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Biomaterials Research

Research article
Open Access

Regeneration of rabbit calvarial defects using cells-implanted nano-hydroxyapatite coated silk scaffolds

  • Jin-Young Park1,
  • Cheryl Yang1,
  • Im-Hee Jung3,
  • Hyun-Chang Lim1,
  • Jung-Seok Lee1,
  • Ui-Won Jung1,
  • Young-Kwon Seo2,
  • Jung-Keug Park2 and
  • Seong-Ho Choi1Email author
Biomaterials Research201519:7

https://doi.org/10.1186/s40824-015-0027-1

©  Park et al.; licensee BioMed Central. 2015

Received: 4 January 2015

Accepted: 24 February 2015

Published: 21 March 2015

Abstract

Background

The aim of this study was to characterize the efficacy of nano-hydroxyapatite-coated silk fibroin constructs as a scaffold for bone tissue engineering and to determine the osteogenic effect of human dental pulp and periodontal ligament derived cells at an early stage of healing in rabbits. 3D silk fibroin constructs were developed and coated using nano-hydroxyapatite crystals. Dental pulp and periodontal ligament cells from extracted human third molars were cultured and seeded onto the silk scaffolds prior to in vivo implantation into 8 male New Zealand White rabbits. Four circular windows 8 mm in diameter were created in the calvarium of each animal. The defects were randomly allocated to the groups; (1) silk scaffold with dental pulp cells (DPSS), (2) silk scaffold with PDL cells (PDLSS), (3) normal saline-soaked silk scaffold (SS), and (4) empty control. The animals were sacrificed 2 (n = 4) or 4 weeks (n = 4) postoperatively. The characteristics of the silk scaffolds before and after cell seeding were analyzed using SEM. Samples were collected for histologic and histomorphometic analysis. ANOVA was used for statistical analysis.

Result

Histologic view of the experimental sites showed well-maintained structure of the silk scaffolds mostly unresorbed at 4 weeks. The SEM observations after cell-seeding revealed attachment of the cells onto silk fibroin with production of extracellular matrix. New bone formation was observed in the 4 week groups occurring from the periphery of the defects and the silk fibers were closely integrated with the new bone. There was no significant difference in the amount of bone formation between the SS group and the DPSS and PDLSS groups.

Conclusion

Within the limitations of this study, silk scaffold is a biocompatible material with potential expediency as an osteoconductive scaffold in bone tissue engineering. However, there was no evidence to suggest that the addition of hDPCs and hPDLCs to the current rabbit calvarial defect model can produce an early effect in augmenting osteogenesis.

Keywords

Bone regenerationSilk scaffoldNano-hydroxyapatiteTissue engineering

Background

Bone grafting has numerous applications in dentistry such as alveolar ridge augmentation during implant therapy and reconstructive surgeries involving large bone defects. The preferred treatment is autograft, known to produce the best clinical outcome due to its osteogenic cellular component [1]; however, the use of autologous bone has its limitations due to donor site morbidity, increased surgery time and limited quantity [2,3]. Hence bone substitute materials of various organic and synthetic origins are commercially manufactured and used to provide the osteoconductive bulk upon which healing at the cellular level can be induced. Tissue engineering concepts have recognized the potential for graft materials to benefit from the addition of stem/progenitor cells aimed at enhancing the rate and quality of defect repair. According to the principles of tissue engineering, elements of successful bone regeneration include osteoblastic progenitor cells, suitable growth factors and an osteoconductive scaffold that allows the formation of vascular network [4,5].

The ideal requirements of bone tissue engineering scaffolds include biocompatibility, appropriate chemistry, morphology and structure to promote growth and differentiation of osteoblastic progenitor cells for synthesis of new bone matrix [5]. Silk fibroin is a promising biomaterial that has been used for both in vitro and in vivo applications due to the mechanical strength, biocompatibility, and a slow degradation rate that enables gradual replacement of fibroin with newly formed tissue [2]. Natural bone extracellular matrix consists of a loose network of collagen fibrils and hydroxyapatite crystals. Osteoconductive and osteoinductive properties of the scaffold can be reinforced by the addition of mineral hydroxyapatite (HA) due to its structural similarities to natural bone extracellular matrix. Incorporation of HA was shown not only to enhance the surface characteristics of the scaffold by increasing its roughness, but also promote viability of stem cells and their proliferation [6].

