Stem Cells International

Stem Cells International / 2020 / Article

Research Article | Open Access

Volume 2020 |Article ID 8811963 | https://doi.org/10.1155/2020/8811963

Jun Ying, Qinwen Ge, Songfeng Hu, Cheng Luo, Fengyi Lu, Yikang Yu, Taotao Xu, Shuaijie Lv, Lei Zhang, Jie Shen, Di Chen, Peijian Tong, Luwei Xiao, Ju Li, Hongting Jin, Pinger Wang, "Amygdalin Promotes Fracture Healing through TGF-β/Smad Signaling in Mesenchymal Stem Cells", Stem Cells International, vol. 2020, Article ID 8811963, 13 pages, 2020. https://doi.org/10.1155/2020/8811963

Amygdalin Promotes Fracture Healing through TGF-β/Smad Signaling in Mesenchymal Stem Cells

Academic Editor: Darius Widera
Received15 Jun 2020
Revised13 Aug 2020
Accepted21 Aug 2020
Published07 Sep 2020

Abstract

Chondrogenesis and subsequent osteogenesis of mesenchymal stem cells (MSCs) and angiogenesis at injured sites are crucial for bone fracture healing. Amygdalin, a cyanogenic glycoside compound derived from bitter apricot kernel, has been reported to inhibit IL-1β-induced chondrocyte degeneration and to stimulate blood circulation, suggesting a promising role of amygdalin in fracture healing. In this study, tibial fractures in C57BL/6 mice were treated with amygdalin. Fracture calluses were then harvested and subjected to radiographic, histological, and biomechanical testing, as well as angiography and gene expression analyses to evaluate fracture healing. The results showed that amygdalin treatment promoted bone fracture healing. Further experiments using MSC-specific transforming growth factor- (TGF-) β receptor 2 conditional knockout (KO) mice (Tgfbr2Gli1-Cre) and C3H10 T1/2 murine mesenchymal progenitor cells showed that this effect was mediated through TGF-β/Smad signaling. We conclude that amygdalin could be used as an alternative treatment for bone fractures.

1. Introduction

Bone fractures, mainly caused by traumatic incidents and medical conditions, including osteoporosis, are a growing global health burden currently affecting millions of people [1, 2]. Even with treatment, fractures are associated with great economic burden, loss of independence, and high rates of morbidity and mortality [3]. In clinical practice, fractures can be stabilized using various fixation methods, such as braces and internal, external, and intramedullary fixation [46]. However, fracture nonunion is observed in 5-10% of patients annually [7]. In addition, bedfast patients receiving conservative treatment have higher risks of pressure ulcers, hypostatic pneumonia, lower extremity venous thromboembolism, and death.

Bone fracture healing is a complicated biological process that involves specific regenerative patterns and diverse gene expression changes [8, 9]. Secondary healing is the most common form of bone healing, which normally includes endochondral and intramembranous bone healing that can be separated into three consecutive stages: inflammation, bone repair, and remodeling [9]. The inflammatory phase is characterized by the formation of a hematoma and the immediate release of soluble inflammatory mediators that induce immune cell infiltration [10].

Mesenchymal stem cells (MSCs) can migrate to the fracture site and differentiate into chondrocytes, which form a cartilaginous soft callus. This primary callus is subsequently surrounded by new bone material produced by osteoblasts in the perichondrium and permeated with blood vessels. The cartilaginous callus then undergoes remodeling to replace the cartilage with new bone. Thus, the promotion of chondrogenesis/osteogenesis and angiogenesis can accelerate fracture healing. The origin of MSCs is not fully understood, but the recruitment, proliferation, and differentiation of these cells are indispensable for fracture healing [11]. Successful bone repair and remodeling are also dependent on an adequate blood supply and revascularization of the injured area [12].

Amygdalin (D-mandelonitrile-β-gentiobioside) is derived from bitter apricot kernel and has been used clinically for the treatment of asthma, aplastic anemia, tumors, and alloxan-induced diabetes [1315]. Amygdalin has also been reported to inhibit IL-1β-induced chondrocyte degeneration in endplates and to both improve microcirculation and relieve blood stasis [16, 17]. Amygdalin has been implicated in the regulation of transforming growth factor- (TGF-) β/Smad signaling [18], which has a fundamental regulatory function for bone homeostasis [19, 20]. Therefore, we hypothesized that amygdalin can promote bone fracture healing through TGF-β/Smad signaling.

2. Materials and Methods

2.1. Preparation and Administration of Amygdalin

Amygdalin (CAS NO. 29883-15-6, , Sigma, St. Louis, MO, USA) (Figure 1(a)) used in this study was purchased from the National Institutes for Food and Drug Control of China and dissolved in sterile normal saline (NS) (0.05 mg/mL). In the amygdalin-treated group, mice were intraperitoneally injected with 0.5 mg/kg of amygdalin daily from day 1 postoperation. Mice in the control group were intraperitoneally injected with an equal amount of phosphate-buffered saline (PBS).

2.2. Experimental Animals

This study was approved by the Animal Experimentation Ethics Committee of Zhejiang Chinese Medical University. The animal center of the Zhejiang Chinese Medical University provided C57BL/6 mice (SCXK, Shanghai, 2012-0002). Gli1-CreER transgenic mice can efficiently target MSCs by injecting tamoxifen (TM) to induce the formation of Cre (CreERT2) from the endogenous Gli1 locus [21]. The Gli1-CreER transgenic mice were crossed with Tgfβr2flox/flox mice [22] to specifically knock out the TGF-β receptor 2 (Tgfbr2) in MSCs. Tamoxifen was administered (5 mg, dissolved in corn oil) once daily for 5 consecutive days by intraperitoneal injection.

