BioMed Research International

BioMed Research International / 2014 / Article

Research Article | Open Access

Volume 2014 |Article ID 672409 | 12 pages |

Collagen-Glycosaminoglycan Matrix Implantation Promotes Angiogenesis following Surgical Brain Trauma

Academic Editor: Kuo-Sheng Hung
Received15 Jun 2014
Accepted25 Jul 2014
Published17 Sep 2014


Surgical brain injury (SBI) is unavoidable during many neurosurgical procedures intrinsically linked to postoperative neurological deficits. We have previously demonstrated that implantation of collagen glycosaminoglycan (CG) following surgical brain injury could significantly promote functional recovery and neurogenesis. In this study we further hypothesized that this scaffold may provide a microenvironment by promoting angiogenesis to favor neurogenesis and subsequent functional recovery. Using the rodent model of surgical brain injury as we previously established, we divided Sprague-Dawley male rats (weighting 300–350 g) into three groups: (1) sham (2) surgical injury with a lesion (L), and (3) L with CG matrix implantation (L + CG). Our results demonstrated that L + CG group showed a statistically significant increase in the density of vascular endothelial cells and blood vessels over time. In addition, tissue concentrations of angiogenic growth factors (such as VEGF, FGF2, and PDGF) significantly increased in L + CG group. These results suggest that implantation of a CG scaffold can promote vascularization accompanied by neurogenesis. This opens prospects for use of CG scaffolds in conditions such as brain injury including trauma and ischemia.

1. Introduction

A criterion for tissue engineering scaffold to replace or restore the function of damaged tissues after surgical trauma is to mimic the complexity and microarchitecture of biological tissues, particularly the formation of functional vascular structures [1]. Our previous study suggests that applying collagen-glycosaminoglycan (CG) scaffolds not only provides a physical support structure but also promotes functional recovery and neurogenesis after surgical brain injury [2].

Promoting both angiogenesis, the formation of new capillaries from preexisting blood vessels, and neurogenesis, the formation of new nerve tissues, is therefore crucial when developing a specific cerebral microenvironment. Subsequent neuronal regeneration depends on a combination of angiogenesis and neurogenesis, which means that any microenvironment for developing the vasculature must also be accompanied by the proliferation and differentiation of neural precursor cells [3].

It is known that vascularization is of critical importance to tissue engineering, and, without it, the development of clinically applicable replacement tissue is extremely limited. Angiogenesis is the primary mechanism for vascularization of engineered biomaterials [4]. Neurogenesis and angiogenesis may play important roles in mediating functional recovery following experimental traumatic brain injury [5].

The aim of this work was to evaluate the potential of CG scaffolds as a biodegradable platform for coupling neurogenesis and angiogenesis and to further understand the role played by collagen-GAG and how its cellular and molecular microenvironments influence angiogenesis. This report describes the potential of collagen-GAG for use in promoting angiogenesis accompanying neurogenesis following surgical brain trauma.

2. Materials and Methods

2.1. CG Preparation and Assessment

We produced a biodegradable collagen matrix of 1% collagen/0.02% GAG copolymer as previously described with modifications [68]. In brief, type I CG was prepared as a weak acidic aqueous solution and was stirred at high speed to form a slurry-like composition. After lyophilization, it was cross-linked via thermal dehydration in a vacuum, followed by exposure to UV light [9]. The C-GAG copolymer matrix scaffold was cut into blocks of 6 × 4 × 3 mm (72 mm3) before implantation, and we designated an optimal degradation time of around 28 days, in step with the time course of endogenous neural stem cell (NSC) proliferation and differentiation [10]. We also coated selected sections of dehydrated CG with 5 nm of gold in an Emitech K550 sputter-coater and examined the microstructures under a scanning electron microscope (S-360, Cambridge Instruments, Cambridge, UK) (Figures 1(a) and 1(b)). The biomaterial characteristics of the CG were then assessed by the strain-pressure interaction (Figure 1(b)). We measured the change in height of a CG following gradual application of an external force. A change in matrix height/original matrix height was defined as the strain [11]. When the CG was compressed by external pressure, its height was gradually reduced. During application of the increased external force on the matrix, the strain gradually increased (Figure 1(b)) [12].