Cytocompatibility of silk scaffold and the subsequent formation of extracellular matrix onto silk fibroin have been demonstrated previously [7]. Addition of a cellular component may improve the osteoinductivity of a scaffold and help to increase the speed of bone formation. Various stem cells such as bone marrow stem cells, adipose tissue-derived stem cells and embryonic stem cells have been widely used in studies of bone tissue engineering [8-10]. Bone marrow derived mesenchymal stem cells (BMMSCs) in particular are the most studied, and have been shown to be capable of differentiating into multiple cell lineages including osteogenic, chondrogenic, adipogenic, myelosupportive stroma, myogenic, and neurogenic lineages. But due to certain shortcomings of obtaining the BMMSCs including pain, morbidity, and low cell number upon harvest, alternative sources for MSCs have been sought. Dental tissues are specialized tissues that do not undergo continuous remodeling; therefore dental tissue derived progenitor cells may be more restricted in differentiation potency in comparison to BMMSCs. Nevertheless, dental tissue derived cells can be easily acquired from tooth extractions and recent studies have proven dental stem cells to be a potent source for fabrication of bone structures [11]. This is due to their good osteogenic activity potentially as a result of their biological function to form hard mineralized tissue during tooth development [11]. Dental pulp stem cells (DPSCs) isolated from the dental pulp tissue could differentiate into osteoblastic precursors under stimulatory conditions, and were able to synthesize living fibrous bone tissue in vitro. Furthermore, following transplantation of the bone matrix into immunocompromised rats, lamellar bone tissues containing osteocytes were generated [12]. Several studies have demonstrated successful use of DPSCs seeded in scaffolds. For example, porous calcium phosphate ceramic discs [13], resorbable collagen sponges [14,15] and poly(lactic-co-glycolic acid) copolymers [16] have all been used to construct adequate cell-scaffold matrices for in vivo transplantations.

Osteogenic differentiation of cultured periodontal ligament stem cells (PDLSCs) has also been reported [17-19]. In vivo transplantation of PDLSCs into periodontal defects showed regeneration of the periodontal tissues, identified to be closely related to the adjacent trabecular bone, suggesting their involvement in alveolar bone regeneration [17]. Subsequent studies containing in vitro and in vivo experiments have shown use of PDLSCs with bone tissue engineering scaffolds such as nano-hydroxyapatite coated chitosan [20] and in vitro-derived extracellular matrix [21].

In the present study, a collective population of cells from the human dental pulp (DPCs) and periodontal ligament (PDLCs) were isolated and cultured. The rabbit calvarial defect model was used to evaluate the efficacy of the SF construct for bone regeneration in vivo, and to determine whether the addition of cellular component may improve the rate and quality of defect repair.

Methods

Preparation of silk scaffolds coated with nano-hydroxyapatite

Silk sutures were purchased from Won Corporation (Seoul, South Korea) and silk scaffolds were constructed using a weaving machine. The silk scaffolds were processed by extracting sericin, a glue-like protein that coats the native silk fibroin, using an aqueous solution containing 0.02 M Na2CO3 and 0.3% Ivory detergent. 0.15 g of nano-hydroxyapatite (Sigma) was dissolved in 10 ml of PBS and 1ml of the solution was dried on the silk scaffold (0.8×1.2 cm) in air. The scaffolds were then soaked in a 1% type atelocollagen solution (Bioland, Korea) and lyophilized in a freeze dryer (Samwon Freezing Engineering Co., Korea) at −80°C for 48 h. The silk scaffolds were incubated in 20 ml of 40% (v/v) ethanol containing 50 mM 2-morpholineoehtane sulfonic acid (MES, Fluka Chemic AG) (pH 5.5) for 30 min at room temperature. The silk scaffolds were then immersed in 20 ml of 40% (v/v) ethanol containing 50 mM MES (pH 5.5), 24 mM 1-ethyl-3-(3-dimethyl aminopropyl) carbodiimide (Fluka Chemic AG) and 5 mM N-hydroxysuccinimide (Fluka Chemic AG) for 12 h at room temperature. Once the reaction was complete, the composite silk scaffold was washed twice in 0.1 M Na2HPO4 (pH9.0) for 12 h. The scaffolds were washed twice in 1 M NaCl for 6 h, then in 2 M NaCl for 2 days and finally rinsed with distilled water. The washed scaffolds were lyophilized again and sterilized with γ-irradiation at 15 KGy.

Primary cell culture

DPCs

Extracted third molars were used in experiments with the approval of patients. The patients provided informed consent for their tissue being used in accordance with guidelines approved by the Institutional Review Board, College of Dentistry, Yonsei University (IRB No. 2-2010-0009). The extracted third molars were washed with PBS containing antibiotic antimycotic (AA) (Welgene, Korea) for 3 mins after washing with 70% ethanol. The third molars were wavered with pliers and the dental pulp was removed. The pulp tissues were digested in a solution of 3 mg/mL collagenase type I (Sigma St. Louis, Mo., USA) and 4 mg/mL dispase (Siga, St. Louis, MO., USA) for 12 h at 4°C. The pulp tissue was then incubated in 3 mL of 0.25% trypsin for 15 min at 37°C. After trypsin digestion, the trypsin solution was diluted in alpha Modified Eagle’s Medium (α-MEM, Sigma) containing 10% fetal bovine serum (FBS, BioWhittakerTM, Cambrex, MD, USA). The cells were isolated from the dental pulp by pipetting. After centrifugation at 800 rpm for 5 min, the supernatant was removed and added to 10 mL of α-MEM. The cell suspensions were seeded in 100 mm culture dishes.

PDLCs

Human periodontal tissue was obtained from several extracted third molars of patients who had given their informed consent (IRB No. 2-2010-0009). The extracted third molars were washed with PBS containing antibiotic antimycotic solution (AA) (Welgene, Korea) for 3 min after washing with 70% ethanol.