A DNA extraction kit (Sigma, USA) was used to determine mouse genotyping. The sequences of primers used for genotyping were as follows: Cre, Fw: 5-ATT GCT GTC ACT TGG TCG TGGC-3; Rv: 5-GAA AAT GCT TCT GTC CGT TTGC-3; Tgfbr2 loxP, Fw: 5-TAA ACA AGG TCC GGA GCC CA-3; Rv: 5-ACT TCT GCA AGA GGT CCC CT-3 (wild-type, 420-base-pair PCR product; homozygotic type, 540-base-pair PCR product). Cre-negative littermates were used as controls.

2.3. Cell Culture

C3H10 T1/2 murine mesenchymal progenitor cells (ATCC, Manassas, VA, USA) were cultured in Dulbecco’s modified Eagle medium (DMEM) (Hyclone, Logan, Utah, USA) supplemented with 10% fetal bovine serum (FBS), 100 U/mL penicillin and 100 mg/mL streptomycin (Gibco, Grand Island, NY, USA) in a 5% CO2 humidified incubator at 37°C. After reaching 80% confluence, cells were collected and divided into the control group, the TGF-β1 group (treated with 10 ng/mL recombinant TGF-β1), the amygdalin group (treated with 10 μM amygdalin), the TGF-β1 plus TGF-β/Smad pathway inhibitor-SB525334 group (treated with 10 ng/mL recombinant TGF-β1 and 10 μM SB525334), the amygdalin plus SB525334 group (treated with 10 μM amygdalin and 10 μM SB525334), and the SB525334 group (treated with 10 μM SB525334). After 4 hours of treatment, the cells were collected, and changes in the levels of phosphorylated-Smad2/3 were analyzed. In addition, relative chondrogenic (Col2a1, Sox9) gene expressions were analyzed following three days in culture.

2.4. Tibial Fracture Model

Right transverse tibial fractures were performed and fixed with an intramedullary needle [23]. Ten-week-old male C57BL/6, Tgfβr2f/f, and Tgfβr2Gli1Cre mice were anesthetized with ketamine (60 mg/kg) by intraperitoneal injection. After local disinfection, a 1.0 cm long cut in the anteromedial skin of the tibia was created. A 26-gauge syringe needle was then inserted into the bone marrow cavity through the tibial plateau at the medial of patellar ligament. The needle was then removed, and the tibia was transected using a No.11 surgical blade. The 26-gauge syringe needle was reinserted into tibia to simulate intramedullary fixation. A 5-0 silk suture was selected to close the incision, and buprenorphine administration (in drinking water) was used to reduce pain during the first three days following surgery. Immediately following surgery, X-ray tests (Carestream, FX Pro, USA) were performed on the right lower limb in the anterior-posterior and lateral directions to confirm the correctness of osteotomy and the alignment of the bone. The mice were then divided into groups for analysis: C57BL/6 mice treated with amygdalin or PBS, and Tgfβr2Gli1Cre and Cre-negative controls both treated with amygdalin.

2.5. X-Ray and μCT Analyses

At days 4, 7, 10, 14, and 21 postsurgery, mice were euthanized, and tibiae were collected for X-ray and microcomputed tomography (μCT) (Skyscan 1176; Bruker μCT, Kontich, Belgium) analyses to examine fracture healing quality. At each time point, harvested specimens were scanned using μCT at 8.73-micron isotropic resolution, with settings of 42 kV and 555 μA and 786 ms integration time. Followed by radiographic union scale (RUST) in the tibial fracture score system, semiquantitative analyses of the X-ray were performed. Callus bone volume (BV) and callus mineralized volume fraction (BV/TV) (%) parameters were then measured.

2.6. Biomechanical Testing

Full-length tibiae were harvested and removed from their surrounding soft tissues ( at days 4, 7, 10, 14, and 21). Both ends of each tibia were then fixed in bone cement to ensure that the fracture site was exposed. Specimens were installed on an Endura Tec TestBench TM system (200 N mm torque cell; Bose Corporation, Minnetonka, MN, USA) to apply torsion at a rate of 1°/s until failure to determine the modulus of elasticity and maximum loading of the fracture callus.

2.7. Histology and Histomorphometry

After three days of fixation with 10% normal buffered formalin, the bone samples were decalcified in 14% ethylenediaminetetraacetic acid (EDTA) for two weeks. The decalcified bones were dehydrated and embedded in paraffin and sectioned (3 μm). Alcian blue/H&E (ABH) staining and tartrate-resistant acid phosphatase (TRAP) staining were performed. Quantitative histomorphometry was performed on the ABH- and TRAP-stained sections using the ImageJ 1.46r software (Wayne Rasband, National Institute of Health, USA). The cartilage area per periosteal callus area (%, Cg.Ar/http://Ps.Cl.Ar) and the mineralized area per periosteal callus area (%, Md.Ar/http://Ps.Cl.Ar) were measured as described previously [24]. Immunohistochemistry (IHC) was performed on sections using high-pressure heating in pH 6.0 sodium citrate solution for 2 minutes to achieve antigen retrieval. The tissues were then incubated with a rabbit anti-mouse anti-p-Smad2 antibody (Abcam, ab188334, 1 : 200), anti-pSmad1/5/8 antibody (Millipore, AB3848, 1 : 200), and anti-CD31 antibody (Arigo, ARG52748, 1 : 100) overnight at 4°C. PBS was incubated on negative group slides. The following day, a biotinylated anti-rabbit secondary antibody and an enzyme conjugate (Histostain-Plus Kit, Invitrogen, USA) were separately incubated on sections. IHC signals were developed using DAB chromogen (Histostain-Plus Kit) and counterstained for nuclei using Tacha’s CAT Hematoxylin.

