Calcitonin gene-related peptide enhances osteogenic differentiation and recruitment of bone marrow mesenchymal stem cells in rats.

The present study evaluated the effects of calcitonin gene-related peptide (CGRP) on bone marrow mesenchymal stem cells (BMMSCs) in vitro and in a rat model of mandibular distraction osteogenesis (MDO). Rat BMMSCs were isolated then treated with CGRP or CGRP antagonist (CGRP8-37). The proliferation and migration ability of BMMSCs was determined using 5-bromo-2'-deoxyuridine and Transwell assays, respectively. Osteogenic-related gene expression was analyzed with reverse transcription-quantitative polymerase chain reaction. For the in vivo analysis, thirty MDO rats were randomly assigned to control, CGRP or CGRP8-37 groups. To evaluate the mobilization of BMMSCs, nestin and stromal cell-derived factor 1 (SDF-1) were detected by immunohistochemistry and ELISA. Rats were sacrificed following 14 days and new bone formation was assessed by histological and micro-computed tomography analysis. In the in vitro results, the CGRP group demonstrated significantly higher migration and proliferation, as well as enhanced alkaline phosphatase and runt-related transcription factor 2 expression compared with the control. In the in vivo experiments, bone mineral density of the newly formed bone in the CGRP group was significantly higher than controls. The nestin and SDF-1 expression in the CGRP group was also significantly upregulated. In conclusion, the present study demonstrated that CGRP administration increased new bone formation, possibly via enhancing BMMSC migration and differentiation in MDO rats.

Introduction

Craniofacial defects can be caused by inflammation, trauma, tumor and congenital malformations amongst other things. For reconstruction of defects or deformities in oral and maxillofacial regions, distraction osteogenesis (DO) techniques have been broadly applied to regenerate bone tissues and are considered to be the gold-standard treatment. However, the longer period required for bone consolidation may lead to clinical complications such as fracture of the distraction device or infections (1). Therefore, acceleration of bone formation is urgently required.

The nervous system has been demonstrated to have pivotal regulatory effects on the metabolism and repair of bones (2,3). Damage to peripheral nerves is often followed by osteoporosis (4). Our previous study reported that a locally applied nerve growth factor (NGF) promotes the rehabilitation of the inferior alveolar nerve (IAN) (5). In addition, delivery of human NGFβ in gels accelerates bone regeneration in DO rabbit models (6). Skeletal sensory terminals can secrete various neurotransmitters including substance P, calcitonin gene-related peptide (CGRP), which regulates the metabolism of osteoblasts and osteoclasts (7,8). In a bilateral periodontal defect model, the osteoprotegerin expression levels decrease along with CGRP when rats undergo transection of the left inferior alveolar nerve (9). Furthermore, the secretion of CGRP from sensory peptidergic fibers in the periosteum and bone is functional during load-induced bone regeneration (10). However, it remains unclear whether CGRP accelerates bone regeneration in DO by targeting bone marrow mesenchymal stem cells (BMMSCs). CGRP8-37 is the most widely used selective pharmacological antagonist of CGRP (11). In the present study, the effects of CGRP and CGRP-37 on BMMSCs were investigated in vitro and in vivo in a rat model of mandibular DO.

Materials and methods

Rat BMMSC culture and identification

A total of 4 male Sprague-Dawley rats (6 weeks old; 60–80 g) from the animal care center of the Fourth Military Medical University were housed under specific pathogen-free conditions (22°C; 12-h light/dark cycle; 50% humidity) with free access to food pellets and tap water. Briefly, rats were sacrificed and mandibles were resected aseptically (12,13). The cell suspension was prepared by repeated aspiration through a 20-gauge needle. The collected cells were then seeded into 6 well plates at a density of 1×106 cells per well and incubated under standard conditions (5% CO2, 37°C). The culture medium consisted of α-minimum essential medium (αMEM) supplemented with 10% (v/v) fetal bovine serum (FBS), 0.25 µg/ml Fungizone, and 1% (v/v) penicillin and streptomycin (all purchased from Sigma-Aldrich; Merck KGaA).