The periodontal tissue was removed from the roots of the teeth and then divided into small pieces with scissors and tissues were digested in a solution of 3 mg/mL collagenase type I (Sigma, St. Louis, MO, USA) and 4 mg/mL Protease (Sigma, P 3417, USA) for 12 h at 4°C. Then, PDL tissues were incubated in 3 mL of 0.25% trypsin for 15 min at 37°C. After trypsin digestion, the trypsin solution was diluted with alpha Modified Eagle’s Medium (α-MEM, Sigma) containing 10% fetal bovine serum (FBS, BioWhittakerTM, Cambrex, MD, USA).

After centrifuging at 800 rpm for 5 min, the supernatant was removed and pipetted with 10 mL of α-MEM. The cell suspensions were seeded in 100 mm culture dish. The PDL fibroblasts from third to five passages were used.

Seeding of cells in silk scaffolds

DPCs and PDLCs, suspended in alpha Modified eagle’s Medium (α-MEM, Sigma) supplemented with 10% fetal bovine serum (FBS, BioWhitekerTM, Cambrex Bioscience Walkersville, Inc., MD), were seeded onto the silk scaffolds. To obtain a very high cell seeding density, the cells were seeded onto the silk scaffolds under a dried condition. 100 μl of a harvested suspension – containing 2.8 × 104 human dental pulp cells or 1 × 106 human PDL cells – and silk scaffolds were placed in the petri dish in a humidified 5% CO2 incubator, and 3h later, 10 ml of α-MEM was added to the petri dish. The medium was replaced every 3 days for 7 days. After incubation for additional 7 days, the scaffolds were cultured in differentiation medium, which was replaced every 2 days for 3 weeks. The differentiation medium for DPCs was alpha Modified Eagle’s Medium (α-MEM, Sigma) supplemented with 10% fetal bovine serum (FBS, BioWhittakerTM, Cambrex, MD, USA), 1% AA, 100 nM dexamethasone, 0.05 mM Ascorbic acid and 10 mM β-glycerophospate. The differentiation medium for PDLCs was α-MEM containing 10% FBS, 10 mM β-glycerophosphate (Sigma), 50 μM L-ascorbate2-phosphate (Sigma) and 10−7 M dexamethasone (Sigma). The result of cell-seeding procedure was checked with scanning electron microscopy.

Animals

Eight male New Zealand White rabbits weighing 2.8-3.2 kg and age 16–20 weeks were used in this study. Animal selection and management, surgical protocol and preparation followed the routines approved by the Institutional Animal Care and Use Committee, Yonsei Medical Center, Seoul, Korea.

Study design

Four circular defects (8mm diameter) were created in each animal, which were randomly allocated to the four study groups including PDLC-silk scaffold group (PDLSS group), DPC-silk scaffold group (DPSS group), normal saline-soaked silk scaffold group (SS group) and an empty control group. The animals were euthanized at either 2 or 4 weeks postsurgery.

Surgical protocol

General anaesthesia was induced in all animals using intramuscular injections of zoletil (15 mg/kg) and rompun (5 mg/kg). The head of the rabbit was shaved and disinfected using povidone iodine prior to local anaesthetic injections at the surgical site using 2.2 ml Lidocaine Hydrochloride 2% with adrenaline 1:80,000. An incision was made along the midline from the frontal bone to the occipital bone and a full-thickness flap was elevated. Under copious saline irrigation, four standardized round defects 8 mm in diameter were created using a trephine bur (Figure 1). The resected bones were removed carefully to avoid injury to the underlying brain tissue. The defects were filled with the experimental materials according to the assigned group. The flaps were repositioned and sutured with resorbable suture material.
Figure 1
Figure 1

Surgical procedure. A. Four standardized defects 8 mm in diameter were created using a trephine bur. B. The defects in each animal were assigned into four groups. Clockwise from bottom left: sham control, silk scaffold (SS), dental pulp cells seeded on SS (DPSS), periodontal ligament cells seeded on SS (PDLSS). C. The silk scaffold was made at 8 mm in diameter in order to fit into the defects.

The animals were sacrificed at either 2 or 4 weeks postsurgery. The skin flaps were reflected to expose the periosteum and the entire calvarium was resected and harvested from each animal.

Histologic processing

Block sections of the surgical sites were fixed in 10% formalin for 10 days. The fixed specimens were decalcified in 5% formic acid for 14 days and then embedded in paraffin. Serial 5 μm thick sections were cut along the midline of the calvarial defects. Only sections located at the middle of the defects were selected, and stained with hematoxylin-eosin for histologic and histometric analysis.

Analysis methods

Histomorphometric analysis

After the conventional microscopic examination, computer-assisted histometric measurements in the calvarial defect were performed using an automated image analysis system (Image-Pro Plus; Media Cybernetics, Silver Spring, MD). The following parameters were measured from each histologic section of the defect areas.

  • Total augmented area (mm2) – Total sum of the area of new bone, residual particles, connective tissue, adipose tissue, blood vessels within the defect area.

  • Residual material (mm2) – Area of the remaining silk scaffold within the defect.

  • New bone (mm2) – Area of newly formed bone within the defect.

Statistical analysis

The statistical analysis was performed using a commercially available software program (SPSS 18.0, SPSS, Chicago, IL). Histomorphometric records from the calvarial defect samples were used to calculate the mean and standard deviation (SD) values of groups. One-way analysis of variance (ANOVA) was used to analyze the difference between the groups at 2 and 4 weeks. Statistical significance was considered when P <0.05.