2.8. Quantitative Real-Time Polymerase Chain Reaction

The callus was cut with a range of 2 mm around the fracture line. Total RNA was extracted from the callus and three duplicated wells of C3H10 T1/2 cells in the third passage by using the RNeasy kit (Qiagen, Germany) following the manufacturer’s instructions. Then, complementary DNA (cDNA) was synthesized using a cDNA reverse transcription kit (Takara, Otsu, Japan). Quantitative real-time polymerase chain reaction (qRT-PCR) was performed using the SYBR Premix EX Taq™ kit (Takara) according to the manufacturer’s instructions. Primer sequences for Sox9, Col2a1, Col10a1, Osteocalcin, Runx2, vascular endothelial growth factor (Vegf), and β-actin are shown in Table 1.


Primer nameSequences

β-Actin forward5-GGAGATTACTGCCCTGGCTCCTA-3
β-Actin reverse5-GACTCATCGTACTCCTGCTTGCTG-3
Sox9 forward5-GAGGCCACGGAACAGACTCA-3
Sox9 reverse5-CAGCGCCTTGAAGATAGCATT-3
Col2a1 forward5-TGGTCCTCTGGGCATCTCAGGC-3
Col2a1 reverse5-GGTGAACCTGCTGTTGCCCTCA-3
Col10a1 forward5-ACCCCAAGGACCTAAAGGAA-3
Col10a1 reverse5-CCCCAGGATACCCTGTTTTT-3
Runx2 forward5-GAGGGCACAAGTTCTATCTGGA-3
Runx2 reverse5-GGTGGTCCGCGATGATCTC-3
Osteocalcin forward5-AGGGAGGATCAAGTCCCG-3
Osteocalcin reverse5-GAACAGACTCCGGCGCTA-3
VEGF forward5-GCACATAGAGAGAATGAGCTTCC-3
VEGF reverse5-CTCCGCTCTGAACAAGGCT-3

2.9. Western Blot Analysis

Three duplicated wells of C3H10T1/2 cells at passage 3 were prepared for protein extraction. Cell lysates were extracted using a modified radioimmunoprecipitation assay (RIPA) lysis buffer that contained 1 mM phenylmethylsulfonyl fluoride (PMSF) and a protease inhibitor cocktail (Cell Signaling Technology, USA). Following centrifugation at 12000g for 30 minutes, the supernatant was collected to detect the total protein concentrations using a BCA Protein Assay kit (Thermo Scientific, USA). Protein extracts were boiled for 5 minutes in loading buffer. Then, 40 μg protein was loaded and electrophoresed on a sodium dodecyl sulfate polyacrylamide gel electrophoresis (SDS-PAGE) gel and transferred to a polyvinylidene difluoride (PVDF) membrane. The membrane was blocked in a 5% skim milk solution and incubated with primary antibodies overnight at 4°C. The primary antibodies were β-actin (Sigma, A1978), Smad2/3 (Cell Signaling Technology, #8685), and phosphorylated-Smad2/3 (Cell Signaling Technology, #8828). The membrane was then incubated with a fluorescent secondary antibody (LI-COR, 926-32212) (1/1000), for 1 hour at room temperature (Vector Laboratories, Burlingame, VT, USA). The blots were visualized using a LI-COR Odyssey® scanner (LI-COR Biosciences, USA). The relative density of the p-Smad2/3 bands was normalized to their corresponding actin bands.

2.10. Wound Scratch Test and Transwell Cell Migration

C3H10 T1/2 cells were seeded in six-well plates and cultured with DMEM/F12 supplemented with 5% FBS, penicillin, and 100 g/L streptomycin. After reaching 80%-90% confluence, a scratch of ~0.5 mm was made using a sterile pipette tip and then washed with PBS to clear cellular debris. After injury, the cells were cultured with low glucose DMEM/F12 containing 5% () FBS with 0, 10 μM amygdalin, 10 ng/mL TGFβ1, 10 μM amygdalin plus 10 μM SB525334, 10 ng/mL TGFβ1 plus 10 μM SB525334, or 10 μM SB525334. The migrations of C3H10 T1/2 cells into the scratch were photographed using an inverted microscope (Olympus, Tokyo, Japan) at 24 hours post insult.

Transwell assays were performed using 8 μm-pore Transwell polycarbonate membranes (Corning Inc., Corning, New York, USA). cells were seeded with 200 μL DMEM/F12 containing 2% FBS in the upper chamber, and in the lower chamber, 500 μL DMEM/F12 containing 2% FBS with 0, 10 μM amygdalin, 10 ng/mL TGFβ1, 10 μM amygdalin plus 10 μM SB525334, 10 ng/mL TGFβ1 plus 10 μM SB525334, or 10 μM SB525334. After incubating for 48 h, the migratory cells were fixed with 4% paraformaldehyde for 15 min and stained with crystal violet. Three random images were taken in the fields.

