Involvement of CB2 signalling pathway in the development of osteoporosis by regulating the proliferation and differentiation of hBMSCs

Abstract

The aim of the present study was to explore the potential mechanism underlying the involvement of CB2 in osteoporosis. Micro‐CT was utilized to examine femur bone architecture. Also, real‐time PCR and Western blot analysis were utilized to detect the effect of 2‐AG on the expression of CB2 and Notch, or the interaction between CB2 and Notch 2. 2‐AG treatment up‐regulated BMD, Tb.Sp and SMI in OVX mice, whereas proportion of bone volume in total volume (BV/TV), trabecular thickness (Tb.Th), trabecular number (Tb.N) and bone mineral density (BMD) were decreased in 2‐AG‐treated OVX mice. Accordingly, 2‐AG administration up‐regulated Notch 1 expression in OVX mice but had no effect on CB2 and Notch 2 expression. Meanwhile, 2‐AG administration promoted the differentiation of hBMSCs in OVX mice, while exhibiting no effect on the proliferation of hBMSCs. Furthermore, in the cellular models, 2‐AG treatment also up‐regulated Notch 1 expression but had no effect on CB2 and Notch 2 expression, while Notch 1 shRNA had no effect on CB2 and Notch 2 expression. 2‐AG promoted cell proliferation and differentiation, which were inhibited by Notch 1 shRNA. NICD had no effect on CB2 level but increased Notch 1 expression, and CB2 shRNA decreased CB2 and Notch 1 expression. Finally, CB2 shRNA inhibited cell proliferation and differentiation, whereas NICD promoted proliferation and differentiation of hBMSCs. Our results provided further evidence for the association of CB2 gene with BMD and osteoporosis, and identified CB2 as a promising target for the treatment of osteoporosis.

1. INTRODUCTION

According to the description of World Health Organization (WHO), osteoporosis is a progressive disorder featured by microarchitectural deterioration of bone tissues and low bone mass, with a subsequent elevation in bone fragility and proneness to fracture. ¹ Several recent studies explored the differentiation of hBMSCs towards osteoblasts or the differentiation of haematopoietic stem cells towards osteoclasts. Some reports indicated that, compared with cells from non‐osteoporotic controls, hBMSCs from osteoporotic patients have less osteogenic capacity and show adipogenesis instead of osteogenesis. ² However, other reports revealed that in both groups, hBMSCs upon chemically triggered differentiation exhibit the same level of differentiation. ³

The Notch signalling pathway (NSP) is highly conserved and related to apoptosis, self‐renewal potential, and cell‐fate determination. ⁴ NSP was identified to be implicated in the proliferation and differentiation of hBMSCs. The study conducted by Ugarte et al indicated that NS suppressed adipocyte differentiation and promoted osteoblast differentiation of hBMSCs. ⁵ Moreover, NS was shown to be associated with the differentiation of BMSCs into other types of cells. The levels of a range of neuron‐specific indicators were elevated when the production of Notch 1 was blocked by mNotch‐1 shRNA, indicating that NS plays a critical role in the BMSC differentiation into neurons in vitro. ⁶ Other studies also found that NSP induced the differentiation of BMSCs to endothelial cells. ⁷ This system is consisted of the relevant degradative enzymes monoacylglycerol lipase and fatty acid amide hydrolase (FAAH), 2‐arachidonoylglycerol (2‐AG), anandamide (AEA), their endogenous ligands, and the G‐protein coupled cannabinoid (CB) receptors CB1 and CB2. ⁸ A recent report has shown that endocannabinoids have an effect opposite to that of NS on cholangiocarcinoma growth. ⁹ The increased Notch 1 signalling enhances the expression of Hes genes, which may be a mechanism underlying the role of cannabinoids in regulating and maintaining the neural progenitor cell pool. ¹⁰

Persistent bone loss primarily contributes to substantial decrease in bone formation and osteoblast number in majority of osteoporosis patients. It was shown that CB2 triggers aggravated age‐related osteoporosis due to increased bone turnover. ¹¹ It has been shown that bone loss in ageing mice with CB2 deficiency is related to increased bone resorption coupled to a substantial decrease in one formation and number of osteoblasts. ¹² Consistent with this, in ovariectomized mice, stimulation of peripheral CB2 receptors prevents bone loss by augmenting bone formation indicators. ¹¹ These results—together with proof demonstrating solid correlation of CB2 polymorphisms with osteoporotic women—indicated that CB2 agonists are promising activators of bone formation in osteoporosis. ¹³