SEM observations

The morphology of nHA-coated scaffolds before and after the cell-seeding procedure were observed by scanning electron microscopy (SEM; S-3000N, Hitachi, Tokyo, Japan) at an accelerating voltage of 30 kV.

Clinical and histological findings

Throughout the healing periods, the animals were carefully monitored for adverse reactions around the surgical site. The specimens were examined by a single, blinded examiner with the aid of a binocular microscope (DM LB, Leica Microsystems, Wetzlar, Germany) equipped with a camera (DC300F, Leica Microsystems). Images of the slides were acquired and saved as digital files.

Results

SEM observations of nHA-coated silk scaffolds

SEM observations of the surface of the nHA-coated silk scaffold revealed a combination of porous architecture of the silk fibroin. A closer examination at a higher magnification revealed organization of the fibrous structures into bundles. Cross-sectional view revealed interconnected porous structure of the silk fibroin construct. Pore sizes varied between 20–80 μm with mean pore diameter of 65 μm (Figure 2A). Longitudinal sections showed an internal structure with fibrous bundles mainly oriented parallel to the scaffold surface.
Figure 2
Figure 2

Scanning electron microscopy images. A and B shows the cross section and longitudinal section of the silk scaffold respectively prior to the cell culture. Porous, interconnected structure can be observed, ×100 magnification. C and D show the cross section and longitudinal section of the silk scaffold respectively, following the cell culture, ×400 magnification. Arrows represent spreading of the cells with secreted extracellular matrix on the silk fibroin. Arrowheads represent nHA crystals on silk fibroin.

At 400 magnification view (Figure 2C, D) homogenous distribution of nano-HA crystals on pure silk fiber substrates can be observed as small round granules. In parts, nHA crystals displayed formation of clusters with attachment of the cellular matrix. The implanted cells were well spread out and attached to the surfaces of scaffolds. Also, the formation of an ECM was observed. This is a typical response that is indicative of cytocompatibility and adaptation of the cells onto silk fibroin.

Clinical findings

Healing of all surgery sites was without any adverse reactions or postoperative complications such as abnormal bleeding or infection. Signs of inflammation such as swelling appeared to be minimal, and the grafted materials were confirmed to be intact within the defects at the time of sacrifice and sample collection.

Histologic & histomorphometric analysis

In the control group, negligible amount of new bone formation was observed. The defect spaces were filled by the underlying brain tissues as well as the overlying periosteum that was collapsed into the vacant space.

In DPSS, PDLSS and SS groups, the silk fibroin constructs occupied the defect spaces and exhibited well-maintained structure in all sites. The scaffolds were superficially covered by the overlying periosteum and the silk fibers were surrounded by the connective tissue of ECM comprising loose collagen network stained by the light blue coloration of Masson’s trichrome staining.

At 2 weeks, the interconnected porous structures were occupied by the inflammatory cells mainly macrophages, which were evenly distributed (Figure 3). The scaffold showed compact arrangement of silk fibers organized into bundles and blood vessels formed vascular networks around the bundles of silk fibroin. Minimal new bone formation was observed (Figure 4).
Figure 3
Figure 3

Histological view of the groups at 2 weeks postoperatively. A – DPSS group, B – PDLSS group, C – SS group. All experimental groups showing inflammatory cells mainly macrophages evenly distributed around the silk scaffold. ×200 magnification, Mason’s trichrome staining.

Figure 4
Figure 4

Histological view of the groups at 2 weeks postoperatively. A –control group shows negligible amount of bone formation. Minimal bone formation observed in: B – SS group, C – PDLSS group, D – DPSS group, ×40 magnification, Mason’s trichrome staining.

At 4 weeks, the inflammatory cells no longer existed around the fibrous network. Angiogenesis had occurred surrounding the fibrous bundles evident by the appearance of blood vessels, however none were seen to penetrate the internal structure of the porous network. ECM appeared visibly denser than at 2 weeks and early new bone formation was observed occurring mainly from the periphery of the defects. The newly formed bone was seen to be in close contact with the individual fibers of silk scaffold (Figure 5).
Figure 5
Figure 5

Histological view of the groups at 4 weeks postoperatively. A – Control group shows negligible amount of bone formation. B – SS group, C – PDLSS group, D – DPSS groups all display early bone formation at the periphery of the defects shown by the arrows. ×40 magnification, Mason’s trichrome staining.

Histomorphometric analysis revealed no statistical significance between DPSS, PDLSS and SS groups in terms of the area of new bone (Table 1, Figure 6). However, the total augmented area showed to be significantly greater in the DPSS, PDLSS and SS groups compared to the control group, which invariably is due to the unresorbed silk fiber constructs at both 2 and 4 weeks. There was no remarkable difference in the appearance of the remaining silk fibers between the two time periods in all groups, and histomorphometric analysis showed no significant difference in the area of residual material between 2 and 4 weeks.
Table 1

Total grafted area, new bone area, remaining material at 2 and 4 weeks

 

Parameters (mm 2 )

Control

SS

DPSS

PDLSS

2 Weeks

Total grafted area

6.2 ± 1.7

*11.66 ± 2.1

*12.46 ± 1.63

*10.68 ± 0.91

 

New bone area

1.13 ± 0.88

0.4 ± 0.13

0.84 ± 0.93

0.7 ± 0.5

 

Remaining material

NA

3.9 ± 1.5

6.15 ± 2.5

5.77 ± 2.7

4 Weeks

Total grafted area

7.63 ± 1.38

*15.47 ± 4.37

*13.28 ± 1.23

*13.35 ± 1.17

 

New bone area

1.37 ± 0.29

1.36 ± 0.47

0.67 ± 0.39

0.54 ± 1.23

 

Remaining material

NA

4.61 ± 0.62

5.83 ± 1.27

5.29 ± 1.15

*Significantly different from the control (P < 0.05).