To characterize rat BMMSCs, the morphology of adherent BMMSCs was observed using a phase contrast microscope (Nikon TE 2000-U; Nikon Corporation). Immunofluorescence staining of MSC markers thy-1 cell surface antigen (CD90) and integrin subunit β1 (CD29) was performed using a standard procedure. Cells were fixed for 30 min at room temperature in 4% paraformaldehyde, washed twice with PBS then treated with 0.1% Triton X-100 at room temperature for 1–2 min to permeate the cell membrane. In brief, cells were blocked with 5% bovine serum albumin (BSA)/PBS (1 h, 25°C), then incubated in 1% BSA/PBS with either isotype controls, anti-CD29 (cat. no. 610468; 1:1,000; BD Biosciences) or anti-CD90 antibodies (cat. no. 554893; 1:1,000; BD Biosciences) for 12 h at 4°C. The cells were then washed three times with 0.5% BSA/PBS. Samples were then incubated in TRITC goat anti-rabbit fluorescent secondary antibody (cat. no. 150077; 1:200; Abcam). Stained cells were observed using a fluorescence microscope (magnification, ×400; DXM 1200F; Nikon Corporation). In addition, the multidifferentiation potential of rat BMMSCs was determined using adipogenic or osteogenic media followed by Oil Red (Sigma-Aldrich, Merck KGaA) or Alizarin Red staining (ARS) (Sigma-Aldrich; Merck KGaA), respectively.

Mineralization assay

ARS is used to quantify calcium within the deposited mineral matrix. Following 3 weeks of culture, cells were stained with 2% Alizarin red for 10 min. When bound to the calcium salts in cell matrix, Alizarin red was eluted with 10% cetylpyridinium chloride. The absorbance of supernatant aliquots (~150 µl) were measured at 540 nm using a spectrophotometer then standardized with the absorbance of crystal violet staining at 590 nm.

Cell proliferation assessment

BMMSCs at passage 3 were cultured with α-MEM containing 10−7 mol/l CGRP, α-MEM medium containing 10-7 mol/l CGRP8-37 or α-MEM medium only. 5-bromo-2′-deoxyuridine (BrdU; 3.1 µg/ml) was added at 72 h post-seeding then incubated for 4 h. After washing in PBS, cultures were fixed in ice-cold 70% ethanol for 10 min and denatured in 4 mmol/l HCl for 20 min. Samples were then incubated with mouse anti-BrdU primary antibody (cat. no. 5292S; 1:1,000; Cell Signaling Technology, Inc.) for 1 h at 37°C and then with HRP-conjugated second antibodies (cat. no. 7076S; 1:200; Cell Signaling Technology, Inc.) for 1 h at RT. The samples were washed then stained with diamino-benzidine (DAB) and hematoxylin for nuclei staining. Cell proliferation was measured as a percentage of BrdU+ cells relative to the total number of nuclei. Images were captured in 5 randomly selected fields per slide (magnification, ×200). The BrdU+ cells were counted manually by an experienced pathologist. All the experiments were conducted in triplicate.

Alkaline phosphatase (ALP) activity

Cultured BMMSCs were fixed in fresh 10% neutral buffered formalin at week 1, 2, and 3. Then ALP activity was determined by the commercial ALP activity kit. After all protocols were performed according to the manufacturer's instructions, the absorbance was measured at 410 nm with a spectrophotometer and the cell number was counted using crystal violet staining as previously reported (14,15,16).

Animal study

A total of 30 male Sprague-Dawley rats (10 weeks old; 100–120 g) from the animal care center of the Fourth Military Medical University were randomly divided into three groups: control, CGRP and CGRP8-37. The rats were housed under specific pathogen-free conditions (22°C; 12-h light/dark cycle; 50% humidity) with free access to food pellets and tap water. This study was specifically approved by the Institutional Ethics Committee at the Fourth Military Medical University (approval number ky-034). All animals were cared for according to the guidelines published by the Animal Center for Medical Experiment at Fourth Military Medical University.