2.11. In Vivo Angiography

After injecting a mouse with ketamine (60 mg/kg), the right atrium was perforated, and 10 mL PBS/heparin sodium was injected through the apex of the left ventricle. Subsequently, 10 mL of 4% paraformaldehyde was perfused using the same method. Finally, 10 mL MICROFIL was injected with more pressure due to its viscosity and conserved overnight at 4°C. Muscles around the bone callus were removed to eliminate the influence of muscle blood vessels. μCT scanning was first used to locate the callus surrounding the fracture. After decalcification of the harvested bone samples for 3 days, the samples were scanned again, using the same volume of interest (VOI). The analysis area included 400 slices by considering the fracture line as the midline. The CTAn Software (Skyscan, Version 1.16) was used to build three-dimensional (3D) models and to measure relative vessel volume.

2.12. Statistical Analysis

All data were obtained from 6 individual mice in every experiment and 3 duplicated wells of C3H10 T1/2 cells. Values are showed as the mean. Two-way ANOVA followed by the Tukey-Kramer posttest (multiple groups) and unpaired Student’s -test (two groups) were used for statistical analyses. The SPSS 17.0 software was used to perform the statistical tests. was considered significant.

3. Results

3.1. Amygdalin Facilitates Bone Fracture Healing in Mice

To assess the effects of amygdalin on fracture healing, mice were treated with PBS or amygdalin (0.5 mg/kg/day). X-ray results showed that treatment with amygdalin promoted earlier formation of bone callus (Figure 1(b)). In the amygdalin group, a clear callus profile could be observed at day 10, and the callus became more radiopaque at day 14 postfracture. In contrast, the callus was not apparent in the control group until day 14 postfracture.

In addition, 3D reconstructions of μCT images showed that obvious fracture gaps could be observed in the control group at days 4, 7, 10, and 14, and newly formed bone had not fully bridged the gaps until day 21 (Figure 1(c), left). In contrast, in the amygdalin-treated group, the fracture gap appeared indistinct at day 14, indicating a higher proportion of mineralized bone in the callus (Figure 1(c), right). μCT analysis revealed that the bone volume (%, BV/TV) in the amygdalin group was significantly increased compared to the control group at days 10 and 14 (Figure 1(d)), consistent with the radiographic results.

Furthermore, biomechanical testing showed that the modulus of elasticity and maximum loading increased significantly in tibia samples at days 10, 14, and 21 in the amygdalin-treated group compared to the PBS control group (). These data demonstrated that bone mechanical strength has been improved by amygdalin treatment (Figure 2).

Because radiographic evaluation cannot detect changes in cartilage and soft tissues, Alcian blue/Hematoxylin/Orange G (ABH/OG) staining and histomorphometric analysis of the fractured bone were performed. The cartilage area (%, Cg.Ar/http://Ps.Cl.Ar) was significantly reduced by day 14 postfracture, and the mineralized bone area was significantly increased (%, Md.Ar/http://Ps.Cl.Ar) at days 10-21 postfracture in amygdalin-treated mice compared to the control. At day 21, the cartilage was no longer detectable in either group (Figures 3(a)3(c)). In addition, phospho-Smad2 and phospho-Smad1/5/8 IHC was performed to observe activation of TGF-β/Smad and BMP2 signaling during fracture healing. As shown in Figure 3(d), amygdalin treatment could increase phospho-Smad2 expression at day 7 but have no obvious effect on phospho- Smad1/5/8 expression at day 10. TRAP staining was also performed in the fracture callus at day 14. No significant changes in osteoclast numbers were found after amygdalin treatment at day 14 (Figure 3(e)).

We also measured the expression of marker genes related to bone fracture healing. The gene expression of early chondrogenesis, such as Sox9 and Col2a1, was similar in amygdalin-treated and control mice during fracture healing, except that Sox9 expression was reduced at day 21 (Figures 4(a) and 4(b)). Levels of Col10a1, a marker of late hypertrophic cartilage, were upregulated at days 10 and 14 in the amygdalin treatment group (Figure 4(c)); this supported the histologic results of decreased cartilage area at day 14. Osteogenic marker genes, runt-related transcription factor 2 (Runx2), and osteocalcin (OCN), were also increased at days 10 and 14 in the amygdalin treatment group compared to the control group (Figures 4(d) and 4(e)). In addition, expression of Vegf at days 10 and 14 was increased in the amygdalin-treated group compared to the controls, indicating that amygdalin may stimulate angiogenesis during fracture healing (Figure 4(f)).

Angiographic results demonstrated that amygdalin stimulated angiogenesis and increased the vessel volume in the cartilaginous bone around the fracture callus () (Figure 5(a)). Protein expression of the endothelial cell marker, CD31, was assessed by IHC at the callus area on day 10. Fracture callus samples from amygdalin-treated mice showed increased CD31 expression (Figure 5(b)), consistent with upregulation of the angiogenesis-related marker gene Vegf.

3.2. Amygdalin Accelerates Bone Fracture Healing through TGF-β/Smad Signaling of MSCs In Vivo

TGF-β/Smad signaling plays fundamental roles in bone homeostasis [25], and amygdalin has been implicated in the regulation of this pathway. To determine whether TGF-β/Smad signaling in MSCs is directly required for amygdalin-induced fracture healing, tibia fractures were performed on MSC-specific Tgfβr2 conditional KO (Tgfβr2Gli1Cre) mice and Cre-negative mice.