SS – silk scaffold.

DPSS – dental pulp cells with silk scaffold.

PDLSS – periodontal ligament cells with silk scaffold.

Figure 6
Figure 6

Graphs showing total grafted area, new bone area, remaining material (mm 2 ). A – after 2 weeks of healing, B – after 4 weeks of healing.

Discussion

Silk fibroin is a promising material due to its excellent mechanical strength, biocompatibility and porous architecture to act as the artificial extracellular matrix required for 3D tissue engineering application. The objectives of this study were to evaluate the efficacy of silk fibroin constructs for the regeneration of bone defects and determine the effect of the added cellular components in vivo. The current experimental model has previously been shown to be suitable for the evaluation of bone substitutes at the early stage of healing when study periods of 2 and 4 weeks were combined [22]. Negligible amount of bone formation was noticed in the defects of the control group at both 2 and 4 weeks as the surrounding soft tissue structures appeared to have collapsed into the defect spaces. The histomorphometric analysis shows that all the experimental groups had greater total augmented area than the control group at both 2 and 4 weeks, however, no significant difference was revealed in regards to the area of new bone between the groups. This result indicates that the silk scaffold was effective in maintaining the defect space for at least 4 weeks, but the addition of cellular components had no effect in the amount of bone regeneration.

Silk fibroin scaffolds have been demonstrated to be mechanically robust in previous studies [23,24]. In the present study, the grafted volumes were well maintained in all of the experimental groups which had led to new bone formation occurring from the periphery of the defects. The early new bone appeared to be in close contact with the fibrous bundles of the silk scaffold, and the provisional collagen matrix seemed to surround the individual silk fibers without any adverse reaction. This histologic evidence demonstrates biocompatibility of the silk fibroin in vivo to act as the osteoconductive basis for bone regeneration. Silk fibroin is known for its biocompatibility and low immunogenicity following implantation once rendered devoid of sericin, a glycosylated protein emitting immunogenicity [25]. In vitro studies have demonstrated that silk is enzymatically broken down by a family of proteases directly into peptides and amino acids, which indicates that the biodegradation products of silk fibroin do less or no harm to the human body [26]. In this study, inflammatory cells mainly macrophages were found evenly distributed within the scaffold at 2 weeks. However, no abnormal clinical findings were observed during follow up of the animals, and the inflammatory cells had completely vanished at 4 weeks suggesting that this would have been part of the normal wound healing sequence. Macrophages are known to predominantly appear during the inflammatory phase of the wound healing and contribute to inducing angiogenesis and laying down a new ECM. At 4 weeks, denser collagenous provisional matrix was observed throughout the scaffold, evident by the increased blue coloration around the SF by the Masson’s trichrome staining and formation of blood vessels around the fibrous bundles. However, the vascular network failed to penetrate the bundles of silk fibers. This could be due to the compact organization of the fibrous bundles as well as the lack of biodegradation of the material in order to accommodate sufficient space for angiogenesis.

The silk fibroin constructs remained unresorbed after 4 weeks in this study. This is concurrent with previous literature in which silk was demonstrated to be proteolytically biodegraded and resorbed in vivo typically within a year [26]. The slow biodegradation of silk may be responsible for the small amount of bone formation in all experimental groups, as new bone formation cannot occur if the defect space is already occupied. In vivo degradation kinetics of the silk scaffold should closely match the functional needs and mechanical properties specific to the defect type [27]. In consideration of slow degradation, mechanical toughness and the pattern of bone formation occurring from the periphery, SF constructs could be advantageously used in highly loaded areas where cortical bridging and long-term support of function is critical. In non-stress bearing defects such as the one used for this study, long term support may not be necessary but rather dynamic resorption of the implant material and bone remodeling occurring synchronously in a gradual substitution process [28]. Hence, timely resorption of SS can be considered favorable in the promotion of osteogenesis. It has been shown that resorption rate of silk fibroin can be modulated by varying the pore size, crystallinity and molecular weight distribution [29]. Wang et al. have shown that the in vivo behavior of silk fibroin can be predictably altered and controlled to match the tissue-specific requirements of the scaffold characteristics and resorption rates [30]. Furthermore, acid-degraded silk fibroin fragments with low molecular weight has been shown to produce highly osteogenic properties by inducing increases in ALP, type-I collagen and fibronectin levels [31].

