. Conf, confidence of prediction; Pred, predicted secondary structure; AA, target sequence. Data in (b–e,g,h) represent the mean±SD (n=4). **P<0.01

β1 integrin mediates VnP-16-induced osteogenic cell attachment

Next, we examined which specific adhesion receptor for VnP-16 mediates cell attachment in human osteogenic cells. Cell attachment to VnP-16 was not inhibited by heparin (Figure 3a), suggesting that the cell surface proteoglycan receptor is not the receptor for VnP-16. Because binding of integrins and α-dystroglycan to their ligands requires a divalent cation such as Ca2+ or Mn2+,34 we investigated the effect of EDTA, a metal-chelating reagent, on cell attachment to VnP-16. Pretreatment of osteogenic cells with EDTA inhibited their attachment to VnP-16 completely, whereas treatment with Mn2+ enhanced cell attachment significantly (Figure 3a). Investigation of the effects of integrin subunit-blocking antibodies on cell attachment to VnP-16 revealed a significant inhibitory effect of a β1-blocking antibody (Figure 3b). β3 integrin also plays a key role in cell attachment and migration;35 however, it was not involved in VnP-16-mediated osteogenic cell attachment. Furthermore, suppression of β1 integrin expression by transfection of cells with a β1 integrin-specific small interfering RNA (siRNA; Figures 3c and d) inhibited cell attachment to VnP-16 significantly (Figure 3e). Next, to further explore whether VnP-16 directly binds to and activates cell surface β1 integrins, we cultured human osteogenic cells on biotinylated VnP-16-coated dishes for 30 min, performed a pulldown assay with streptavidin beads, and then measured the level of β1 integrin by immunoblotting. Biotinylated VnP-16 directly bound to cell surface β1 integrins (Figure 3f). These data indicate that β1 integrin functions as a major surface receptor for VnP-16 in human osteogenic cells.

Figure 3.

Figure 3

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VnP-16 promotes osteogenic cell attachment through direct interaction with β1 integrin. (a) Attachment of human osteogenic cells pretreated with EDTA (5 mM), MnCl2 (500 μM), or heparin (100 μg/ml) to VnP-16. The cells were seeded onto plates that were precoated with VnP-16 (9.1 μg/cm2) for 1 h. (b) The effects of various integrin-blocking antibodies on cell attachment to VnP-16. (c–e) Immunoblotting (c) and densitometric analysis (d) of β1 integrin, and cell attachment to VnP-16 (e) in osteogenic cells that were transfected with a control (Con) or β1 integrin-specific siRNA (10 nM; β1 integrin). (f) Streptavidin-bead pulldown assay with the biotinylated SP or biotinylated VnP-16 peptides from extracts of osteogenic cells that were cultured on biotinylated SP- or biotinylated VnP-16-coated dishes for 30 min. Data in (a,b,e) (n=4), and (d) (n=2) represent the mean±SD. **P<0.01

FAK activation plays an essential role in osteoblast differentiation

To investigate the downstream pathways stimulated by VnP-16/β1 integrin-mediated signaling, we examined whether binding of VnP-16 to osteogenic cells induced FAK activation. Compared with that in vehicle- or scrambled peptide (SP)-treated control cells, the levels of FAK phosphorylation at Tyr-397 and -577 were higher after VnP-16-mediated attachment and spreading of osteogenic cells; however, the levels of phospho-FAK Tyr-407, -576, and -861 were retained at basal levels (Figures 4a and b). Because FAK Tyr397 is an autophosphorylation site that promotes interaction with c-Src or Fyn,36 we also measured the expression level of phospho-c-Src. The level of phospho-c-Src Tyr416 was increased in vitronectin- or VnP-16-treated cells, but those of phospho-Akt Ser473 and phospho-PKCδ Thr505 were not (Figures 4a and b), suggesting that FAK phosphorylation at Tyr-397 and -577, and c-Src phosphorylation at Tyr416 are linked to VnP-16/β1 integrin-mediated signaling. Furthermore, cell attachment to VnP-16 was inhibited in a dose-dependent manner by pretreatment of the cells with PF-573228 (Figures 4c–e), a known FAK inhibitor that effectively blocks phosphorylation of the protein at Tyr397.37

Figure 4.

Figure 4

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VnP-16 promotes osteogenic differentiation through β1 integrin/FAK signaling. (a,b) Immunoblotting (a) and densitometric analyses (b) of phospho-FAK, phospho-Akt Ser473, phospho-PKCδ Thr505, and phospho-c-Src Tyr416 in osteogenic cells that were cultured for 3 h on plates coated with vitronectin (0.23 μg/cm2), SP, or VnP-16 (9.1 μg/cm2). (c,d) Immunoblotting (c) and densitometric analyses (d) of total FAK (t-FAK) and phospho-FAK Tyr397 in osteogenic cells that were pretreated with PF-573228 for 1 h. (e) Attachment of cells that were treated with PF-573228 for 1 h in serum-free medium to plates precoated with VnP-16 (9.1 μg/cm2). (f) The effects of VnP-16 on alkaline phosphatase activity and calcium deposition in SKP-derived mesenchymal precursors (MPs), mouse calvarial osteoblast precursors (MC3T3-E1), and human osteogenic cells (Osteogenic). The cells were cultured in osteogenic differentiation medium containing VnP-16 or SP (50 μg/0.5 ml) for 2 weeks. (g) The effects of PF-573228 on alkaline phosphatase activity and calcium deposition in SKP-derived mesenchymal precursors, MC3T3-E1, and human osteogenic cells. The cells were cultured on VnP-16-treated (9.1 μg/cm2) plates in osteogenic differentiation medium with or without 1 μM PF-573228 for 2 weeks. (h–j) Immunoblotting (h) and densitometric analyses (i) of t-FAK, and dose-dependent attachment (j) of control or FAK-specific siRNA-treated (100 nM) osteogenic cells to VnP-16. (k) Determination of apoptotic cells in osteogenic cells that were cultured for 24, 48, and 96 h on plates coated with SP or VnP-16 (9.1 μg/cm2) by TUNEL assay. Data in (b, d and i) (n=3), and (e, j and k) (n=4) represent the mean±SD. *P<0.05 or **P<0.01 compared to vehicle or control siRNA