It has been reported that CB2 is a regulator of Notch signalling pathway. ⁹ The Notch signal has been known to be a regulator of proliferation and differentiation of hBMSCs, and dysregulation of proliferation and differentiation of hBMSCs is believed to play an important role in the development of osteoporosis. ¹⁴ , ¹⁵ At the same time, Notch signalling has been shown to regulate the expression of CB2, so we hypothesized that CB2 and Notch could form a negative feedback loop to maintain the homoeostasis of various components in the system and regulate the proliferation and differentiation of hBMSCs. ¹⁶ In this study, we verified the hypothesis in an animal model of osteoporosis.

2. MATERIALS AND METHODS

2.1. Establishment of animal model

All animal tests were carried out according to the Principles of Laboratory Animal Care. All animals were 10 weeks old with a body mass of 20 ~ 30 g. For the first in vivo experiment, 24 mice were subdivided into four groups, and a control group of mice (N = 5) received surgery without an ovariectomy. Distilled water supplemented with gum acacia was utilized to treat the mice once a day on the 8th day after the surgery. A total of 19 mice received bilateral oophorectomy, and 4 mice died during the surgery. Seven days post‐ovariectomy (OVX) treatment, 15 mice were divided randomly and evenly into 3 groups of OVX, OVX + DHEA, and OVX + E2 with 5 mice in each group. In the OVX group, saline was utilized to administer the mice intragastrically. In the OVX + DHEA group, DHEA was utilized to administer the mice intragastrically at a final concentration of 5 mg/kg per day. In the OVX + E2 group, oestrogen (17‐β‐estradiol) was utilized to administer the mice intragastrically once a day. After 12 weeks of treatment, the mice were weighed. Then, all mice were sacrificed to collect tissue and blood samples for further analysis. Another in vivo experiment was carried out to examine whether DHEA served as a metabolite or an oestrogen derivative. A total of 40 mice received bilateral oophorectomy, whereas saline was utilized to treat 20 mice and DHEA was utilized to treat the other 20 mice. Saline‐treated OVX mice or DHEA‐treated OVX mice were divided into 4 groups and received the following treatment: The carrier solvent was utilized to treat one group, and 0.04, 0.2 or 2 μg/d of an aromatase inhibitor letrozole was utilized to treat the other 3 groups for 3 months.

2.2. Analysis of bone mineral density

For analysis of BMD (bone mineral density) performed following previous protocol, ¹⁷ the left lumbar and femur vertebrae were collected post‐dissection. An animal PIXImus densitometer (Lunar; GE Copr.) was utilized to carry out dual energy X‐ray absorptiometry (DEXA). Uniformity was maintained via selecting a consistent region of interest.

2.3. Bone microarchitecture assessment by micro‐CT

Explore Locus SP Pre‐Clinical Specimen Micro‐CT (GE Healthcare Bio‐Sciences) was utilized to scan bone microarchitecture in the distal femur with a 8 mm resolution, an 80 µA tube current and an 80 kV tube voltage. A Micro‐CT system (GE Healthcare Bio‐Sciences, MicroView 1.1 software) was utilized to carry out reconstruction and 3D quantitative analyses. In femora, the regions of scanning were limited to distal metaphysis and were extended about 2.0 mm from proximal tip of the primary spongiosa. For micro‐CT section, each trabecular bone region was outlined. For above regions, the endocortical bone surfaces were the boundaries to separate trabecular bone from cortical bone. The 3D indices listed below were analysed: bone mineral density (BMD), trabecular separation (Tb.Sp), proportion of bone volume in total volume (BV/TV), structure model index (SMI), trabecular thickness (Tb.Th) and the trabecular number (Tb.N).