The present study incorporated the use of nHA-coated silk fibroin. Although a control group containing pure silk scaffold without nHA-coating may have demonstrated potential benefits of the nHA-coating, the primary end point in the current study was to investigate the effects of the addition of two cellular components in osteogenesis. Furthermore, in vitro studies [32,33] have demonstrated that nHA-coating on silk fibroin may improve cytocompatibility compared to the pure silk fibroin. Fibrous substrates have been shown to support cell attachment, proliferation and differentiation, while the hydroxyapatite constituent promotes the secretion of ECM for mineralization of new bone [34]. The degradation of nHA changes the Ca/P metabolism and triggers the activation of osteoblasts [35]. The nHA particles showed higher calcium release and increased osteoblast attachment than the conventional sized HA. The SEM appearance of the nHA crystals with overlying ECM is a concurrent finding to the reports in previous studies. In vitro study by Wei et al. [36] suggested that surface topography had a crucial influence on cell behavior, which was accompanied by attenuated proliferation rates on rougher surfaces. Nevertheless, after 2 weeks of cultivation, cell number of osteoblasts on mineralized silk was slightly higher than that on pure silk.

In the present study, the DPCs and PDLCs were cultured and seeded onto the nHA-coated SF constructs for 3 weeks. It has been shown that pre-culture of cells on silk scaffold prior to implantation improved the distribution of ECM mineralization due to better cell distribution within the scaffold [7]. Ideally, greater quantity of ECM should be produced with a larger number of cells. However, large cell numbers on silk scaffolds might be counter-productive for cell-attachment due to limited scaffold surface area. The cells were prepared according to a coherent protocol to existing literatures, in which osteoblastic precursors were obtained in vitro, and successful bone regeneration was achieved in vivo [11,12,20,37]. The SEM observations of the silk fibroin constructs after cell culture showed presence of the cellular components surrounded by ECM.

The silk scaffold used in the present study contained mean pore diameter of 65 μm. Due to scaffold shrinkage during drying this pore size is likely to be a reduced figure, which would be reversible when scaffolds were again placed in liquid. A previous study [7] demonstrated that small scaffold pores with average pore diameters below 100 μm did not constrain medium penetration into the middle of the scaffold, even in a static set-up. On the other hand, the smallest pores (61.6 ± 5.0 μm) presented the largest growth surface to the cells and allowed better migration of cells to the inner most parts of the scaffold resulting in more homogenous distribution of mineralized tissue, despite the general belief that larger pores improve cell and medium distribution.

However, histologically at 2 and 4 weeks in vivo, no significant difference in the amount of bone formation was observed in both DPSS and PDLSS groups compared to the SS group. A possible explanation could be that the proportion of stem cells within the cultured population may not have been enough to produce a significant impact on bone formation. The purity of the stem cells could have been enriched by initial validation of their ability to generate clonogenic cell clusters in vitro followed by further isolation of the stem cells using protocols such as magnetic bead cell separation based on the expression of mesenchymal stem cell associated markers [38].

In addition, xenogeneic cells of human origin were transplanted into rabbits that were not immunocompromised. The lack of host-verses-graft response at the grafted sites may be attributed to the initial scarcity of blood vessels at the site of implantation as well as the isolated nature of the contained-type defects in the calvaria. Had allogeneic cells been used, it remains possible that greater synergy might have been achieved. Previous studies have shown that although xenogeneic supply of mesenchymal stem cell (MSC) are likely to be rejected by the host after transplantation, allogeneic MSCs are well-tolerated by the recipient hosts [39]. DPSCs have also been shown to possess immunosuppressive effects [40].

Furthermore, it is impossible to verify in the present study whether new bone originated from the grafted cells or native cells. Future studies should employ cell labelling techniques to confirm that neo-osteogenesis derived from the recruited hDPCs and hPDLCs rather than the endogenous rabbit MSCs that could have migrated to the defect site.

Conclusions

In summary, the results supported the biocompatibility of nHA-coated silk and its potential usefulness as an osteoconductive scaffold. However, there is a lack of evidence to suggest that using the current method of preparation, hPDLCs and hDPCs can produce an early effect in bone regeneration. Resorption rate of the silk fibroin should be modulated in order to promote timely substitution of the silk fibroin by living tissues. Further studies should be performed using confirmed stem cell population with longer healing periods for proper evaluation of its effects.

Availability of supporting data

The data sets supporting the results of this article are included in the article.

Declarations

Acknowledgement

This study was supported by a grant of the Korea Health technology R & D 567 Project, Ministry of Health & Welfare, Republic of Korea (101578).

Authors’ Affiliations

(1)
Department of Periodontology, Research Institute of Periodontal Regeneration, Yonsei University College of Dentistry, Seoul, South Korea
(2)
Department of Medical Biotechnology, Dongguk University, Seoul, South Korea
(3)
Department of Dental Hygiene, College of Health Sciences, Eulji University, Seong-nam, Republic of Korea