To assess the effects of VnP-16 on osteoblast differentiation, osteoblast precursors and osteogenic cells were cultured in osteogenic differentiation medium containing VnP-16 or SP. VnP-16 increased the alkaline phosphatase activity and calcium deposition in the osteoblast precursors (Figure 4f), indicating that VnP-16 promotes osteoblast differentiation. Next, to investigate the role of FAK phosphorylation at Tyr397 on osteoblast differentiation, osteoblast precursors and osteogenic cells were cultured on VnP-16-treated plates in osteogenic differentiation medium containing PF-573228 or vehicle alone. PF-573228 reduced the alkaline phosphatase activity and calcium deposition in the osteoblast precursors (Figure 4g), indicating that the suppression of FAK phosphorylation at Tyr397 inhibits osteoblast differentiation. In addition, PF-573228 did not affect cell growth at the concentrations and incubation times used here (data not shown), excluding the possibility that the observed inhibition of cell attachment to VnP-16 was caused by general cytotoxicity. Furthermore, suppression of FAK expression using a specific siRNA inhibited cell attachment to VnP-16 significantly, whereas a control siRNA did not (Figures 4h–j). On the other hand, VnP-16 did not affect the apoptosis of the osteogenic cells at the concentration (9.1 μg/cm2) that promoted osteogenic cell behavior (Figure 4k). Overall, these data support the concept that FAK phosphorylation at Tyr397 plays an essential role in VnP-16/β1 integrin-mediated signaling and osteoblast differentiation.

VnP-16 promotes bone formation in vivo

To explore whether VnP-16 promoted bone formation in vivo, we used an 8 mm critical-sized calvarial defect rat model.38 Microcomputed tomographic (μCT) images of calvarial defects demonstrated that the vehicle- and SP-treated control groups showed limited new bone formation at the defect margins 2 weeks after surgery, whereas the VnP-16-treated group showed distinctive bone healing (Figure 5a). The amount of regenerated bone in the VnP-16-treated group was comparable to that in the recombinant human bone morphogenetic protein 2 (rhBMP-2)-treated group (Figure 5a). Quantitative bone morphometric analyses of the bone recovery rate (Figure 5b), bone volume/tissue volume ratio (BV/TV; Figure 5c), and calvarial thickness (Figure 5d), consistent with the greater amount of osteoid shown by Masson’s trichrome staining (Figure 5e), confirmed that the VnP-16-treated group displayed a higher level of bone regeneration than the SP-treated groups. In the vehicle- and SP-treated control groups, the defects were mostly filled with loose fibrous connective tissues and degradation remnants of the absorbable collagen sponges used as scaffolds (Figure 5e). The number of osteoblasts per bone perimeter was significantly higher in the VnP-16-treated group than the SP-treated group, and the number of osteoblasts in the VnP-16-treated group was comparable to that in the rhBMP-2-treated group (Figure 5f). Furthermore, the expression levels of alkaline phosphatase and bone sialoprotein, early markers of osteoblast differentiation, were significantly higher in the VnP-16-treated group than the SP-treated control group (Figure 5g). These data demonstrate that VnP-16 has a strong anabolic effect on bone formation by stimulating osteoblast differentiation and increasing osteoblast number.

Figure 5.

Figure 5

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The effects of VnP-16 on bone regeneration in vivo. (a) μCT images of the bone defects in each group. Critical-sized rat calvarial defects were implanted with absorbable collagen sponges treated with vehicle (DMSO), rhBMP-2 (2 μg/scaffold), SP (1 mg/scaffold), or VnP-16 (1 mg/scaffold). (b–d) Quantitative bone morphometric analyses of the bone recovery rate (b), BV/TV (c), and calvarial thickness (d) in the region of the defects. (e) μCT images of the bone defects and Masson’s trichrome staining (MT) of rat calvarial sections 2 weeks after transplantation. The triangles indicate the wound edges. For histomorphometric analysis, the specimens were decalcified with 12% EDTA for 4 weeks and embedded in paraffin. The paraffin-embedded samples were sectioned at a thickness of 4 μm and then stained with Masson’s trichrome. Scale bars, 1 mm. (f) The number of osteoblasts per bone perimeter from rat calvarial sections 2 weeks after transplantation. Ob.N, osteoblast number; B.Pm, bone perimeter. (Scale bars, 50 μm.) (g) qPCR analysis of the expression levels of osteogenic markers in each group. ALP, alkaline phosphatase; BSP, bone sialoprotein. Data in (b–d, f and g) represent the mean±SD (n=5 per group). **P<0.01

VnP-16 restrains osteoclast differentiation by suppressing Janus N-terminal Kinase (JNK)-c-Fos-NFATc1 signaling