To determine the Tgfβr2 knockout efficiency in Tgfβr2Gli1Cre mice, IHC of p-Smad2 on fracture callus sections of Cre-negative mice and Tgfbr2Gli1Cre mice at day 10 was performed. The protein expression of p-Smad2 was obviously reduced in Tgfbr2Gli1Cre mice, indicating inhibition of TGFβ/Smad pathway signaling (Figure 6(a)). Following fractures, amygdalin was administrated to all mice. X-ray results showed that fracture lines disappeared at days 14 and 21 in the Cre-negative group but were still clearly visible until day 21 in the Tgfβr2Gli1Cre group (Figure 6(b)). Furthermore, μCT results indicated that amygdalin treatment increased bone volume and BV/TV around the fracture lines in Cre-negative mice compared to the Tgfβr2Gli1Cre mice, especially at days 10 and 14 (Figures 6(c) and 6(d)).

In histological analyses of fracture callus tissues, the Tgfβr2Gli1Cre mice showed delayed fracture repair (Figure 7(a)). The cartilage area (%, Cg.Ar/http://Ps.Cl.Ar) in Tgfβr2Gli1Cre mice was significantly increased compared with controls at day 14 (Figure 7(b)). In addition, Tgfβr2Gli1Cre mice showed a weaker ability for formation of woven bone at days 10, 14, and 21 postfracture (Figure 7(c)), indicating its slower transformation from cartilage into woven bone. Even though the osteoclast number in Cre-negative mice was higher than that in Tgfβr2Gli1Cre mice, the difference was not significant (Figure 7(d)).

3.3. Amygdalin Promotes Migration and Differentiation of MSCs through TGF-β/Smad Signaling In Vitro

Yu Shi et al. [21] recently found that Gli1+ osteogenic mesenchymal progenitors mainly facilitate normal bone formation and fracture healing. To determine if amygdalin promotes MSC migration and differentiation through TGF-β/Smad signaling, we conducted in vitro wound scratch tests and Transwell cell migration assays using C3H10 T1/2 cells. Both TGF-β1 (10 ng/mL) and amygdalin (10 μM) treatment significantly enhanced the migration of C3H10 T1/2 cells, which could be effectively inhibited after TGFβ/Smad signaling was blocked by treating with SB525334 (Figure 8).

Furthermore, TGF-β1 and amygdalin promoted chondrogenesis in C3H10 T1/2 cells, as shown by the upregulation of chondrogenic genes, including Sox9, Col2a1, and Tgfbr2 (Figure 9(a)). However, the effect was obviously inhibited by treatment with SB525334. In addition, phosphorylated SMAD2/3, which can regulate chondrogenesis of MSCs, was analyzed to explore the mechanism of amygdalin-induced early chondrogenic differentiation of MSCs. The p-SMAD2/3 protein expression was significantly increased in amygdalin-treated C3H10T1/2 cells, but this upregulation was inhibited in C3H10T1/2 cells treated with amygdalin plus SB525334 (Figure 9(b)). These results indicate that amygdalin can promote MSC migration and differentiation through TGF-β/Smad signaling.

4. Discussion

Bone fracture is common clinically and can cause significant patient morbidity. Several products, such as Dalbergia sissoo, Peperomia pellucida, and leaves of the Ginkgo biloba tree, have been investigated for potential effects on fracture repair [2628]. The effect and molecular mechanisms of amygdalin on fracture healing, however, has not been determined. Our study demonstrated that treatment with amygdalin promotes fracture healing mainly through TGF-β/Smad signaling in MSCs.

Initially, two doses (0.5 and 1.0 mg/kg/day) of amygdalin were used to treat fractures in C57BL/6 mice. However, in consideration of the better effects of treatment with amygdalin at 0.5 mg/kg/day in preexperiments, we selected this lower dose for subsequent experiments. The results showed that amygdalin treatment significantly promoted endochondral ossification in the fracture callus. Radiographic data demonstrated that the radiographic union score increased after 10 days in the amygdalin group compared to the control group. μCT analysis determined that amygdalin treatment significantly promoted deposition of osteoid callus, which filled the fracture gap with a higher proportion of mineralized bone, accompanied by increased bone volume. This conclusion is consistent with the results of histologic and histomorphometric analyses.

Fracture healing is a dynamic process. In mice, indirect fracture healing (also known as secondary healing) is the most common form of bone healing, usually consisting of stages of fibrocartilaginous callus formation, bony callus formation, and bone remodeling. The bone remodeling is initiated in mice from day 14 after amygdalin treatment. It is attributable to osteoclast-induced bony callus volume reduction. Radiographic union scores consist of callus formation and fracture line existence. Although there is no change of callus formation between groups, we observed fracture line and increased total radiographic union scores, which are the other indicators of improved fracture healing, in amygdalin-treated group. Fracture lines were clear at day 21 in the control group, but blurred in the amygdalin group at the same time point, indicating a better connection of cortical bone. Thus, biomechanical properties were improved with amygdalin treatment at day 21. Amygdalin treatment reduced the cartilage area and accelerated woven bone formation. However, amygdalin treatment did not increase the cartilaginous composition in early fracture callus compared to the control group. Because mineralization of the cartilaginous callus and formation of woven bone were increased by amygdalin treatment, the cartilage area of callus tissues began to decrease after day 14 compared to the control group. The transition from chondrogenesis to osteogenesis was associated with decreased gene expression of Sox9, a marker of chondrogenic differentiation [29], and increased expression of osteogenic markers (Runx2 and osteocalcin) after amygdalin treatment. Because of further mineralization, angiogenesis and endochondral bone formation can be regulated by the later cartilage hypertrophic marker Col10a1 [2931]. Similarly, Col10a1 expression was also upregulated in the amygdalin group at days 10 and 14. In addition to morphological changes, the mechanical properties of the bone could serve as an important indicator of fracture healing [32].