2.4. RNA isolation and real‐time PCR

A miRNeasy Midi kit (Qiagen) was utilized to isolated total RNA from cultured cells and tissue samples. A High‐Capacity cDNA Archive kit (Applied Biosystems) was utilized to perform MultiScribe reverse transcription to synthesize cDNA from 1μg of total RNA. A LightCycler480 PCR system (Roche Diagnostics) was utilized along with a DNA binding SYBR Green dye (Applied Biosystems) to perform real‐time quantitative PCR to detect the relative expression of CB2, Notch1, Notch2, ALP and collagen type I mRNA. The PCR reactions were carried out at 95°C for 15 minutes for initial denaturation, followed by 50 cycles of 95°Cfor 15 seconds for denaturation, 55°C for 15 seconds for annealing and 72°C for 15 seconds for extension. The β‐actin and small RNA U6 were used as internal controls. 1.5% agarose gels were utilized to perform electrophoresis to visualize PCR products, and the comparative 2 −ΔΔCt method was utilized to calculate the relative expression of CB2 (Forward: 5'‐AGTGTTGGCTGTGCTCCTCATC‐3'; Reverse: 5'‐GTTGATGAGGCACAGCATGGAG‐3'), Notch1 (Forward: 5'‐ GGTGAACTGCTCTGAGGAGATC‐3'; Reverse: 5'‐ GGATTGCAGTCGTCCACGTTGA‐3'), Notch2 (Forward: 5'‐ GTGCCTATGTCCATCTGGATGG‐3'; Reverse: 5'‐ AGACACCTGAGTGCTGGCACAA‐3'), ALP (Forward: 5'‐ GCTGTAAGGACATCGCCTACCA‐3'; Reverse: 5'‐ GCTGTAAGGACATCGCCTACCA‐3'), and collagen type I mRNA (Forward: 5'‐ GATTCCCTGGACCTAAAGGTGC‐3'; Reverse: 5'‐ AGCCTCTCCATCTTTGCCAGCA‐3'), which were normalized to the expression of β‐actin and small RNA U6. Each reaction was repeated three times.

2.5. Cell culture and transfection

The RPMI culture medium (Gibco, Invitrogen) supplemented with 10% FBS (foetal bovine serum), 1% streptomycin‐penicillin (Invitrogen) and 2 mmol/L glutamine (Euroclone) was used to incubate the hBMSCs under a humidified atmosphere of 5% CO2/95% air at 37°C. On the day of transfection, when the cells reached 80% confluence, Lipofectamine 2000 (Invitrogen) was used to cotransfect the cells with pcDNA3‐NICD, CB2 shRNA and Notch1 shRNA. Each reaction was carried out in triplicate.

2.6. Vector construction

The coding sequence of NICD (Notch 1 intracellular coding domain) was amplified through PCR, and the PCR products were subsequently purified, double digested and cloned into a pcDNA3 vector. Direct Sanger sequencing was performed to confirm the sequence of the clone. All experiments were repeated three times.

2.7. Cell proliferation assay

PcDNA3‐NICD, CB2 shRNA or Notch1 shRNA was applied to hBMSCs. The 3‐(4, 5‐dimethylthiazol‐2‐yl)‐2, 5‐diphenyltetrazolium bromide (MTT) assay was utilized to analyse the proliferation of hBMSCs after 48 hours of transfection. Briefly, hBMSCs were seeded into 96‐well plates at a concentration of 3 × 10³ cells/well. Then, 50 μL of MTT was used to incubate the cells for 4 hours. HCL‐isopropanol was used to dissolve the formazan product, and a SpectraMax® microplate spectrophotometer (Molecular Devices, LLC) was utilized to examined the proliferation of hBMSCs based on the absorbance at 540 nm. Three independent experiments were carried out.

2.8. Western blot analysis

PcDNA3‐NICD, CB2 shRNA or Notch1 shRNA was applied to hBMSCs. At 48 hours post‐transfection, hBMSCs were harvested and lysed in an ice‐cold lysis buffer supplemented with 1% Triton X‐100, 130 mmol/L NaCl, 20 mmol/L Tris‐HCl [pH 8], 1 mmol/L sodium orthovanadate, 10% glycerol, 1 mmol/L PMSF, 2 mmol/L EDTA and protease inhibitors. Then, the lysates were subjected to centrifugation at 15 000× g for 10 minutes at 4°C, and 8%‐12% SDS‐PAGE was utilized to separate above lysates to obtain target proteins of CB2, Notch1, Notch2, ALP and collagen type I. Then, the proteins were electrophoretically transferred to polyvinylidene difluoride membranes (Millipore, Billerica, MA) for 2 hours at 90V, and TBS (150 mmol/L NaCl, 20 mmol/L Tris [pH 7.5]) containing 1% BSA was utilized to block the membranes at 25°C for 10 minutes to avoid non‐specific binding. The primary antibodies against CB2, Notch1, Notch2, ALP, collagen type I (1:8000) and anti‐β‐actin (1:10 000) were utilized to incubate the membranes at 4℃ overnight; then, the horseradish peroxidase (HRP)‐conjugated secondary antibody (1:13 000 dilution, Boster) was used to incubate the membranes for 60 minutes. The Chemi‐Doc™ XRS System (BIO‐RAD) and an immobilon Western chemiluminescent HRP Substrate (Millipore) were used to visualize the immune complexes and analyse the relative protein expression of CB2, Notch1, Notch2, ALP and collagen type I. All tests were repeated three times.