Surgical procedures

Animals were anaesthetized with 1% pentobarbital sodium (intraperitoneal injection 30 mg/kg). A vertical osteotomy was made in the right mandible between the molar region and the mandibular ramus. Surgeries were performed cautiously to avoid damage in the IAN. A custom-made distraction device was fixed along a plane perpendicular to the osteotomy cut. The device was activated following a latency period of 5 days, and the distraction was carried out at the rate of 0.2 mm, twice per day for 10 days. During the distraction period, the CGRP group received a daily CGRP injection (Sigma-Aldrich; Merck KGaA; 10−8 mmol/l, in normal saline, total volume of 0.2 ml), the CGRP8-37 group was given a daily injection of CGRP8-37 (Sigma-Aldrich; Merck KGaA; 10−6 mol/l, in normal saline, total volume of 0.2 ml), and the control group received normal saline (17). All the drugs were injected into the local callus at the distraction side percutaneously. Following 14 days of treatment, animals were sacrificed and mandibular tissues were collected for histological and micro-computed tomography (micro-CT) analysis. All the analyses were conducted blinded.

Micro-CT evaluation

All mandibular samples were examined with a Micro-CT system (Inveon CT; Siemens AG) at the standard resolution (1888×2048 pixels). Each mandibular sample included ~1,000 images with an isotropic voxel size of 15 µm. The scanning was set at 500 mA, 80 kV, and the integration time was 800 msec. The bone and accurate 3-dimensional data sets were isolated using the same optimal thresholds from all segmented images. The region of interest was defined as a rectangle of 2.5×10 mm covering the distraction gap. The micro-CT measurements contained both bone mineral density (BMD) and bone volume/total volume (BV/TV), which indicates the portion of the mineralized tissue in bony defects. The newly generated BV in the distraction gap was quantified and compared to the total distraction area. Following micro-CT evaluation, all samples underwent histological analysis.

BMD analysis and immunohistochemistry

The mandibular samples were fixed in 4% paraformaldehyde for 24 h and decalcified in 30% buffered formic acid for 7 days at room temperature. Following dehydration and cleaning, samples were stained with hematoxylin and eosin (H&E). Analysis of the histological sections was performed using the Image-Pro Plus analysis software (v11.0; Media Cybernetics, Inc.) by a single, unbiased examiner who was blinded in this study.

For immunohistochemistry, endogenous peroxidase activity was eradicated by 3% hydrogen peroxide for 10 min at room temperature. Then the tissue slices were permeabilized with 0.25% Triton X-100 in PBS for 30 min, and blocked in 5% fetal bovine serum in PBS, 2% glycine and 2% BSA for 1 h at room temperature. The slices were then incubated with anti-nestin primary antibodies (cat. no. 4760S; 1:1,000; Cell Signaling Technology, Inc.) overnight at 4°C, followed by incubation with horseradish peroxidase-conjugated secondary antibodies (1:200; cat. no. 150077; Abcam) for 1 h at room temperature. Samples were washed and then stained with diamino-benzidine (DAB). To quantify the proportions of nestin+ cells in bone generating areas, these areas, consisting of woven bones and fibrosis, were characterized by presence of bone trabeculae and osteoid rimmed osteoblasts within a bridging callus. Nestin+ cells were manually counted under a fluorescent microscope (DMLRB; Leica Microsystems, Inc.) in 5 random high-power fields (magnification, ×400) per slide. Each assay was performed in triplicate.

ELISA

Rat BMMSC supernatant was analyzed for stromal cell-derived factor 1 (SDF-1) using SDF-1 ELISA kit (cat. no. E-EL-R0922; Civic Bioscience Inc.) following the manufacturer's protocols.