At the fracture site, angiogenesis and blood supply also has a direct influence on the fracture healing process. Abundant vascular distribution provides cells, growth factors, and some other constituents necessary for normal fracture healing [33, 34]. We performed angiography to examine how amygdalin impacts angiogenesis and found that it increased the volume of newly formed vessels in the cartilaginous bone. In our study, amygdalin significantly increased Vegf expression and CD31 protein expression in callus tissue; these findings were consistent with the results of increased angiogenesis. Previous reports revealed that angiogenesis can be induced by activation of TGF-β signaling [35, 36] and attenuated after inhibition of ALK5/Smad2/3 [37]. Collectively, amygdalin could promote angiogenesis during fracture healing, mainly dependent on the normal function of TGF-β/Smad signaling. In our study, amygdalin treatment could enhance phosphorylation of Smad2 at day 7 in vivo, indicating that amygdalin can upregulate TGF-β/Smad signaling during the fracture healing process.

During bone fracture healing, MSCs are recruited and differentiate into chondrocytes that generate cartilage extracellular matrix, which then mineralizes. Eventually, osteoblasts penetrate and promote osteogenesis [8, 38]. The fracture healing process is required for multiple cell types to repair bone structure [39]. Using lineage-tracing techniques in vivo, some experiments have shown that perinatal Sox9+, Col2+, or Agc1+ cells can produce osteoblasts and MSCs in mice [39]. Recently, however, a new type of cell, Gli1+ cells, were found to give rise to osteoblasts and chondrocytes in the process of bone fracture healing and to promote normal bone formation [21]. Gli1+ cells have been proposed to be MSCs in many bone-related studies [40, 41]. To determine whether amygdalin promotes chondrogenic and osteogenic differentiation of Gli1+ MSCs through TGF-β/Smad signaling, we tracked the fracture healing of Cre-negative and Tgfβr2Gli1-Cre mice treated with amygdalin. The MSC-specific loss of Tgfβr2 resulted in delayed maturation and mineralization of the cartilaginous callus. Remarkably, X-ray and μCT results showed delayed fracture healing in Tgfβr2Gli1-Cre mice, providing strong evidence that the stimulation of fracture healing by amygdalin depends on TGF-β/Smad signaling. Consistent with the in vivo results, both TGF-β1 and amygdalin-activated TGF-β/Smad signaling in MSCs promoted the migration of MSCs and chondrogenesis in vitro. Importantly, TGF-β/Smad inhibition by a TGF-β1 blocker attenuated MSC migration and the chondrogenic responses induced by TGF-β1 or amygdalin treatment in MSCs, confirming that amygdalin promotes facture healing in a TGF-β/Smad signaling-dependent mechanism.

In conclusion, this study demonstrated that amygdalin could promote the migration and differentiation of MSCs to accelerate the fracture healing process by regulating TGF-β/Smad signaling. These results support the use of amygdalin-based therapy for fracture healing.

Data Availability

The data in this study are available from the corresponding authors.

Conflicts of Interest

The authors have declared that no conflict of interest exists.

Authors’ Contributions

Jun Ying, Qinwen Ge, and Songfeng Hu contributed equally to this work.

Acknowledgments

This research has been partially supported by the Natural Science Foundation of China (Grant nos. 81774332, 81774346, 81873324, 81873325, 81904223, 81904221, 81804125, 81973869, and 81904219), the Zhejiang Provincial Natural Science Foundation of China (Grant no. LY18H270004), the State Administration of Traditional Chinese Medicine of Zhejiang Province (Grant nos. 2018ZA034, 2018ZZ011, 2019ZQ018, 2020ZA035, and 2020ZA117), the Health Commission of Zhejiang Province (Grant no. 2019RC225), the Opening Project of Zhejiang Provincial Preponderant and Characteristic Subject of Key University (Chinese Traditional Medicine), the Zhejiang Provincial Department of Education Research Project (Grant no. Y201839524), the Zhejiang Chinese Medical University (Grant nos. ZYX2018001, ZYX2018004, and ZYXYB2019003), the Young and Middle-Aged People Research Innovation Fund of Zhejiang University of Traditional Chinese Medicine (KC201932), the Excellent Youth Development Plan of Zhejiang University of Traditional Chinese Medicine (Q2019Y01), and the Cultivation Program for Innovative Talent Graduate Students (Grant no. 311100G00920).