2.9. Immunohistochemistry

Four percentage paraformaldehyde was utilized to fix the tissue, which was then dehydrated, paraffin embedded and cut into 4μm sections. The monoclonal anti‐CB2, anti‐Notch1, anti‐Notch2, anti‐ALP, anti‐collagen type I (1:800) and anti‐β‐actin (1:1000) antibodies were utilized to incubate the sections, and then the horseradish peroxidase (HRP)‐conjugated secondary antibody (1:1500 dilution, Boster) was used to incubate the sections. A DAB (3, 3‐diaminobenzidine) substrate kit was utilized to carry out staining in accordance with manufacturer's instructions. Each experiment was performed in triplicate.

2.10. Statistical analysis

SPSS17.0 software package (SPSS, Inc) was utilized to conduct all statistical analyses. All data were presented as the mean ± SD (standard deviation). ANOVA (one‑way analysis of variance) was performed to compare between two groups. Three‑way ANOVA was performed to compare the differences among three groups. The P value of less than .05 was considered significant.

3. RESULTS

3.1. 2‐AG administration up‐regulated BMD in OVX mice

As shown in Figure 1, evident decreases in the BMD in femur (Figure 1A) and vertebra (Figure 1B) were observed in OVX mice compared with sham‐operated mice, while treatment of 2‐AG could partly restore the inhibited BMD in femur (Figure 1A) and vertebra (Figure 1B) in OVX mice, indicating that 2‐AG could up‐regulate BMD in OVX mice.

Figure 1.

2‐AG treatment improved BMD in OVX mice, and increased BMD in femur (A) and vertebra (B) in OVX mice (*P value < .05 vs sham group; #P value <.05 vs OVX group; OVX: ovariectomy)

3.2. Effect of 2‐AG on structural properties of bone

Alterations of femur bone architecture have been generally considered to be important in evaluating osteoporosis and to be associated with bone strength. To explore the effect of 2‐AG on femur bone architecture, bone microarchitecture in the distal femur was scanned using micro‐CT. As shown in Figure 2, BV/TV (Figure 2A), Tb.Th (Figure 2B), Tb.N (Figure 2D) and BMD (Figure 2E) were evidently decreased while Tb.Sp (Figure 2C) and SMI (Figure 2F) were significantly increased in the OVX group. Meanwhile, higher levels of BV/TV (Figure 2A), Tb.Th (Figure 2B), Tb.N (Figure 2D) and BMD (Figure 2E) were noted in the OVX + 2‐AG group, and lower levels of Tb.Sp (Figure 2C) and SMI (Figure 2F) were noted in the OVX + 2‐AG group.

Figure 2.

Femur bone architecture was assessed by micro‐CT (*P value <.05 vs sham group; #P value <.05 vs OVX group; BV/TV, proportion of bone volume in total volume; BMD, bone mineral density; SMI, structure model index; Tb.Th, trabecular thickness; Tb.Sp, trabecular separation; Tb.N, trabecular number). (A) 2‐AG increased BV/TV in OVX mice. (B) 2‐AG increased Tb.Th in OVX mice. (C) 2‐AG decreased Tb.Sp in OVX mice. (D) 2‐AG up‐regulated Tb.N in OVX mice. (E) 2‐AG treatment elevated BMD in OVX mice. (F) 2‐AG down‐regulated SMI in OVX mice

3.3. Effect of 2‐AG on the Notch1 signalling pathway

Furthermore, real‐time PCR and Western blot analysis were carried out to detect the levels of CB2, Notch1 and Notch 2 among the sham, OVX and OVX + 2‐AG groups. As shown in Figure 3, CB2 (Figure 3A) levels in both OVX and OVX + 2‐AG groups were much lower than that in the sham group, while the CB2 level in the OVX group showed no obvious difference from that in the OVX + 2‐AG group. Notch 1 (Figure 3B) mRNA and protein levels in OVX and OVX + 2‐AG groups were much lower than those in the sham group, while Notch 1 level in the OVX + 2‐AG group was partly restored. Notch 2 (Figure 3C) mRNA and protein levels were comparable among sham, OVX and OVX + 2‐AG groups.