Next, we examined whether VnP-16 could inhibit osteoclast differentiation by acting directly on osteoclast precursor cells. M-CSF and RANKL induced the formation of numerous tartrate-resistant acid phosphatase (TRAP)-positive multinucleated osteoclasts from bone marrow-derived macrophages (BMMs; Figure 6a). VnP-16 inhibited M-CSF and RANKL-induced osteoclastogenesis almost completely, whereas vehicle and SP had no effect; notably, vitronectin also had no effect on osteoclastogenesis (Figures 6a–c). The anti-osteoclastogenic effects of VnP-16 were confirmed by its ability to suppress F-actin-mediated cytoskeletal organization in preosteoclasts (Figure 6d); however, VnP-16 had no such effect on mature osteoclasts (Supplementary Figure S4). To investigate whether VnP-16 affects bone resorbing activity in vitro, BMMs were cultured for 6 days on Osteo Assay Surface plates that were coated with vehicle, vitronectin, SP, or VnP-16, in the presence of M-CSF and RANKL. Numerous resorption pits caused by osteoclasts were generated in the vehicle- and SP-treated controls; however, VnP-16 inhibited the number and area of these pits significantly (Figures 6e and f). In addition, when used at the concentration (9.1 μg/cm2) that blocked osteoclastogenesis, VnP-16 did not affect the proliferation or viability of BMMs (Figure 6g), indicating that its inhibitory effect on osteoclastogenesis was not due to cytotoxicity or reduced cell proliferation.

Figure 6.

Figure 6

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The effects of VnP-16 on M-CSF- and RANKL-induced osteoclast formation, F-actin-mediated cytoskeletal organization, resorptive activity, and the expression levels of osteoclastogenesis-related genes. (a–d) BMMs were cultured for 6 days on plates that were precoated with vehicle (DMSO), vitronectin (0.23 μg/cm2), SP (9.1 μg/cm2), or VnP-16 (9.1 μg/cm2), in the presence of 30 ng/ml M-CSF and 100 ng/ml RANKL. The induced cells were stained for TRAP (a) and immunostained with DAPI (blue) and rhodamine-phalloidin (F-actin, red) (d). TRAP-positive multinucleated cells containing three or more nuclei were counted as osteoclasts (b). The sizes of the osteoclasts were obtained by measuring the diameters of multinucleated TRAP-positive cells on × 40 photomicrographs (c). Scale bars, 200 μm. (e and f) The effects of VnP-16 on the bone resorbing activity of osteoclasts. BMMs were cultured for 6 days on Osteo Assay Surface plates that were coated with vehicle (DMSO), vitronectin (0.23 μg/cm2), or synthetic peptide (9.1 μg/cm2), in the presence of 30 ng/ml M-CSF and 100 ng/ml RANKL. The cells were removed and the resorbed pits were photographed (e). The blue arrows indicate the resorption pits formed by osteoclasts. Bone resorption was assessed by pit area measurements (f). Scale bars, 200 μm. (g) The effect of the concentration of VnP-16 (9.1 μg/cm2) that blocked osteoclast formation on the proliferation and viability of BMMs. (h and i) Immunoblotting (h) and densitometric analyses (i) of the osteoclastogenesis-related proteins in BMMs that were cultured for 1–3 days on plates precoated with SP or VnP-16 (9.1 μg/cm2), in the presence of 30 ng/ml M-CSF and 100 ng/ml RANKL. CREB, cAMP-response element-binding protein; ATF-1, activating transcription factor 1. (j,k) Immunoblotting (j) and densitometric analyses (k) of MAPKs in BMMs that were cultured for 3 days on plates precoated with SP or VnP-16 (9.1 μg/cm2), in the presence of 30 ng/ml M-CSF and 100 ng/ml RANKL, serum-starved for 3 h, and stimulated with M-CSF (30 ng/ml) and RANKL (100 ng/ml) for the indicated times. ERK, extracellular signal-regulated kinase. Data in (b,c,f and g) (n=4), and (i and k) (n=3) represent the mean±SD. **P<0.01

To assess the molecular mechanisms underlying the inhibitory effects of VnP-16 on M-CSF and RANKL-induced osteoclast differentiation, we examined the expression levels of c-Fos and NFATc1, which are crucial and fundamental transcription factors involved in osteoclast differentiation.20, 21, 22, 25 Treatment of BMMs with VnP-16 suppressed the M-CSF and RANKL-induced expression of c-Fos and NFATc1 (Figures 6h and i). To investigate the underlying mechanism, we examined the effects of VnP-16 on the activation of MAPKs, the upstream regulators of c-Fos and NFATc1. These RANKL downstream signaling events have been implicated in the expression of c-Fos and NFATc1 and osteoclast differentiation.39, 40 VnP-16 did not affect basal JNK levels but it did inhibit RANKL-stimulated JNK phosphorylation (Figures 6j and k). By contrast, VnP-16 did not affect RANKL-induced phosphorylation of extracellular signal-regulated kinase or p38 (Figures 6j and k). Thus, suppression of JNK phosphorylation by VnP-16 resulted in a decrease of c-Fos and NFATc1 expression, which in turn led to the negative regulation of osteoclast differentiation.