References

  1. Petite H, Viateau V, Bensaid W, Meunier A, de Pollak C, Bourguignon M, et al. Tissue-engineered bone regeneration. Nat Biotechnol. 2000;18(9):959–63.View ArticleGoogle Scholar
  2. Park SY, Ki CS, Park YH, Jung HM, Woo KM, Kim HJ. Electrospun silk fibroin scaffolds with macropores for bone regeneration: an in vitro and in vivo study. Tissue Eng Part A. 2010;16(4):1271–9.View ArticleGoogle Scholar
  3. Kim HJ, Kim UJ, Kim HS, Li C, Wada M, Leisk GG, et al. Bone tissue engineering with premineralized silk scaffolds. Bone. 2008;42(6):1226–34.View ArticleGoogle Scholar
  4. Neman J, Hambrecht A, Cadry C, Jandial R. Stem cell-mediated osteogenesis: therapeutic potential for bone tissue engineering. Biologics. 2012;6:47–57.Google Scholar
  5. Pacifici L, Casella F, Ripari M. [The principles of tissue engineering: role of growth factors in the bone regeneration]. Minerva Stomatol. 2002;51(9):351–9.Google Scholar
  6. Jiang J, Hao W, Li Y, Yao J, Shao Z, Li H, et al. Hydroxyapatite/regenerated silk fibroin scaffold-enhanced osteoinductivity and osteoconductivity of bone marrow-derived mesenchymal stromal cells. Biotechnol Lett. 2013;35(4):657–61.View ArticleGoogle Scholar
  7. Thimm BW, Wust S, Hofmann S, Hagenmuller H, Muller R. Initial cell pre-cultivation can maximize ECM mineralization by human mesenchymal stem cells on silk fibroin scaffolds. Acta Biomater. 2011;7(5):2218–28.View ArticleGoogle Scholar
  8. Correia C, Grayson W, Eton R, Gimble JM, Sousa RA, Reis RL, et al. Human adipose-derived cells can serve as a single-cell source for the in vitro cultivation of vascularized bone grafts. J Tissue Eng Regen Med. 2012;8(8):629–39.View ArticleGoogle Scholar
  9. Huang GT, Gronthos S, Shi S. Mesenchymal stem cells derived from dental tissues vs. those from other sources: their biology and role in regenerative medicine. J Dent Res. 2009;88(9):792–806.View ArticleGoogle Scholar
  10. He P, Sahoo S, Ng KS, Chen K, Toh SL, Goh JC. Enhanced osteoinductivity and osteoconductivity through hydroxyapatite coating of silk-based tissue-engineered ligament scaffold. J Biomed Mater Res A. 2013;101(2):555–66.View ArticleGoogle Scholar
  11. Kim BC, Bae H, Kwon IK, Lee EJ, Park JH, Khademhosseini A, et al. Osteoblastic/cementoblastic and neural differentiation of dental stem cells and their applications to tissue engineering and regenerative medicine. Tissue Eng Part B Rev. 2012;18(3):235–44.View ArticleGoogle Scholar
  12. Laino G, d'Aquino R, Graziano A, Lanza V, Carinci F, Naro F, et al. A new population of human adult dental pulp stem cells: a useful source of living autologous fibrous bone tissue (LAB). J Bone Miner Res. 2005;20(8):1394–402.View ArticleGoogle Scholar
  13. Yang X, Walboomers XF, van den Beucken JJ, Bian Z, Fan M, Jansen JA. Hard tissue formation of STRO-1-selected rat dental pulp stem cells in vivo. Tissue Eng Part A. 2009;15(2):367–75.View ArticleGoogle Scholar
  14. Graziano A, d'Aquino R, Laino G, Papaccio G. Dental pulp stem cells: a promising tool for bone regeneration. Stem Cell Rev. 2008;4(1):21–6.View ArticleGoogle Scholar
  15. d'Aquino R, De Rosa A, Lanza V, Tirino V, Laino L, Graziano A, et al. Human mandible bone defect repair by the grafting of dental pulp stem/progenitor cells and collagen sponge biocomplexes. Eur Cell Mater. 2009;18:75–83.Google Scholar
  16. El-Backly RM, Massoud AG, El-Badry AM, Sherif RA, Marei MK. Regeneration of dentine/pulp-like tissue using a dental pulp stem cell/poly(lactic-co-glycolic) acid scaffold construct in New Zealand white rabbits. Aust Endod J. 2008;34(2):52–67.View ArticleGoogle Scholar
  17. Seo BM, Miura M, Gronthos S, Bartold PM, Batouli S, Brahim J, et al. Investigation of multipotent postnatal stem cells from human periodontal ligament. Lancet. 2004;364(9429):149–55.View ArticleGoogle Scholar
  18. Gay IC, Chen S, MacDougall M. Isolation and characterization of multipotent human periodontal ligament stem cells. Orthod Craniofac Res. 2007;10(3):149–60.View ArticleGoogle Scholar
  19. Yang ZH, Zhang XJ, Dang NN, Ma ZF, Xu L, Wu JJ, et al. Apical tooth germ cell-conditioned medium enhances the differentiation of periodontal ligament stem cells into cementum/periodontal ligament-like tissues. J Periodontal Res. 2009;44(2):199–210.View ArticleGoogle Scholar
  20. Ge S, Zhao N, Wang L, Yu M, Liu H, Song A, et al. Bone repair by periodontal ligament stem cellseeded nanohydroxyapatite-chitosan scaffold. Int J Nanomedicine. 2012;7:5405–14.View ArticleGoogle Scholar