Figure 3.

Real‐time PCR and Western blot analysis were carried out to detect the levels of CB2, Notch1 and Notch 2 among sham, OVX and OVX + 2‐AG groups (*P value <.05 vs sham group; #P value <.05 vs OVX group). (A) CB2 levels in OVX and OVX + 2‐AG groups were much lower than that in the sham group. (B) Notch 1 levels in OVX and OVX + 2‐AG groups were much lower than that in the sham group, and Notch 1 level in the OVX group was lower than that in the OVX + 2‐AG group. (C) Notch 2 level was comparable among sham, OVX and OVX + 2‐AG groups

3.4. Effect of 2‐AG on the proliferation and differentiation of hBMSCs

MTT assay was performed and differentiation biomarkers such as ALP and collagen type I were measured to identify the effect of 2‐AG on the proliferation and differentiation of BMSCs. As shown in Figure 4A, the viability of hBMSCs in OVX and OVX + 2‐AG groups were substantially reduced. Furthermore, the viability of hBMSCs in OVX exhibited no significant difference with that in the OVX + 2‐AG group. As biomarkers of differentiation of hBMSCs, collagen type I (Figure 4B) and ALP (Figure 4C) in OVX and OVX + 2‐AG groups were much lower than those in the sham group, while the 2‐AG treatment partly restored the suppressed levels of collagen type I (Figure 4B) and ALP (Figure 4C) in the OVX group.

Figure 4.

Effect of 2‐AG on the proliferation and differentiation of hBMSCs was determined using MTT assay. (A) Proliferation in sham and OVX + 2‐AG groups was much higher than that in the OVX group. (B) Collagen type I level in OVX and OVX + 2‐AG groups was much lower than that in the sham group, and collagen type I level in the OVX group was even lower. (C) ALP level in OVX and OVX + 2‐AG groups was much lower than that in the sham group, and ALP level in OVX group was even lower

3.5. Effect of Notch1 shRNA on the expression of CB2, Notch1 and Notch2 in 2‐AG‐treated hBMSCs

2‐AG‐treated hBMSCs were transfected with Notch1 shRNA before the levels of CB2, Notch 1 and Notch 2 were detected. As shown in Figure 5, Notch1 shRNA and 2‐AG had no effect on CB2 (Figure 5A) and Notch 2 (Figure 5C) levels. However, 2‐AG substantially increased Notch 1 expression (Figure 5B), while the transfection of Notch shRNA into 2‐AG‐treated hBMSCs obviously decreased Notch 1 expression.

Figure 5.

(A) Notch1 shRNA and 2‐AG had no effect on CB2 expression. (B) Notch 1 level in 2‐AG and 2‐AG + Notch1 shRNA groups was much higher than that in the NC group, and Notch 1 level in 2‐AG group was even higher than that in the 2‐AG + Notch1 shRNA group (*P value <.05 vs negative control group; #P value <.05 vs. 2‐AG group). (C) Notch1 shRNA and 2‐AG had no effect on Notch 2 expression

3.6. Effects of 2‐AG and Notch 1 on the proliferation and differentiation of hBMSCs

As shown in Figures 6A, 2‐AG and 2‐AG + Notch 1 shRNA significantly promoted the proliferation of hBMSCs, while the effect of 2‐AG was stronger than 2‐AG + Notch 1 shRNA. Collagen type I (Figure 6B) and ALP (Figure 6C) levels in 2‐AG and 2‐AG + Notch 1 shRNA groups were much higher than those in the NC group, and collagen type I (Figure 6B) and ALP (Figure 6C) levels in 2‐AG group were even higher than those in the 2‐AG + Notch 1 shRNA group.

Figure 6.