2.2. Animal Model of Surgically Induced Traumatic Brain Injury and Designation of the Experimental Groups

All of the procedures involving animals followed the Guiding Principles in the Care and Use of Animals of the American Physiology Society and were approved by the Animal Care and Use Committee of Taipei Tzu Chi Hospital, Buddhist Tzu Chi Medical Foundation. Adult male Sprague-Dawley rats weighing 300~350 g were anesthetized by an intraperitoneal injection of pentobarbital (65 mg/kg) and placed in a prone position in a stereotaxic apparatus. Surgery was performed under sterile conditions. Animals were placed into one of the following groups. (1) Animals in the sham (SHAM) group received only a craniotomy and replacement of the bone flap. (2) In the lesion (L) group, after a craniotomy and exposure of a square window displaying the underlying right frontal lobe of the brain covered by the dura, the dura was carefully incised with a number 20 needle to minimize bleeding, and a frontal parietal lesion (6 × 4 mm edge) was localized from 1.0 mm anterior to 4.0 mm posterior of the bregma and 1.0 to 5.0 mm lateral to the midline. The depth of the lesion was 3.0 mm from the brain surface. (3) In the lesion + CGM (L + CGM) group, after the procedure for the L groups was carried out, a block of CGM scaffold was placed into the lesion cavity formed following tissue removal from the frontal parietal area (Figure 2(a)). The number in each group was 10 (). All procedures used sterile gauze pads and saline irrigation to control bleeding, and the skin was sutured using 3-0 silk (Ethicon, Taiwan, Taipei). We monitored vital signs throughout the procedures.

2.3. In Vivo Magnetic Resonance Imaging (MRI) Protocol

After implantation of the CG scaffold, a clinical 1.5-T MRI system was used to observe the morphology of the CG scaffold in vivo. Under gas anesthesia with 2% isoflurane, a mouse was placed in a homemade resonance coil with an inner diameter of 3.7 cm. Fast spin echo pulse sequences provided by the vendor were used (TR/TE of 4000/101.4 ms). The slice thickness was 0.8 mm with a 0.2 mm gap, and the field of view (FOV) was 5 × 2.5 cm. The total scan time was 3 min and 20 s at an NEX of 8. Images were then analyzed at a workstation provided by GE Healthcare [12]. We verified the exact location of the graft in living animals by MRI. On a T2-weighted image, the shape of the graft in the left frontal cortex was observed to be preserved as a hypodense rectangular area, which was the best direct evidence of successful implantation of the scaffold (Figure 2(b)).

2.4. Tissue Preparation for Histology

Rats were anesthetized and perfused transcardially with phosphate buffered saline (PBS) followed by 4% paraformaldehyde on D7, D14, D21, and D28. Brains were removed then fixed in 4% paraformaldehyde overnight and embedded in paraffin blocks. Serial sections (6 μm) through the cerebral cortex were processed for double immunofluorescence staining.

2.5. Double Immunofluorescence Staining

For antigen retrieval, brain sections were treated with 50% formamide, 280 mmol/L NaCl, and 30 mmol/L sodium citrate at 65°C for 2 hours, incubated in 2 mol/L HCl at 37°C for 30 minutes, and rinsed in 0.1 mol/L boric acid (pH 8.5) at room temperature for 10 minutes. Sections were blocked in PBS containing 1% goat serum, 0.3% triton X-100 for 1 hour and followed by incubation with primary antibodies, either (1) a mouse monoclonal anti-NeuN antibody (Millipore; 1 : 1000, Temecula, CA) and a rabbit polyclonal anti-Ki-67 antibody (AnaSpec; 1 : 500, San Jose, CA), (2) a mouse monoclonal anti-α smooth muscle actin (SMA) antibody (Sigma; 1 : 500, St. Louis, MO) and a rabbit polyclonal anti-RECAM-1(CD31) antibody (Millipore; 1 : 500), (3) a mouse monoclonal anti-α-SMA antibody (Sigma; 1 : 500) and a rabbit polyclonal anti-Ki67 antibody (AnaSpec; 1 : 500), or (4) a rabbit polyclonal anti-RECAM-1(CD31) antibody (Millipore; 1 : 500) and a mouse monoclonal anti-endothelial cell (RECA-1) antibody (Abcam; 1 : 50, Cambridge, UK) at 4°C overnight and with secondary antibodies (Alexa Fluor, 488 goat anti-mouse immunoglobulin G (IgG; 1 : 200, Invitrogen, Carlsbad, CA) and DyLight 549 anti-rabbit IgG (1 : 200 dilution, Jackson ImmunoResearch, West Grove, PA)) at room temperature for 2 h. Sections were mounted with mounting medium H-1000 (Vector Laboratories, Burlingame, CA). Nonspecific staining was visualized by omitting the primary antibody and was negative. Fluorescent microscopic images were obtained with a Nikon ellipse 80i microscope (Nikon Optical, Tokyo, Japan) and a Nikon Digital Sight DS-5 M camera using NIS-Elements F 2.30 software (Nikon). Digital image processing was performed with Image-pro Plus, version 5.1.