  21. Tour G, Wendel M, Moll G, Tcacencu I. Bone repair using periodontal ligament progenitor cell-seeded constructs. J Dent Res. 2012;91(8):789–94.View ArticleGoogle Scholar
  22. Sohn JY, Park JC, Um YJ, Jung UW, Kim CS, Cho KS, et al. Spontaneous healing capacity of rabbit cranial defects of various sizes. J Periodontal Implant Sci. 2010;40(4):180–7.View ArticleGoogle Scholar
  23. Parry PV, Engh JA. High strength silk protein scaffolds: the future of spinal fusions. Neurosurgery. 2012;71(2):N29–30.View ArticleGoogle Scholar
  24. Qian J, Suo A, Jin X, Xu W, Xu M. Preparation and in vitro characterization of biomorphic silk fibroin scaffolds for bone tissue engineering. J Biomed Mater Res A. 2013;102(9):2961–71.View ArticleGoogle Scholar
  25. Teuschl AH, van Griensven M, Redl H. Sericin removal from raw Bombyx mori silk scaffolds of high hierarchical order. Tissue Eng Part C Methods. 2013;20(5):431–9.View ArticleGoogle Scholar
  26. Cao Y, Wang B. Biodegradation of silk biomaterials. Int J Mol Sci. 2009;10(4):1514–24.View ArticleGoogle Scholar
  27. Kirker-Head C, Karageorgiou V, Hofmann S, Fajardo R, Betz O, Merkle HP, et al. BMP-silk composite matrices heal critically sized femoral defects. Bone. 2007;41(2):247–55.View ArticleGoogle Scholar
  28. Gisep A, Wieling R, Bohner M, Matter S, Schneider E, Rahn B. Resorption patterns of calcium-phosphate cements in bone. J Biomed Mater Res A. 2003;66(3):532–40.View ArticleGoogle Scholar
  29. Minoura N, Tsukada M, Nagura M. Physico-chemical properties of silk fibroin membrane as a biomaterial. Biomaterials. 1990;11(6):430–4.View ArticleGoogle Scholar
  30. Wang Y, Rudym DD, Walsh A, Abrahamsen L, Kim HJ, Kim HS, et al. In vivo degradation of three-dimensional silk fibroin scaffolds. Biomaterials. 2008;29(24–25):3415–28.View ArticleGoogle Scholar
  31. Kim JY, Choi JY, Jeong JH, Jang ES, Kim AS, Kim SG, et al. Low molecular weight silk fibroin increases alkaline phosphatase and type I collagen expression in MG63 cells. BMB Rep. 2010;43(1):52–6.View ArticleGoogle Scholar
  32. Wang J, Wei Y, Yi H, Liu Z, Sun D, Zhao H. Cytocompatibility of a silk fibroin tubular scaffold. Mater Sci Eng C Mater Biol Appl. 2014;34:429–36.View ArticleGoogle Scholar
  33. Liu TL, Miao JC, Sheng WH, Xie YF, Huang Q, Shan YB, et al. Cytocompatibility of regenerated silk fibroin film: a medical biomaterial applicable to wound healing. J Zhejiang Univ Sci B. 2010;11(1):10–6.View ArticleGoogle Scholar
  34. Pascu EI, Stokes J, McGuinness GB. Electrospun composites of PHBV, silk fibroin and nano-hydroxyapatite for bone tissue engineering. Mater Sci Eng C Mater Biol Appl. 2013;33(8):4905–16.View ArticleGoogle Scholar
  35. Webster TJ, Siegel RW, Bizios R. Osteoblast adhesion on nanophase ceramics. Biomaterials. 1999;20(13):1221–7.View ArticleGoogle Scholar
  36. Wei K, Li Y, Kim KO, Nakagawa Y, Kim BS, Abe K, et al. Fabrication of nano-hydroxyapatite on electrospun silk fibroin nanofiber and their effects in osteoblastic behavior. J Biomed Mater Res A. 2011;97(3):272–80.View ArticleGoogle Scholar
  37. Riccio M, Maraldi T, Pisciotta A, La Sala GB, Ferrari A, Bruzzesi G, et al. Fibroin scaffold repairs critical-size bone defects in vivo supported by human amniotic fluid and dental pulp stem cells. Tissue Eng Part A. 2012;18(9–10):1006–13.View ArticleGoogle Scholar
  38. Gronthos S, Arthur A, Bartold PM, Shi S. A method to isolate and culture expand human dental pulp stem cells. Methods Mol Biol. 2011;698:107–21.View ArticleGoogle Scholar
  39. Grinnemo KH, Mansson A, Dellgren G, Klingberg D, Wardell E, Drvota V, et al. Xenoreactivity and engraftment of human mesenchymal stem cells transplanted into infarcted rat myocardium. J Thorac Cardiovasc Surg. 2004;127(5):1293–300.View ArticleGoogle Scholar
  40. Pierdomenico L, Bonsi L, Calvitti M, Rondelli D, Arpinati M, Chirumbolo G, et al. Multipotent mesenchymal stem cells with immunosuppressive activity can be easily isolated from dental pulp. Transplantation. 2005;80(6):836–42.View ArticleGoogle Scholar

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© Park et al.; licensee BioMed Central. 2015

This is an Open Access article distributed under the terms of the Creative Commons Attribution License (http://creativecommons.org/licenses/by/4.0), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly credited. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated.

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