VnP-16 suppresses cytoskeletal organizers in osteoclasts by disturbing αvβ3 integrin signaling

Because the average size of the M-CSF and RANKL-induced osteoclasts was reduced by VnP-16 (Figure 6c), we studied the effects of VnP-16 on the levels of αvβ3 integrin signaling-related molecules. PYK2 and c-Src are responsible for organizing the osteoclast cytoskeleton.30, 41, 42 Binding of a ligand to αvβ3 integrin activates c-Src by phosphorylating Tyr416, thereby leading to organization of the actin cytoskeleton,43 and engagement of c-Src and PYK2 with αvβ3 integrin is related to the resorptive function of mature osteoclasts.30, 41 Therefore, we suspected that αvβ3 integrin signaling might be involved in the inhibition of M-CSF- and RANKL-induced resorptive function by VnP-16. In BMMs, VnP-16 disturbed the M-CSF- and RANKL-induced phosphorylation of c-Src at Tyr416 and PYK2 at Tyr402 (Figures 7a and b). Similarly, VnP-16 inhibited and suppressed the phosphorylation of these proteins in preosteoclasts (Figures 7c and d) and mature osteoclasts (Figures 7e and f), respectively. Furthermore, VnP-16 altered the level of GTP-bound Rac1, the final molecular effector of αvβ3 integrin signaling, during M-CSF- and RANKL-induced osteoclastogenesis in BMMs (Figures 7g and h). Notably, unlike SP, VnP-16 inhibited GTP-bound Rac1 expression in preosteoclasts (Figures 7i and j). Taken together, these data demonstrate that VnP-16 suppresses αvβ3 integrin signaling-related molecules during the M-CSF- and RANKL-induced bone resorption process, thereby inhibiting cytoskeletal organization in osteoclasts.

Figure 7.

Figure 7

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The effects of VnP-16 on M-CSF- and RANKL-induced activation of cytoskeletal organizers during osteoclastogenesis. (a–f) Immunoblotting (a,c,e) and densitometric analyses (b, d and f) of c-Src, PYK2, and CREB in BMMs (a and b), preosteoclasts (c and d), and mature osteoclasts (e and f). The cells were cultured for 1 day (a and e) or 3 days (c) on plates that were precoated with SP or VnP-16 (9.1 μg/cm2), in the presence of 30 ng/ml M-CSF and 100 ng/ml RANKL, serum-starved for 3 h, and then stimulated with M-CSF (30 ng/ml) and RANKL (100 ng/ml) for the indicated times. (g–j) Immunoblotting (g and i) and densitometric analyses (h and j) of active (GTP-Rac1) and total Rac1 levels in BMMs (g and h) and preosteoclasts (i and j). The assay conditions were the same as those described for (a and c). The cells were lysed and incubated with PAK1 PBD Agarose beads for 1 h at 4 °C. Active Rac1 proteins were detected by immunoblotting using an anti-Rac1 antibody. Data in (b, d, f, h and j) represent the mean±SD (n=3)

VnP-16 inhibits bone resorbing activity of pre-existing osteoclasts and prevents interleukin-1α (IL-1α)-mediated bone loss in vivo

To assess the resorptive activity of pre-existing osteoclasts in vitro, mature osteoclasts were cultured on Osteo Assay Surface plates that were coated with vehicle, vitronectin, SP, or VnP-16, in the presence of M-CSF and RANKL. After 12 and 24 h, numerous resorption pits caused by osteoclasts were generated in the vehicle- and SP-treated controls; however, VnP-16 inhibited the area of these pits significantly (Figures 8a and b; Supplementary Figures S5a and b). VnP-16, however, had no effect on osteoclast survival (Supplementary Figure S5c).

Figure 8.

Figure 8

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The effects of VnP-16 on bone resorbing activity in vitro and IL-1-induced bone destruction in vivo. (a and b) The effects of VnP-16 on the bone resorbing activity of mature osteoclasts. The assay conditions were the same as in Figure 6e, except that mature osteoclasts cultured for 12 h on Osteo Assay Surface plates were used (a). Bone resorption was assessed by pit area measurements (b). Scale bars, 200 μm. (c–e) The effects of VnP-16 on IL-1-induced bone destruction in vivo. A collagen sponge treated with vehicle (DMSO), IL-1 (2 μg), synthetic peptides (125 μg), or synthetic peptides (125 μg) plus IL-1 (2 μg) was implanted over the calvarial bone of 5-week-old ICR mice. TRAP staining and μCT imaging of whole calvariae were performed (c); the black spots indicate eroded surfaces. Bone mineral content (d) and BV/TV (e) were measured by quantitative bone morphometric analysis. (f–h) Histological sections of calvarial bones were stained with H&E (f, bottom) and histochemically for TRAP (f, top). The osteoclast number (g) and surface area (h) were determined by histomorphometric analysis. Oc.N, osteoclast number; Oc.S, osteoclast surface. Scale bars, 200 μm. Data in (b, d, e, g and h) represent the mean±SD (n=5 per group). *P<0.05, **P<0.01

To ascertain the biological potency of VnP-16 on bone resorption in vivo, we investigated the effects of VnP-16 on IL-1α-induced bone destruction in mice. μCT images and TRAP staining of whole calvariae revealed that IL-1α treatment resulted in severe bone destruction (Figure 8c). Compared with that in the IL-1α- plus SP-treated group, bone destruction was significantly lower in the IL-1α- plus VnP-16-treated group (Figure 8c). Furthermore, IL-1α decreased the mineral content and BV/TV of calvarial bones, and these effects were significantly less pronounced in the VnP-16-treated group than the SP-treated group (Figures 8d and e). Histological and histomorphometric analyses of calvarial bones showed that IL-1α increased the number and its surface area of TRAP-positive osteoclasts; however, VnP-16 significantly reduced these IL-1α-induced parameters (Figures 8f–h).