2.6. Cell Counting

Following double immunofluorescence staining, numbers of positively stained cells in the intramatrix zone (IMZ) and lesion boundary zone (LBZ) on day 7 (D7), D14, D21, and D28 were counted manually in three to five different fields per section of each rat brain (using an eyepiece grid covering an area of 0.0625 mm2) by an individual who was blinded to the experimental design. Vessels and blood cells were excluded. Sections were observed, and images were acquired using a Nikon epifluorescent microscope. Total cells in the IMZ and LBZ were visualized by DAPI staining at 20x magnification using Openlab software (Improvision, Cambridge, MA). Ki67+ cells were visualized as fluorescent red (DL 549), and NeuN+ cells were visualized as fluorescent green (Alexa 488) in the IMZ and LBZ at 20x, while double-positive cells were visualized as yellow. For double immunofluorescence staining, double-positive cells were also manually counted in the same manner. Finally, we present the results as the number of immunopositive cells per field.

2.7. Enzyme-Linked Immunosorbent Assay (ELISA) for Measurement of the Tissue Concentrations of Platelet-Derived Growth Factor (PDGF), Fibroblast Growth Factor-2(FGF2), and Vascular Endothelial Growth Factor (VEGF)

Brains from the sham, L, and L + CG groups of animals were removed after cervical dislocation on D7, D14, D21, and D28 after surgery. A 3 mm coronal section was taken from the injured area over the parietal cortex, snap-frozen in liquid nitrogen, and stored at −70°C until used. All brain samples were homogenized in buffer consisting of 0.05 M Tris HCl, 0.15 M NaCl, 0.1% Nonidet 40, 0.5 M phenylmethylsulfonyl fluoride, 50 mg/mL aprotinin, 10 mg/mL leupeptin, 50 mg/mL pepstatin, 4 mM sodium orthovanadate, 10 mM sodium fluoride, and 10 mM sodium pyrophosphate. Homogenates were centrifuged at 4°C and 12,000 g for 15 min. Then the supernatants were removed and assayed in duplicate using VEGF and PDGF assay kits (R&D Systems, Minneapolis, MN) and a FGF2 assay kit (MyBioSource, CA) according to the manufacturer’s guidelines. Concentrations of tissue proteins (VEGF, PDGF, and FGF2) were expressed as picograms of antigen per milligram of protein. In our experiments, the concentration of VEGF from tissue samples was measured on D7, D14, D21, and D28 with an ELISA kit.

2.8. Statistical Analysis

Comparisons between multiple groups were conducted using a one-way analysis of variance (ANOVA) with the post hoc Bonferonni -test for multiple comparison. All statistical analyses were performed using Sigma Stat version 2.0 from Jandel Scientific (San Diego, CA). Data are expressed as the mean ± standard deviation (SD). Differences were considered significant as , , and for L or L + CG groups versus the sham group; +, ++, and +++ for L + CG versus L.

3. Results

3.1. Increased Proliferating Neurons Cells within the Lesion Boundary Zone (LBZ) in the L + CG Group

Representative photomicrographs show double immunofluorescence staining with antibodies against Ki-67 (red, a cellular marker of proliferation), and NeuN (green, a neuronal marker) of brain sections from L + CG rats on D14 following injury. Further, we counted the density (cells/mm2) of NeuN+/Ki67+ cells in the LBZ of the sham, L, and L + CG groups of rats at various time points. The L + CG group also showed a significant increase in NeuN+/Ki67+ cells on D7 after the surgical brain lesion, with levels sustained and peaking with a slight increase on D28. CG implantation promoted proliferation of neurons as defined by NeuN+/Ki67+ immunoreactivity in the LBZ of surgical brain lesions after implantation. See Figure 3.

3.2. Increased Proliferating Smooth Muscle Cells in Vessel Walls in the LBZ of the L + CG Group

α-SMA is commonly used as a marker of myofibroblast formation [13]. To identify if the existence of proliferative smooth muscle cells was correlated with angiogenesis, we examined the density of α-SMA+/Ki67+ cells within the LBZ. Double immunofluorescent staining of α-SMA+/Ki67+ cells identified double-positive cells (proliferative smooth muscle cells) in the IMZ and LBZ (Figure 4). We also measured the density (cells/mm2) of α-SMA+/Ki67+ cells in the LBZ of the sham, L, and L + CG groups of rats at various time points. The L + CG group also showed a significant increase in α-SMA+/Ki67+ cells on D7 after the surgical brain lesion, with levels sustained and peaking with a slight increase on D28. We also found some α-SMA+/Ki67+ cells existed in the IMZ of the L + CG group.