Reverse transcription-quantitative polymerase chain reaction (RT-qPCR)

Total RNA was extracted from BMMSCs using the RNeasy Mini Kit (Qiagen, Inc.), then the purity and concentration were determined spectrophotometrically. For each sample, 1 µg of total RNA was reverse transcribed to cDNA using the PrimeScript™ RT reagent kit (Takara Bio, Inc.). The normalized cDNA was then amplified with SYBR Premix ExTM Taq II RT-PCR kit in Applied Biosystems 7,500 RT-PCR System. Thermocycling conditions were as follows: 95°C for 30 sec, followed by 40 cycles of 95°C for 5 sec and 60°C for 30 sec. mRNA expression was calculated as previously reported (18), with GAPDH used as the housekeeping gene. The primer sequences were as follows: SDF-1 forward, 5′-GAGAGCCACATCGCCAGAGC-3′ and reverse, 5′-GGATCCACTTTAATTTCGGGTCAA-3′; runt-related transcription factor 2 (Runx2) forward, 5′-CACTGGCGCTGCAACAAGA-3′ and reverse, 5′-CATTCCGGAGCTCAGCAGAATAA-3′; ALP forward, 5′-GCTCCCTTGTCTGGTCTTT-3′ and reverse, 5′-GGACGCCGTGAAGCAGGTGA-3′; and GAPDH forward, 5′-AGCCGCATCTTCTTTTGCGTC-3′ and reverse, 5′-TCATATTTGGCAGGTTTTTCT-3′.

Western blot analysis

Rat BMMSCs from cell culture were collected for western blot analysis. Proteins were extracted from the cells using Membrane protein isolation mammalian protein extraction reagent (Thermo Fisher Scientific, Inc.). Bicinchoninic acid assay was used to quantify protein concentration. A total of 25% volume of protein sample buffer was added, boiled for 5 min then proteins (50 µg loaded per lane) were separated via SDS-PAGE on an 8% gel. The separated proteins were then transferred to polyvinylidene difluoride membranes. Following blocking with 7% fat-free dry milk for 2.5 h at 4°C, the membranes were incubated with primary antibodies against ALP (cat. no. 194297; 1:1,000; Abcam) and Runx2 (cat. no. 12556S; 1:1,000; Cell Signaling Technology, Inc.) at 4°C overnight. Following primary incubation, membranes were incubated with horseradish peroxidase-conjugated IgG secondary antibody (cat. no. 150077; 1:200; Abcam) for 1 h. Membranes were then treated with enhanced chemiluminescent substrate (Thermo Fisher Scientific, Inc.) to visualize the bands. β-actin was used as an endogenous reference. Each experiment was performed three times.

Statistical analysis

The statistical analysis was performed by SPSS software (v.19.0; IBM Corp.) and the data were presented as mean ± standard deviation. One-way analysis of variance followed by the Neuman-Keuls post hoc test was used for analysis. P<0.05 was considered to indicate statistical significance.

Results

Effects of CGRP on osteogenic differentiation and proliferation in vitro

Using a well-established method, rat BMMSCs were isolated. It was determined that morphology was typically fibroblastic at P0 and spindle-like at P3 (Fig. 1A). Immunofluorescence staining demonstrated that rat BMMSCs were positive for MSC markers CD90 and CD29 (Fig. 1A). In addition, rat BMMSCs differentiated into adipocytes using adipogenic medium or osteoblasts using osteogenic medium, as indicated by Oil Red or ARS, respectively (Fig. 1A and B). The osteoblast phenotype of the control, CGRP and CGRP8-37 treatment groups was confirmed by the presence of matrix mineralization. After 21 days, osteogenic differentiation of BMMSCs was significantly enhanced by CGRP treatment and attenuated by CGRP8-37 (Fig. 1B and C). Runx2, SDF-1 and ALP mRNA expression levels were evaluated at 1, 3, 7, 14 and 21 days. mRNA expression began to rise from day 3 and peaked at day 14. At day 14, ALP expression in the CGRP group increased 4.2-fold (P<0.05; Fig. 1D), SDF-1 increased 3.8-fold (P<0.05; Fig. 1H) and Runx2 increased 3.2-fold (P<0.05; Fig. 1E), compared to day 1. ALP and Runx2 expression of cells was further validated using western blot analysis (Fig. 1F and G). ELISA analysis further confirmed that concentrations of SDF-1 significantly increased in the CGRP group at day 7 and 14 (P<0.05; Fig. 1I). The effect of CGRP on cell proliferation was assessed by the BrdU incorporation assay. CGRP significantly increased the percentage of BrdU+ BMMSCs over the total number of cells, whilst CGRP8-37 significantly decreased the percentage of BrdU+ BMMSCs (P<0.05; Fig. 2).