(A) Viability of hBMSCs in 2‐AG and 2‐AG + Notch 1 shRNA groups was enhanced, and the effect of 2‐AG on cell viability was stronger than 2‐AG + Notch 1 shRNA. (B) Collagen type I differentiation biomarkers such as ALP and collagen type I were measured to identify the effect of 2‐AG on the proliferation and differentiation of BMSCs. Collagen type I level in 2‐AG and 2‐AG + Notch 1 shRNA groups was much higher than that in the NC group (*P value <.05 vs negative control group; #P value <.05 vs 2‐AG group). (C) ALP level in 2‐AG and 2‐AG + Notch 1 shRNA groups was much higher than that in the NC group (*P value <.05 vs negative control group; #P value <.05 vs 2‐AG group)

3.7. Effect of CB2 shRNA and NICD on the expression of CB2 and Notch signals.

Real‐time PCR and Western blot analysis were performed to examine the levels of CB2, Notch 1 and Notch 1 in cells transfected with CB2 shRNA and CB2 shRNA + NICD. As shown in Figure 7A, both CB2 shRNA transfection and cotransfection of CB2 shRNA + NICD significantly decreased CB2 levels, and the inhibitory effect of CB2 shRNA was comparable with that of CB2 shRNA + NICD. The Notch 1 (Figure 7B) level in the CB2 shRNA group was much lower than that in the NC group, while the transfection of CB2 shRNA along with NICD almost fully restored Notch 1 level compared with the CB2 shRNA group. Finally, CB2 and NICD had no effect on Notch 2 expression.

Figure 7.

(A) CB2 levels in CB2 shRNA and CB2 shRNA + NICD groups were much lower than that in the NC group (*P value <.05 vs negative control group). (B) Notch I level in CB2 shRNA + NICD and NC groups was much higher than that in the CB2 shRNA group (*P value <.05 vs negative control group; #P value <.05 vs CB2 shRNA group). (C) CB2 shRNA and CB2 shRNA + NICD had no effect on Notch 2 expression

3.8. Effects of CB2 shRNA and NICD on the proliferation and differentiation of hBMSCs

As shown in Figure 8A, CB2 shRNA significantly suppressed the proliferation of hBMSCs, and transfection of CB2 shRNA along with NICD fully restored hBMSCs viability. CB2 shRNA significantly inhibited collagen type I (Figure 8B) and ALP (Figure 8C) expression, while the presence of NICD fully restored collagen type I and ALP expression in CB2 shRNA‐transfected cells.

Figure 8.

(A) Survival of hBMSCs in CB2 shRNA + NICD and NC groups was much higher than that in the CB2 shRNA group. (B) Collagen type I level in CB2 shRNA + NICD and NC groups was much higher than that in the CB2 shRNA group (*P value <.05 vs negative control group; #P value <.05 vs CB2 shRNA group). (C) ALP level in CB2 shRNA + NICD and NC groups was much higher than that in the CB2 shRNA group (*P value <.05 vs negative control group; #P value <.05 vs CB2 shRNA group)

4. DISCUSSION

Two identified cannabinoid receptors in the G‐protein coupled receptor family, CB1 and CB2, are bound and activated by endocannabinoids and their synthetic analogues. ¹⁸ CB1 and CB2 receptors are coupled to cyclic adenosine monophosphate (cAMP) and adenylyl cyclase together with a lot of other second messengers such as PI3 Kinase/Akt and phospholipase C. ¹⁹ CB1 is primarily expressed in the brain, while CB2 is mainly expressed in the immune cells. ²⁰ Recent studies, however, have shown that CB1 and CB2 receptors are also found in other organs, tissues and cells such as adipocytes and bone cells. ¹¹ It has been shown that 2‐AG stimulates Notch 2 while AEA stimulates Notch 1. Recently, in dendritic cells with Δ⁹‐tetrahydrocannabinol elevating the production of Jagged 1 and reducing the expression of Notch ligand Delta 4, a similar stimulation of the NSP by cannabinoids has been observed. ²¹ This first suggested that cannabinoid plays a role in NS. ⁹ In this study, we established an animal model of osteoporosis, which was further treated with 2‐AG. Next, we performed MTT assay and examined the differentiation of biomarkers such as ALP and collagen type I to identify the effect of 2‐AG on the proliferation and differentiation of BMSCs. Accordingly, we found that 2‐AG promoted the differentiation of hBMSCs in OVX mice.