3.3. Increased Endothelial Cells and Smooth Muscle Cells in the IMZ and LBZ with Implantation of CG Scaffolds

To evaluate angiogenesis, we used CD31 which is mainly used immunohistochemically to define the presence of endothelial cells [14]. The earliest marker common to both endothelial and hematopoietic precursors so far identified is CD31 [15]. We verified that lumens with simultaneous CD31 and α-SMA staining were arterioles. Isolated cells that stained positive for α-SMA with or without elongating transformation were regarded as myofibroblasts [11]. We also examined whether CD31+/α-SMA+ cells existed in the IMZ and LBZ of surgical traumatic brain lesions after implantation of the CG scaffold. Double immunofluorescent staining of CD31+/α-SMA+ cells allowed recognition of double-positive cells (both endothelial cells and smooth muscle cells in vessel walls) in the IMZ of surgical traumatic brain lesions with implantation of the CG (Figure 5). We also measured the density (cell/mm2) of CD+ cells and CD31+/α-SMA+ cells in the LBZ of the sham, L, and L + CG groups of animals at various time points. The L + CG group also showed significant increases in both CD31+ cells and CD31+/α-SMA+ cells in the LBZ on D7 with a sustained increase up to D28 (Figures 5(d) and 5(e)).

3.4. Increased Proliferative Endothelial Cells in the LBZ after CG Implantation

To further identify proliferative endothelial cells in the LBZ, we instituted double immunofluorescent staining of RECA-1+/Ki67+ cells to confirm whether angiogenesis existed. RECA-1 is a well-known endothelial cell antibody in rat studies and is especially used to further identify the character and function of endothelial cell-specific antigens [16]. Double immunofluorescent staining of RECA-1+/Ki67+ cells identified double-positive cells (proliferative endothelial cells) in the IMZ and LBZ (Figure 6). We further measured the density (cells/mm2) of RECA-1+/Ki67+ cells in the LBZ of the sham, L, and L + CGM groups of rats at different time points. The L + CG group also showed a significant increase in RECA-1+/Ki67+ cells on D7 after the surgical brain lesion, although significant increases in RECA-1+ cells, both RECA-1+ and RECA-1+/Ki67+ cells, were shown with sustained increases in levels.

3.5. Increased Tissue Concentrations of FGF2, PDGF, and VEGF

We further measured tissue concentrations of FGF2, PDGF, and VEGF in the LBZ of the sham, L, and L + CG group rats on D7, D14, D21, and D28 after the surgical brain lesion. The L + CG group showed significant increases (all ) in tissue concentrations of FGF2, PDGF, and VEGF as early as D7 (F(2, 12) = 72.84, 107.63, 386.78, resp.); and all exhibited peak levels on D21 (F(2, 12) = 476.94, 818.76, 1127.37, resp.) and sustained to D28 (F(2, 12) = 185.63, 672.47, 333.75, resp.). In addition to significant increases compared to sham group (all ), post hoc analysis (Bonferroni multiple comparison) also indicated significant increases (all ) in tissue concentrations of FGF2, PDGF, and VEGF in L + CG group compared to L group at D7, D14, D21, and D28 (Figure 7).

4. Discussion

In the present study we have demonstrated promotion of angiogenesis accompanied by neurogenesis after CG implantation in a rat surgical brain lesion model. We have also demonstrated histological findings of proliferative neurons in the LBZ of the L + CG group and proliferating smooth muscle cells (SMA+/Ki67+) in vessel walls in the LBZ of the L + CG group. We found an increase in endothelial cells (CD31+) after implantation of the CG scaffold following surgical brain trauma, and proliferative endothelial cells (CD31+/Ki67+) also significantly increased. Tissue concentrations of VEGF, FGF2, and PDGF also increased after CG scaffold implantation.