Figure 1.

Effects of CGRP on osteogenic differentiation and proliferation in vitro. (A) Stem cell identification of the cultured P3 bone marrow mesenchymal stem cells extracted from the rat mandible. (B) Alizarin Red staining and (C) quantification for in vitro osteogenic differentiation. (D) mRNA expression levels of ALP and (E) RUNX2 measured by RT-qPCR. Protein expression of (F) ALP and (G) RUNX2 measured by western blot analysis. (H) Gene expression of SDF-1 measured by RT-qPCR. (I) Concentration of SDF-1 in cell culture media. *P<0.05 vs. control; #P<0.05 vs. CGRP. CGRP, calcitonin gene-related peptide; ALP, alkaline phosphatase; RUNX2, runt-related transcription factor 2; RT-qPCR, reverse transcription-quantitative PCR; SDF-1, stromal cell-derived factor 1; BMMSCs, bone marrow mesenchymal stem cells; CD29, integrin subunit β1; CD90, thy-1 cell surface antigen; D, days.

Figure 2.

Effects of CGRP on osteogenic differentiation and proliferation in vitro. Micrographs demonstrating BrdU incorporation (brown staining) and hematoxylin (blue staining, nuclei). Quantification of BrdU+ cells. *P<0.05 vs. control; #P<0.05 vs. CGRP. CGRP, calcitonin gene-related peptide; BrdU, 5-bromo-2′-deoxyuridine.

Effects of CGRP on bone regeneration in vivo

All three groups demonstrated successful mandible lengthening. Micro-CT imaging determined that the distraction gaps were filled with newly formed bone in the control and CGRP groups, while only scattered bone trabeculae were present in the CGRP8-37 group (Fig. 3A). The BMD and BV/TV ratio in the CGRP group were significantly higher than other two groups, which indicated increased new bone generation (P<0.05; Fig. 3B and C). The morphology of new bone in the CGRP group was tighter and more continuous compared with the control group (Fig. 3D).

Figure 3.

Effects of CGRP on bone regeneration in vivo. (A) Micro-computed tomography micrographs of rat mandibles. (B) Quantification of BMD and (C) BV/TV. (D) Histology analysis of each group. *P<0.05 vs. control; #P<0.05 vs. CGRP. CGRP, calcitonin gene-related peptide; BMD, bone mineral density; BV, bone volume; TV, total volume.

HE staining demonstrated that there was no inflammation in any group. The CGRP group had a large amount of woven bone in the distraction axial direction, which is associated with osteoblasts and new blood vessels. In addition, the trabeculae were orderly arranged. The CGRP8-37 group exhibited increased fibrous connective tissues and fewer bone masses and trabeculae. The trabeculae were disorderly arranged in the CGRP8-37 group (Fig. 3B).

To further investigate the relationship between new bone and Nestin+ BMMSCs, immunohistochemistry was used to evaluate the migration of Nestin+ BMMSCs from the perivascular area to the DO gap. In the CGRP group, the Nestin+ BMMSCs were extensively distributed in bone generating areas of the callus whilst they were mainly distributed in the perivascular areas, rather than bone generating areas, in the other two groups (Fig. 4A). The number of Nestin+ cells in bone generating areas were notably higher in the CGRP compared with the control (P<0.05; Fig. 4A). In addition, SDF-1 expression in both the peripheral blood and regenerating region were significantly higher in the CGRP group compared with the other groups (P<0.05; Fig. 4B and C). These findings suggested that CGRP treatment improved the migration of BMMSCs from the perivascular area to bone generating areas.

Figure 4.

Effects of CGRP on bone regeneration in vivo. (A) Immunohistochemistry micrographs of Nestin+ BMMSCs (brown) with quantification of Nestin+ BMMSCs in the DO region. (B) SDF-1 expression in PB and (C) DO region. *P<0.05 vs. control; #P<0.05 vs. CGRP. CGRP, calcitonin gene-related peptide; BMMSCs, bone marrow mesenchymal stem cells; DO, distraction osteogenesis; PB, peripheral blood; SDF-1, stromal cell-derived factor 1; D, days.