VnP-16 substantially reverses estrogen deficiency-induced bone loss

To explore whether VnP-16 restored bone loss in vivo, we examined whether it could reverse the established bone loss induced by ovariectomy (OVX) in mice. We found that OVX mice displayed noticeable trabecular bone loss (Supplementary Figure S6a). Quantitatively, bone mineral density (BMD), BV/TV, trabecular number, and osteoblast number were significantly reduced (Supplementary Figures S6b–e), but the number and its surface area of TRAP-positive osteoclasts were significantly increased (Supplementary Figures S6f and g) in mice at 12 weeks following OVX, demonstrating that OVX induces severe bone loss in the femur. Next, to evaluate the therapeutic value of VnP-16, we administered synthetic peptides, rhBMP-2, or vehicle to OVX mice once via intra-femoral injection, waited for 1 week, and then performed μCT analysis and histological staining of femurs from these mice. VnP-16-treated OVX mice showed marked bone restoration (Figure 9a) and significantly higher degrees of BMD (Figure 9b), BV/TV (Figure 9c), and trabecular number (Figure 9d) than vehicle- or SP-treated OVX mice. Similarly, Masson’s trichrome staining confirmed that VnP-16 enhanced osteoid formation in vivo (Figure 9e). In this regard, rhBMP-2 also had a strong bone anabolic effect in OVX mice; surprisingly, the bone-restorative effect of VnP-16 in OVX mice was similar to that of rhBMP-2 (Figures 9a–e), which is known as the most effective osteoinductive protein. Quantitatively, VnP-16 and rhBMP-2 restored 42% and 29% of the BMD, respectively, compared with vehicle- or SP-treated OVX mice (Figure 9b).

Figure 9.

Figure 9

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VnP-16 substantially alleviates osteoporosis by reversing OVX-induced bone loss. (a–d) μCT reconstruction of metaphyses of distal femurs (a) as well as BMD (b), BV/TV (c), and trabecular number (d) in OVX mice at 1 week after administration of vehicle, rhBMP-2, SP, or VnP-16. The images represent femurs (a, upper panel) and its trabecular bones (a, lower panel) of vehicle-, rhBMP-2-, or peptide-treated OVX mice. (e and f) Masson’s trichrome (e) and H&E (f) staining of femur sections from OVX mice at 1 week after administration of vehicle, rhBMP-2, SP, or VnP-16. Scale bars, 200 μm. (g and h) Morphometric analysis of the osteoblast number (g) and osteoblast surface (h) in OVX mice at 1 week after administration of vehicle, rhBMP-2, SP, or VnP-16. (i) TRAP staining of osteoclasts surrounding trabecular bones in OVX mice at 1 week after administration of vehicle, rhBMP-2, SP, or VnP-16. Scale bars, 200 μm. (j and k) Morphometric analysis of the osteoclast number (j) and osteoclast surface (k) in OVX mice at 1 week after administration of vehicle, rhBMP-2, SP, or VnP-16. (l) Proposed pathway for reversing estrogen deficiency-induced bone loss by a vitronectin-derived peptide VnP-16. OB, osteoblasts; OC, osteoclasts; M, bone marrow-derived macrophages. Data in (b–d, g, h, j and k) represent the mean±SD (n=7 per group). *P<0.05, **P<0.01

To further evaluate whether the marked bone restoration induced by VnP-16 treatment is primarily due to either osteoblastogenesis or inhibition of osteoclastogenesis, we examined the ability of VnP-16 to generate osteoblasts and osteoclasts from femoral trabecular bone in OVX mice. Hematoxylin and eosin (H&E) staining and histomorphometric analysis revealed that the osteoblast number was significantly higher and the osteoblast surface was significantly larger in VnP-16-treated OVX mice than in vehicle- or SP-treated OVX mice (Figures 9f–h). By contrast, the osteoclast number was significantly lower and the osteoclast surface was significantly smaller in VnP-16-treated OVX mice than in vehicle- or SP-treated OVX mice (Figures 9i–k). Quantitatively, the osteoblast number was 2.4-fold higher but the osteoclast number was 0.5-fold lower in VnP-16-treated OVX mice than in vehicle-treated OVX mice (Figures 9g and j).

Discussion

In this study, we performed a series of in vitro and in vivo studies to demonstrate that the vitronectin-derived VnP-16 peptide could be an attractive therapeutic agent for the treatment of osteoporosis by blocking bone catabolism and promoting bone anabolism (Figure 9l). Using three different, but complementary, animal models, we demonstrated that VnP-16 could enhance bone regeneration in rat calvarial critical-sized bone defects by promoting osteoblast differentiation and increasing osteoblast number, and alleviate IL-1α-induced bone resorption by restraining osteoclast differentiation and function. Moreover, VnP-16 could reverse OVX-induced bone loss by both inhibiting bone resorption and promoting bone formation. In vivo, both osteoblastogenesis and inhibition of osteoclastogenesis actively occurred to an almost equal extent in VnP-16-treated OVX mice, although the level of the former was slightly higher than that of the latter. In addition, VnP-16 did not promote the attachment of primary human keratinocytes, which suggests that it effectively enhances the bone regeneration capacity without causing epithelial migration. Notably, periodontal regeneration can only be achieved when epithelial migration on the treated root surface is prevented.44, 45

To further elucidate the molecular mechanism by which VnP-16 inhibited bone resorption and promoted bone formation, we examined each key step of osteoblast and osteoclast differentiation and how they were affected by this peptide in vitro. VnP-16 inhibited osteoclastogenesis and bone resorption by suppressing JNK-c-Fos-NFATc1-induced osteoclast differentiation and αvβ3 integrin-c-Src-PYK2-mediated resorptive function, while it promoted bone formation by enhancing osteoblast differentiation via direct interaction with β1 integrin. Therefore, VnP-16 holds promise as a potential therapeutic agent for osteoporosis. Peptides can elicit different responses depending on their receptors and the cellular context. VnP-16, which is predicted to have two β-strands, promoted osteogenic cell functions through β1 integrin by inducing phosphorylation of FAK at Tyr-397 and -577, and c-Src at Tyr416; in fact, FAK activation by VnP-16 was crucial for osteoblast differentiation. Consistent with this, the rapid phosphorylation of FAK at Tyr397 is a hallmark of FAK activation upon integrin-mediated cell attachment and spreading.46