References

  1. S. Amin, S. J. Achenbach, E. J. Atkinson, S. Khosla, and L. J. Melton, “Trends in fracture incidence: a population-based study over 20 years,” Journal of Bone and Mineral Research, vol. 29, no. 3, pp. 581–589, 2014. View at: Publisher Site | Google Scholar
  2. C. M. Court-Brown and B. Caesar, “Epidemiology of adult fractures: a review,” Injury, vol. 37, no. 8, pp. 691–697, 2006. View at: Publisher Site | Google Scholar
  3. S. R. Cummings and L. J. Melton, “Epidemiology and outcomes of osteoporotic fractures,” Lancet, vol. 359, no. 9319, pp. 1761–1767, 2002. View at: Publisher Site | Google Scholar
  4. O. Beytemur, C. Albay, O. Adanir, S. Yuksel, and M. A. Gulec, “Is intramedullary nailing applicable for distal tibial fractures with ankle joint extension?” Eklem Hastalik Cerrahisi, vol. 27, no. 3, pp. 125–131, 2016. View at: Publisher Site | Google Scholar
  5. H. J. Kim, J. M. Yi, H. G. Cho et al., “Comparative study of the treatment outcomes of osteoporotic compression fractures without neurologic injury using a rigid brace, a soft brace, and no brace: a prospective randomized controlled non-inferiority trial,” The Journal of Bone and Joint Surgery, vol. 96, no. 23, pp. 1959–1966, 2014. View at: Publisher Site | Google Scholar
  6. Y. C. Meng and X. H. Zhou, “External fixation versus open reduction and internal fixation for tibial pilon fractures: a meta-analysis based on observational studies,” Chinese Journal of Traumatology, vol. 19, no. 5, pp. 278–282, 2016. View at: Publisher Site | Google Scholar
  7. R. Zura, Z. Xiong, T. Einhorn et al., “Epidemiology of fracture nonunion in 18 human bones,” JAMA Surgery, vol. 151, no. 11, article e162775, 2016. View at: Publisher Site | Google Scholar
  8. T. A. Einhorn and L. C. Gerstenfeld, “Fracture healing: mechanisms and interventions,” Nature Reviews Rheumatology, vol. 11, no. 1, pp. 45–54, 2015. View at: Publisher Site | Google Scholar
  9. R. Marsell and T. A. Einhorn, “The biology of fracture healing,” Injury, vol. 42, no. 6, pp. 551–555, 2011. View at: Publisher Site | Google Scholar
  10. F. Loi, L. A. Cordova, J. Pajarinen, T. H. Lin, Z. Yao, and S. B. Goodman, “Inflammation, fracture and bone repair,” Bone, vol. 86, pp. 119–130, 2016. View at: Publisher Site | Google Scholar
  11. X. Wang, Y. Wang, W. Gou, Q. Lu, J. Peng, and S. Lu, “Role of mesenchymal stem cells in bone regeneration and fracture repair: a review,” International Orthopaedics, vol. 37, no. 12, pp. 2491–2498, 2013. View at: Publisher Site | Google Scholar
  12. U. Saran, S. Gemini Piperni, and S. Chatterjee, “Role of angiogenesis in bone repair,” Archives of Biochemistry and Biophysics, vol. 561, pp. 109–117, 2014. View at: Publisher Site | Google Scholar
  13. T. Fukuda, H. Ito, T. Mukainaka, H. Tokuda, H. Nishino, and T. Yoshida, “Anti-tumor promoting effect of glycosides from Prunus persica seeds,” Biological & Pharmaceutical Bulletin, vol. 26, no. 2, pp. 271–273, 2003. View at: Publisher Site | Google Scholar
  14. R. E. Heikkila and F. S. Cabbat, “The prevention of alloxan-induced diabetes by amygdalin,” Life Sciences, vol. 27, no. 8, pp. 659–662, 1980. View at: Publisher Site | Google Scholar
  15. J. Makarević, J. Rutz, E. Juengel et al., “Amygdalin influences bladder cancer cell adhesion and invasion in vitro,” PLoS One, vol. 9, no. 10, p. e110244, 2014. View at: Publisher Site | Google Scholar
  16. K. Niu, Y. J. Zhao, L. Zhang, C. G. Li, Y. J. Wang, and W. C. Zheng, “The synergistic effect of amygdalin and HSYA on the IL-1beta induced endplate chondrocytes of rat intervertebral discs,” Yao Xue Xue Bao, vol. 49, no. 8, pp. 1136–1142, 2014. View at: Google Scholar
  17. X. Zhang, J. Hu, Y. Zhuo et al., “Amygdalin improves microcirculatory disturbance and attenuates pancreatic fibrosis by regulating the expression of endothelin-1 and calcitonin gene-related peptide in rats,” Journal of the Chinese Medical Association, vol. 81, no. 5, pp. 437–443, 2018. View at: Publisher Site | Google Scholar
  18. Z. Wang, K. Fang, G. Wang et al., “Protective effect of amygdalin on epithelial-mesenchymal transformation in experimental chronic obstructive pulmonary disease mice,” Phytotherapy Research, vol. 33, no. 3, pp. 808–817, 2019. View at: Publisher Site | Google Scholar
  19. G. Chen, C. Deng, and Y. P. Li, “TGF-β and BMP signaling in osteoblast differentiation and bone formation,” International Journal of Biological Sciences, vol. 8, no. 2, pp. 272–288, 2012. View at: Publisher Site | Google Scholar
  20. J. L. Crane and X. Cao, “Bone marrow mesenchymal stem cells and TGF-β signaling in bone remodeling,” Journal of Clinical Investigation, vol. 124, no. 2, pp. 466–472, 2014. View at: Publisher Site | Google Scholar
  21. Y. Shi, G. He, W. C. Lee, J. A. McKenzie, M. J. Silva, and F. Long, “Gli1 identifies osteogenic progenitors for bone formation and fracture repair,” Nature Communications, vol. 8, no. 1, p. 2043, 2017. View at: Publisher Site | Google Scholar