Discussion

The present study investigated the effects of CGRP throughout DO in vivo, as well as proliferation, differentiation and migration of BMMSCs in vitro. A modified titanium distractor device, similar to previously described devices (19,20) was utilized to successfully establish the DO model. Micro-CT and histomorphometric analysis demonstrated that local injection of CGRP effectively increased and accelerated osteogenesis, whilst CGRP8-37 significantly impaired bone formation. In addition, Nestin+ cells in the DO gap and SDF-1 expression was significantly increased following CGRP administration, which suggested that CGRP promoted the recruitment of BMMSCs to the new bone generating area. To support the in vivo study, in vitro results demonstrated that CGRP treatment modulated bone metabolism in osteoprogenitor differentiation and maturation.

Neurotransmitters (e.g., substance P) have been proven to stimulate proliferation and osteogenic differentiation of MSCs in numerous animal models (29). Our previous study demonstrated that local injection of substance P accelerates the generation of bone during mandibular distraction in rats (21). Hong et al (8) demonstrated that systemic administration of substance P promotes the mobilization of BMMSC to the bone generating regions. Therefore, the present study hypothesized that CGRP may have an effect on sensory nerves serving a similar role in promoting the mobilization of MSCs akin to substance P.

CGRP belongs to the calcitonin superfamily of peptides consisting of calcitonin, amylin, adrenomedullin, adrenomedullin 2 (intermedin) and calcitonin-receptor-stimulating peptide. Calcitonin is mainly produced by thyroid C cells whilst CGRP is secreted and stored in the nervous system. Calcitonin can inhibit osteoclast motility and cause bone resorption disorders; however, there is limited evidence of the direct effect of calcitonin on osteoblasts. Notably, neuropeptides, such as CGRPs, are pivotal in suppressing bone resorption via the receptor activator of nuclear factor-κB/osteoprotegerin pathway (22). CGRPs are less potent than calcitonin in inducing hypocalcemia by several orders of magnitude (23,24) but it has been suggested that CGRP stimulates osteoblasts and bone formation. Activation of osteoblastic CGRP receptors enhances the proliferation of osteoblasts in vitro (25) and treatment of the osteocalcin promoter on transgenic mice resulted in an enhanced bone mass level (26). It has also been reported that exogenous CGRP can accelerate the proliferation of MSCs in the logarithmic growth phase (27). Furthermore, CGRP modulates the differentiation of SCs towards osteoblasts in vivo (28) and also regulates cell differentiation in the induced pluripotent and embryoid body stages (29). Therefore, CGRP has an important role in mediating osteoblasts in cellular and autocrine activities. The CGRP-containing fibers distribute abundantly in bone marrow and periosteum, which suggests a mechanistic connection between osteoblasts and CGRP-containing nerve fibers. In addition, CGRP-containing fibers in the epiphyseal trabeculae are rarely covered by the Schwann cell sheaths which may promote the interaction of BMMSCs with CGRP released from the fibers (29). Another characteristic of CGRP-containing fibers is their persistent contact with the bone surface. The links between CGRP-containing fibers and osteoblasts by the uncovered varicosities are maintained by bone generation. After bone injury or fracture, the CGRP-containing fibers may trigger bone regeneration around the blood vessels. However, CGRP mRNA and protein expression in osteoblasts has also been observed (28). Therefore, it is highly reasonable that CGRP may influence osteoblastogenesis and the metabolism of bone formation by regulating BMMSC activity. Our future work will determine other osteogenic markers and further investigate the molecular mechanisms underlying the role of CGRP in osteogenic differentiation and BMMSC recruitment.

In conclusion, the present study determined that CGRP could accelerate bone formation during DO. These findings may provide an insight into the mechanisms underlying bone regeneration promoted by sensory nerves, and also provides evidence for the efficiency and safety of DO treatment.