NFATc1 induction is dependent on both the TRAF6-NF-κB and c-Fos pathways, which are activated by RANKL and Ca2+ signaling.22, 25 Here we found that VnP-16 restrained JNK phosphorylation, leading to the suppression of c-Fos and NFATc1, downstream regulators of JNK, during osteoclastogenesis. To explain the VnP-16-mediated osteoclast function, we also examined the effect of this peptide on αvβ3 integrin signaling. The involvement of c-Src in osteoclast function has been validated by studying osteopetrotic Src-deficient mice.47 The interaction of PYK2 with αvβ3 integrin leads to c-Src-dependent phosphorylation at Tyr402 and subsequent activation of PYK2.30, 41 The data presented here show that VnP-16 disturbed or inhibited M-CSF- and RANKL-induced activation of cytoskeletal organizers during osteoclastogenesis. The anti-osteoclastogenic activity of VnP-16 was confirmed by its ability to suppress F-actin-mediated cytoskeletal organization. Moreover, VnP-16 decreased the bone resorbing activity of pre-existing mature osteoclasts without changing their survival rate. Thus, these data reveal the precise mechanism by which VnP-16 affects osteoclast differentiation and function, including the resorptive activity of mature osteoclasts, thereby inhibiting bone resorption.

Most drugs currently used to treat osteoporosis are inhibitors of bone resorption; however, they cannot reverse the substantial bone loss that has already occurred by the time of diagnosis.48 Therefore, a better treatment strategy for osteoporosis would not only block bone resorption, but also promote bone formation while controlling local inflammation.48, 49 Our results suggest that the simultaneous inhibition of bone resorption and promotion of bone formation by VnP-16 make it a better, and perhaps safer, therapeutic agent for the treatment of osteoporosis.

Materials and methods

More in Supplementary Materials and Methods.

Peptides and reagents

All peptides were synthesized on a Pioneer Peptide Synthesizer (Applied Biosystems, Foster City, CA, USA) using the 9-fluorenylmethoxycarbonyl-based solid-phase method with a C-terminal amide. The peptides were purified and characterized by Peptron (Daejeon, Korea). All the peptides used in the study had a purity greater than 95%, as determined using high-performance liquid chromatography. Human plasma vitronectin was purchased from Millipore (Bedford, MA, USA).

Preparation of human primary cells, osteogenic cells, and BMMs

NHEKs, NHOKs, NHDFs, and NHOFs were prepared and maintained as described previously.50, 51 To prepare human osteogenic cells, multipotent SKPs were isolated from human foreskins of 1–3-year-old patients undergoing surgery, as described previously.52, 53 For the serial sphere formation assay, subculturing was performed once a week for 3 weeks after dissociation of the spheres with Accutase solution (Innovative Cell Technologies, San Diego, CA, USA). The SKPs were then differentiated into mesenchymal precursors, as described previously.53 To obtain BMMs, bone marrow cells were collected by flushing the tibiae and femurs of 6-week-old male C57BL/6 mice. After removing the red blood cells with ACK buffer (0.01 mM EDTA, 0.011 M KHCO3, and 0.155 M NH4Cl, pH 7.3), the cells were cultured on 100-mm culture dishes in α-MEM complete media containing 10% fetal bovine serum (FBS), 100 U/ml penicillin, 100 μg/ml streptomycin, and 10 ng/ml M-CSF. Cells that did not attach to the culture plates were incubated with 30 ng/ml mouse M-CSF for a further 3 days, and the adherent cells were used as BMMs. All procedures for obtaining human tissue specimens were reviewed and approved by the Institutional Review Board on Human Subjects Research and the Ethics Committee at Seoul National University Dental Hospital (approval number: CRI12004G).

Osteoclast differentiation assay

To generate osteoclasts from BMM cultures, BMMs (2 × 105 cells/well) were cultured for 6 days on 48-well culture plates coated with vehicle (DMSO), vitronectin (0.23 μg/cm2), or synthetic peptides (9.1 μg/cm2), in the presence of 30 ng/ml M-CSF and 100 ng/ml mouse soluble RANKL. The complete medium was changed on days 3 and 5. After culturing, the cells were fixed and stained for TRAP–a marker enzyme of osteoclasts.

Cell attachment and spreading assays

Cell attachment assays were performed as described previously.54 Briefly, 48-well culture plates were coated with human plasma vitronectin (0.23 μg/cm2) or rVn-FII (5.7 μg/cm2) for 24 h at 4 °C. Peptides (9.1 μg/cm2) were also adsorbed onto plates by drying for 24 h at room temperature. The concentrations of the recombinant protein and synthetic peptides were determined from a dose–response curve, and the lowest concentration that achieved maximum attachment to human osteogenic cells was used. The concentration of human plasma vitronectin was determined according to the manufacturer’s instructions. Substrate-coated plates were blocked with 1% heat-inactivated bovine serum albumin (BSA) in phosphate-buffered saline (PBS) for 1 h at 37 °C, and then washed with PBS. Cells (5 × 104 cells/250 μl) were added to each plate and incubated for 1 h at 37 °C. After the incubation, the unattached cells were removed by rinsing the plates twice with PBS. The attached cells were fixed with 10% formalin for 15 min and stained with 0.5% crystal violet for 1 h. The plates were gently washed three times with double-distilled water (DDW), after which the content of each well was solubilized in 2% SDS for 5 min. The absorbance at 570 nm was measured using a microplate reader. For cell-spreading assays, the cells (3 × 104 cells/250 μl) were added to each substrate-coated plate and incubated for 3 h at 37 °C. The attached cells were fixed with 10% formalin and then stained with 0.5% crystal violet for 1 h. The plates were gently washed three times with PBS. Cell spreading was assessed by measuring the surface areas of the cells with Image Pro Plus software (version 4.5; Media Cybernetics, Silver Spring, MD, USA).