  22. J. Shen, J. Li, B. Wang et al., “Deletion of the transforming growth factor β receptor type II gene in articular chondrocytes leads to a progressive osteoarthritis-like phenotype in mice,” Arthritis & Rheumatism, vol. 65, no. 12, pp. 3107–3119, 2013. View at: Publisher Site | Google Scholar
  23. M. Mi, H. Jin, B. Wang et al., “Chondrocyte BMP2 signaling plays an essential role in bone fracture healing,” Gene, vol. 512, no. 2, pp. 211–218, 2013. View at: Publisher Site | Google Scholar
  24. H. Jin, B. Wang, J. Li et al., “Anti-DKK1 antibody promotes bone fracture healing through activation of β-catenin signaling,” Bone, vol. 71, pp. 63–75, 2015. View at: Publisher Site | Google Scholar
  25. M. Wu, G. Chen, and Y. P. Li, “TGF-β and BMP signaling in osteoblast, skeletal development, and bone formation, homeostasis and disease,” Bone Research, vol. 4, no. 1, 2016. View at: Publisher Site | Google Scholar
  26. N. T. Florence, S. T. S. Huguette, D. J. Hubert et al., “Aqueous extract of Peperomia pellucida (L.) HBK accelerates fracture healing in Wistar rats,” BMC Complementary and Alternative Medicine, vol. 17, no. 1, p. 188, 2017. View at: Publisher Site | Google Scholar
  27. N. Guzel, E. Sayit, O. Aynaci, S. Kerimoglu, E. Yulug, and M. Topbas, “Ginkgo biloba improves bone formation during fracture healing: an experimental study in rats,” Acta Ortopédica Brasileira, vol. 25, no. 3, pp. 95–98, 2017. View at: Publisher Site | Google Scholar
  28. V. Khedgikar, P. Kushwaha, N. Ahmad et al., “Ethanolic extract of Dalbergia sissoo promotes rapid regeneration of cortical bone in drill-hole defect model of rat,” Biomedicine & Pharmacotherapy, vol. 86, pp. 16–22, 2017. View at: Publisher Site | Google Scholar
  29. S. Narakornsak, S. Aungsuchawan, P. Pothacharoen et al., “Sesamin encouraging effects on chondrogenic differentiation of human amniotic fluid-derived mesenchymal stem cells,” Acta Histochemica, vol. 119, no. 5, pp. 451–461, 2017. View at: Publisher Site | Google Scholar
  30. U. I. Chung, E. Schipani, A. P. McMahon, and H. M. Kronenberg, “Indian hedgehog couples chondrogenesis to osteogenesis in endochondral bone development,” Journal of Clinical Investigation, vol. 107, no. 3, pp. 295–304, 2001. View at: Publisher Site | Google Scholar
  31. F. Kugimiya, H. Kawaguchi, S. Kamekura et al., “Involvement of Endogenous Bone Morphogenetic Protein (BMP) 2 and BMP6 in Bone Formation,” Journal of Biological Chemistry, vol. 280, no. 42, pp. 35704–35712, 2005. View at: Publisher Site | Google Scholar
  32. P. Augat, M. Faschingbauer, K. Seide et al., “Biomechanical methods for the assessment of fracture repair,” Injury, vol. 45, Supplement 2, pp. S32–S38, 2014. View at: Publisher Site | Google Scholar
  33. L. Geris, A. Gerisch, J. V. Sloten, R. Weiner, and H. V. Oosterwyck, “Angiogenesis in bone fracture healing: a bioregulatory model,” Journal of Theoretical Biology, vol. 251, no. 1, pp. 137–158, 2008. View at: Publisher Site | Google Scholar
  34. R. E. Tomlinson and M. J. Silva, “Skeletal blood flow in bone repair and maintenance,” Bone Research, vol. 1, no. 4, pp. 311–322, 2013. View at: Publisher Site | Google Scholar
  35. E. Pardali, M. J. Goumans, and P. ten Dijke, “Signaling by members of the TGF-beta family in vascular morphogenesis and disease,” Trends in Cell Biology, vol. 20, no. 9, pp. 556–567, 2010. View at: Publisher Site | Google Scholar
  36. L. A. van Meeteren, M.-J. Goumans, and P. ten Dijke, “TGF-β Receptor Signaling Pathways in Angiogenesis; Emerging Targets for Anti-Angiogenesis Therapy,” Current Pharmaceutical Biotechnology, vol. 12, no. 12, pp. 2108–2120, 2011. View at: Publisher Site | Google Scholar
  37. S. Lin, J. Xie, T. Gong et al., “Smad signal pathway regulates angiogenesis via endothelial cell in an adipose-derived stromal cell/endothelial cell co-culture, 3D gel model,” Molecular and Cellular Biochemistry, vol. 412, no. 1-2, pp. 281–288, 2016. View at: Publisher Site | Google Scholar
  38. A. Oryan, S. Monazzah, and A. Bigham-Sadegh, “Bone injury and fracture healing biology,” Biomedical and Environmental Sciences, vol. 28, no. 1, pp. 57–71, 2015. View at: Publisher Site | Google Scholar
  39. P. Wang, J. Ying, C. Luo et al., “Osthole promotes bone fracture healing through activation of BMP signaling in chondrocytes,” International Journal of Biological Sciences, vol. 13, no. 8, pp. 996–1007, 2017. View at: Publisher Site | Google Scholar
  40. J. Feng, J. Jing, J. Li et al., “BMP signaling orchestrates a transcriptional network to control the fate of mesenchymal stem cells in mice,” Development, vol. 144, no. 14, pp. 2560–2569, 2017. View at: Publisher Site | Google Scholar
  41. H. Zhao, J. Feng, T. V. Ho, W. Grimes, M. Urata, and Y. Chai, “The suture provides a niche for mesenchymal stem cells of craniofacial bones,” Nature Cell Biology, vol. 17, no. 4, pp. 386–396, 2015. View at: Publisher Site | Google Scholar

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