It was shown that osteoporotic BMSCs have elevated adipogenesis, featured by an impaired leptin action. ²² Zhang et al ²³ found the promotion of adipogenic potential and the decrease of osteogenic potential in osteoporotic BMSCs. Osteoporotic BMSCs are different from normal controls in that they have a reduced growth rate and are insensitive to the mitogenic effect of IGF‐1, which is implicated in the MAPK signalling pathway. ²⁴ In osteoporotic postmenopausal women, the ability of BMSCs to produce and maintain type I collagen‐rich extracellular matrix is reduced, promoting the cell differentiation of adipogenesis. ²⁵

Canonical NS is a well‐known modulator of stem cell self‐renewal, proliferation and differentiation. ⁹ Other reports have recently found that, during mouse limb‐bud and postnatal bone development, the RBPjκ‐dependent NSP could function as a suppressor of MPC/BMSC differentiation and a significant trigger of BMSC and mesenchymal progenitor cell (MPC) proliferation. ²⁶ These mouse studies showed that conditional ablation of the components of NSP (HES/HEY factors, RBPjκ, NOTCH1 or NOTCH2) in early BMSCs and MPCs of the limbs led to increased osteogenic and differentiation of chondrogenesis, followed by a depleted BMSC pool. ²⁶ Recent data also showed that one or more of the HES/HEY NOTCH‐associated factors may trigger this BMSC/MPC suppression of differentiation. ²⁶ Other studies have demonstrated that persistent stimulation of the NP in cultured human BMSCs through viral infection with NICD1 or JAG1 inhibited differentiation of chondrogenesis. ²⁷ Moreover, cultured human BMSCs treated with a DAPT (N‐[2S‐(3, 5‐difluorophenyl)acetyl]‐l‐alanyl‐2‐phenyl‐1,1‐dimethylethyl ester‐glycine) suppressor had lower in vitro proliferative capacity. ²⁸ A previous study has shown that γ‐secretase activity can be regulated by the recruitment and dependence of the γ‐secretase complex to structures of lipid raft; hence, it is plausible that agents that disrupt or stabilize lipid raft structures may also modulate the NSP. ²⁹ , ³⁰ In this study, we investigated the relationship among 2‐AG, CB2 and Notch 1, and found that 2‐AG up‐regulated Notch 1 expression, but had no effect on CB2 expression. Furthermore, we investigated the effects of 2‐AG and Notch 1 on the proliferation and differentiation of hBMSCs, and found that 2‐AG and Notch 1 shRNA promoted and inhibited cell proliferation and differentiation, respectively.

An earlier study demonstrated that mice with CNR2 knockout had a reduced bone mass, reminiscent of human osteoporosis. ³¹ , ³² Some reports have shown the relationship between BMD and CNR2 polymorphisms. ¹⁴ Recently, it has been shown that CNR2 gene was related to BMD in postmenopausal women in Korea. ³³ Further evidence supported the relationship between CNR2 gene and BMD. Two SNPs of rs2501431 and rs4237 in CNR2 gene may be indicative of the risk of osteoporosis in Chinese postmenopausal women. ³⁴ In this study, we revealed that CB2 shRNA decreased Notch I level, while NICD increased Notch I level. However, NICD had no effect on CB2 expression. In addition, we also found that CB2 shRNA inhibited cell proliferation and differentiation, while NICD promoted proliferation and differentiation of hBMSCs.

5. CONCLUSION

In conclusion, our results provided further evidence for the association of CB2 gene with BMD and osteoporosis. Our study revealed that CB2 inhibited Notch 1 expression, and Notch 1 served as a regulator of proliferation and differentiation of hBMSCs. Dysregulation of proliferation and differentiation of hBMSCs is believed to play an important role in the development of osteoporosis. Therefore, our study provided a deeper insight into the pathophysiology of osteoporosis and identified CB2 as a promising target for the treatment of osteoporosis.

CONFLICT OF INTERESTS

None.

AUTHOR CONTRIBUTIONS

Feng Tian: Conceptualization (equal); Investigation (equal); Project administration (equal); Validation (equal); Writing‐original draft (equal). Hong‐tao Yang: Formal analysis (equal); Investigation (equal); Methodology (equal); Software (equal); Writing‐original draft (equal). Tao Huang: Investigation (equal); Validation (equal); Visualization (equal). Feng‐feng Chen: Investigation (equal); Methodology (equal); Software (equal); Validation (equal). Fu‐jun Xiong: Conceptualization (equal); Methodology (equal); Project administration (equal); Resources (equal); Supervision (equal); Writing‐original draft (equal).

Tian F, Yang H‐T, Huang T, Chen F‐F, Xiong F‐J. Involvement of CB2 signalling pathway in the development of osteoporosis by regulating the proliferation and differentiation of hBMSCs. J Cell Mol Med. 2021;25:2426–2435. 10.1111/jcmm.16128

DATA AVAILABILITY STATEMENT

The data that support the findings of this study are available from the corresponding author upon reasonable request.