Attachment inhibition assay

The cells (5 × 104 cells/250 μl) were preincubated with 5 mM EDTA, 500 μM MnCl2, 100 μg/ml heparin, and 10 μg/ml function-blocking antibodies against the integrin subunits α1 (FB12), α2 (P1E6), α3 (P1B5), α4 (P4C2), α5 (P1D6), α6 (NKI-GoH3), β3 (B3A; Chemicon, Temecula, CA, USA), αv (AV1), or β1 (6S6; Millipore) for 15 min at 37 °C. The preincubated cells were transferred to plates that were coated with VnP-16 (9.1 μg/cm2) and incubated for 1 h at 37 °C. The attached cells were then quantified as described elsewhere.

TUNEL assay

Apoptosis was analyzed in situ by the TUNEL assay using the In Situ Cell Death Detection Kit, Fluorescein (Roche Applied Science, Mannheim, German) according to the manufacturer’s instructions. To ensure a representative count, each cell culture slide was divided into quarters, and at least two fields were photographed with Olympus BX 50 fluorescence microscope. The number of apoptotic cells was measured by counting the TUNEL-positive cells. Average number and standard deviation were calculated from four independent experiments.

Determination of peptide secondary structures

The secondary structures of the rVn-FII truncation and VnP-16 peptide were analyzed using the PSIPRED protein structure prediction server (http://bioinf.cs.ucl.ac.uk/psipred/).55

Histological staining

Histological staining of osteogenic cells was performed as described previously.56 Briefly, to visualize mineral deposits, the cells were fixed with ice-cold 95% ethanol for 30 min at −20 °C, and then stained with 40 mM Alizarin red S solution (pH 4.2) for 1 h. The stained cells were washed five times with DDW and then rinsed with PBS for 15 min.

Immunoblotting

Human osteogenic cells (1 × 106) were plated onto 60 mm dishes that had been precoated with vitronectin (0.23 μg/cm2) or synthetic peptides (9.1 μg/cm2), and allowed to adhere for 3 h. The cells were then washed with ice-cold PBS and lysed with 150 μl RIPA buffer (50 mM Tris-HCl, pH 7.4, 150 mM NaCl, 1 mM EDTA, 1% Triton X-100, 1 mM PMSF, 2 mM Na3VO4, and 1 mM glycerol phosphate) containing a protease inhibitor cocktail. The proteins present in the RIPA lysates were denatured using SDS sample buffer, resolved by SDS-PAGE, and electroblotted onto nitrocellulose membranes. The membranes were immunoblotted with primary antibodies against focal adhesion kinase (FAK; Upstate Biotechnology, Lake Placid, NY, USA); FAK [pY397], [pY407], [pY576], [pY577], or [pY861] (Invitrogen, Carlsbad, CA, USA); or actin (Sigma-Aldrich, St. Louis, MO, USA). All blots were then incubated with anti-rabbit horseradish peroxidase-conjugated secondary antibodies (Cell Signaling Technology, Danvers, MA, USA). The signals were detected by electrochemiluminescence. The ratio of target protein to total protein or β-actin for each sample was then calculated to correct for differences in protein loading. This ratio was normalized to the target protein/total protein or β-actin ratio of the negative controls to obtain the relative levels of protein.

Transfection

A nonspecific control siRNA (Invitrogen), and siRNAs against human FAK (Sigma-Aldrich) or β1 integrin (Santa Cruz Biotechnology Inc., Santa Cruz, CA, USA) were used for gene silencing. Human osteogenic cells were plated into 100 mm dishes at a density of 1.5 × 105 cells per dish, cultured for 1 day, and then transfected with 10, 50, or 100 nM FAK siRNA, 10 nM β1 integrin siRNA, or 10 or 100 nM control siRNA using 15 μl of Lipofectamine RNAiMAX transfection reagent (Invitrogen).

Pull-down assay of biotin-labeled peptide

Pull-down assays were performed as described previously57 with biotinylated SP and biotinylated VnP-16 peptides. Cells (3 × 106 cells) were seeded onto 100-mm dishes coated with biotin-conjugated peptides (9.1 μg/cm2) for 30 min and washed twice with cold PBS. Cells were scraped with 500 μl lysis buffer (50 mM Tris-HCl, pH 7.5, 150 mM NaCl, 0.1% sodium deoxycholate, 1% Triton X-100, protease, and phosphatase inhibitor cocktail tablets), followed by passing the lysates 15 times through a 26.5-gauge needle and then spinning at 17,000 × g for 10 min at 4 °C. The supernatants were incubated with 60 μl of streptavidin agarose beads (Thermo Scientific, Rockford, IL, USA) for 16 h at 4 °C and spun at 1,500 × g for 2 min at 4 °C. After washing the beads four times with lysis buffer, the precipitated proteins were resolved by 8% SDS-PAGE and analyzed by immunoblotting.

TRAP staining

The TRAP assay was performed using the Leukocyte Acid Phosphatase Assay Kit (Sigma-Aldrich), according to the manufacturer’s instructions. Briefly, the cells were washed, fixed with 10% formalin, and stained with 40 mM sodium tartrate. TRAP-positive multinucleated cells containing more than three nuclei were considered to be osteoclasts.

Bone resorption assay

Mature osteoclasts were prepared from co-cultures of bone marrow cells and primary osteoblasts on collagen gel-coated culture dishes, as described previously.58 For the bone resorption assay, BMMs and mature osteoclasts were cultured on Osteo Assay Surface plates (Corning) for 6 days and 12 h, respectively, coated with vehicle (DMSO), vitronectin (0.23 μg/cm2), or synthetic peptide (9.1 μg/cm2) in the presence of 30 ng/ml M-CSF and 100 ng/ml RANKL. The cells were removed using 10% Clorox (0.56% NaOCl), and the resorbed pits were photographed and analyzed using the Image Pro-Plus program (version 4.0; Media Cybernetics).

Animal experiments

Critical-sized calvarial defects were generated in 8-week-old male Sprague–Dawley rats (n=5 per group). Absorbable collagen sponges (BiolandKorea, Cheonan, Korea) were loaded with rhBMP-2 (2 μg per scaffold, 15 μl volume; Pepro-Tech, Rocky Hill, NJ, USA), synthetic peptides (1 mg per scaffold, 15 μl volume), or vehicle (10 μl of DMSO and 5 μl of DDW). The surgical procedures to perforate an 8 mm circular defect in the parietal bone and implantation of the collagen sponge were performed as described previously.38 The rats were euthanized 2 weeks after surgery, and whole calvariae were fixed in 4% paraformaldehyde for 24 h at 4 °C and then analyzed by μCT scanning. For histomorphometric analysis, the specimens were decalcified with 12% EDTA for 4 weeks and embedded in paraffin. The paraffin-embedded samples were sectioned at a thickness of 4 μm and then stained with Masson’s trichrome.

To study the effects of VnP-16 on IL-1α-induced mouse calvarial bone loss, dried collagen sponges loaded with IL-1α (2 μg), synthetic peptides (125 μg), synthetic peptides (125 μg) plus IL-1α (2 μg), or vehicle (DMSO) were implanted over the calvarial bones of 5-week-old male ICR mice (n=5 per group). The mice were sacrificed on day 7 and the whole calvariae were dissected, cleaned of soft tissue, and fixed in 4% paraformaldehyde for 24 h at 4 °C. TRAP staining and μCT scanning were then performed.

To study the effects of VnP-16 on OVX-induced bone loss in mice, female C57BL/6 mice were ovariectomized at 8 weeks of age. The mice were maintained under standard animal housing conditions (12-h light 12-h dark cycles and free access to food and water). At 12 weeks after surgery, rhBMP-2, synthetic peptides, or vehicle was injected intrafemorally after anesthetizing the mice with an intraperitoneal injection of a mix of 31.25 mg/kg tiletamine/zolazepam and 8.75 mg/kg xylazine (n=7 per group). Both hind limbs were shaved and sterilized with 70% ethanol. The knee was held in a flexed position, and a total volume of 5 μl of rhBMP-2 (2 μg), synthetic peptides (50 μg), or vehicle (50% DMSO) was injected intrafemorally through the knee joint into the medullary cavity using a 10 μl Hamilton syringe and a 31-gauge needle. The needle was withdrawn and the leg immediately straightened and held straight for ~1 min. The mice were killed on day 7, and the bilateral femurs were dissected, cleaned of soft tissue, and fixed in 4% paraformaldehyde at 4 °C for the subsequent ex vivo analysis. TRAP staining and μCT scanning were then performed.

The μCT scans were performed using the Micro-CT Skyscan 1172 system (70 kV, 141 μA, and 38 min integration time; SkyScan, Kontich, Belgium). The scans were integrated into 3D voxel images (2000 × 1048 pixel matrices), and bone images were reconstructed using the NRecon program (version 1.6.9.8; Bruker microCT, Kontich, Belgium). The regenerated bone volume, BMD, and bone mineral content were calculated with CT-Analyser (version 1.14.4.1; Bruker-microCT). The bone recovery rate (%) and calvarial thickness (mm) were also calculated using CT-Analyser according to standardized protocols. H&E, TRAP, and Masson’s trichrome staining were performed with 5-μm paraffin sections. The percentage of the osteoclast surface and the osteoclast number were calculated with OsteoMeasure XP (version 1.01; OsteoMetrics, Decatur, GA, USA), according to standardized protocols. All animal procedures were reviewed and approved by the animal care committee of the Institute of Laboratory Animal Resources of Seoul National University (approval numbers: SNU-130204-1-2, SNU-140917-3, and SNU-151104-4).

Statistical analyses

All data are presented as the mean±SD. The statistical analyses were performed using the STATISTICA 6.0 software package (StatSoft, Tulsa, OK, USA). Results were compared using analysis of variance tests. When significant differences were found, pairwise comparisons were performed using Scheffé’s adjustment. Statistical significance was also calculated using a two-tailed Student’s t-test. A P value of <0.05 was considered significant.

Acknowledgments

We thank Won Jong Jin (Seoul National University) for useful discussions and technical assistance. This work was supported by the Mid-career Researcher Program through a grant from the National Research Foundation of Korea, funded by the Ministry of Science, ICT and Future Planning, Korea government (2016R1A2B2007246), and the Korea Healthcare Technology R&D Project, funded by the Ministry for Health, Welfare & Family Affairs, Republic of Korea (HI15C2455; to B-MM).

Footnotes

Supplementary Information accompanies this paper on Cell Death and Differentiation website (http://www.nature.com/cdd)

Edited by P Bouillet

The authors declare no conflict of interest.

Supplementary Material

Supplementary Information
Click here for additional data file. (889.3KB, pdf)

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