One essential reason for the lack of clinical success in forming viable vascular systems seems to be the complexity of the process of angiogenesis. Formation of new capillary vessels is initiated by certain growth factors. Degradation of the extracellular matrix (ECM) and surrounding parent capillary basement membrane can subsequently release proteinase enzymes, which leads to liberation of ECM-bound growth factors such as VEGF [17]. Our CG scaffold is an analog of the ECM and was previously found to have many applications in the biomedical domain due to its low antigenicity, suitable biodegradability, and good mechanical, hemostatic, and cell-binding features [18, 19]. It is also known that GAG promotes the binding and modulation of growth factors and cytokines and the inhibition of proteases and is involved in the adhesion, migration, proliferation, and differentiation of cells [2022]. Furthermore, GAG is practically nonimmunogenic. In addition to collagen purity and matrix morphology, the chemical methods used for collagen crosslinking and attachment of GAG are essential characteristics; they also influence cellular reactions [23, 24]. In tissue engineering, vascularization of implanted scaffolds is often inadequate, and this seriously obstructs the survival of cells, which perish due to a lack of oxygen and nutrients, and insufficient removal of waste products. Consequently several approaches have been employed to increase the vascularization of engineered tissue constructs. For example, pore sizes of scaffolds were varied to find the optimal diameter for cellular adhesion and migration [25]. Furthermore, some reports included endothelial cells and fibroblasts in CG scaffolds so as to initiate angiogenesis in vitro [26]. Besides, some reports also proved that the addition of GAG and growth factors could increase angiogenesis in vivo [27]. The main concerns in our study were the degradation timing and pore size. We designed a degradation time of about 28 days and found that some growth factors related to vascularization simultaneously increased. Accompanied by increases in permeability and degradation of the surrounding matrix, activated and proliferating endothelial cells were found to migrate and differentiate. In this study, our CG scaffolds also seemed to play a critical role in promoting proliferation of periendothelial cells especially in the area surrounding the lesion.

Our previous report also showed that neurological functional recovery significantly improved following implantation of a CG after surgical brain trauma [2]. It was also reported that neurogenesis and angiogenesis are coupled processes. Neurogenesis is known to be controlled by some intrinsic genetic mechanisms, and the crucial process of migrating NPCs is strongly related to the proliferation of blood vessels, signifying that blood vessels must play an essential role as a scaffold for NPC migration toward the damaged brain region [28, 29].

It is known that many trophic factors have played roles of neuroprotection following neuronal injury. BDNF was known to play important neuroprotective roles through BDNF-TrkB signaling [30] and have beneficial effects of cell survival and synaptic plasticity [31]. Our previous study has shown that CG matrix implantation increased tissue concentration of BDNF following surgical brain trauma [2]. Other previous studies also show that transplantation of BDNF-hypersecreting human mesenchymal cells can improve functional outcome following acute spinal cord injuries [32].

Besides BDNF, VEGF which was originally known to be a specific angiogenic factor is now known to have significantly beneficial effect on neurogenesis after TBI [33]. Another report also shows that VEGF itself have direct neuroprotective effects on neurons [34]. However, the potential neuroprotective effect of VEGF on cortical neurons after mechanical trauma injury has not been clearly established. In addition, PDGF is known to be both angiogenic and neuronal survival factor which is also reported to be an important component of neurovascular crosstalk [35]. FGF2 is also known to be closely involved in neuronal protection and repair after ischemic, metabolic, or traumatic brain injury [36]. In the present study we observed significant increase of FGF2, PDGF, and VEGF in L + CG group. However, which trophic factor is mainly responsible and the detailed molecular mechanisms still need further investigation.

Angiogenesis is a multifactorial process regulated by many factors, and it is also known that the recruitment of periendothelial cells is mediated by many local growth factors. An important stimulating factor in angiogenesis is VEGF. The presence of VEGF allows endothelial cells to proliferate and migrate in the direction of the scaffold, where they begin proliferating and differentiating. FGF2 is also known for its angiogenic potential which stimulates endothelial cells to produce VEGF and increases VEGF receptor expression. FGF2 also stimulates endothelial cell migration, pericyte attraction, and matrix deposition [37]. Additionally, it was reported that PDGF is regarded as a chemoattractant for smooth muscle cells (which comprise the vessel walls of arterioles), while VEGF, possibly via release of PDGF or binding to VEGF receptors, also contributes to this effect [38]. Angiogenesis processes are regulated by various growth factors, and VEGF is the most potent in promoting the formation of new blood vessels [39, 40]. The need for multiple growth factors was investigated by Laschke et al. [41], who found that angiogenesis and blood vessel maturation can be suppressed by complete inhibition of either VEGF, FGF2, or PDGF. It is also known that VEGF contributes to the complexity of the vascular network by stimulating vascular splitting and sprouting [42]. We demonstrated that angiogenesis increases with increasing tissue concentrations of these growth factors. Our results emphasized that increased tissue concentrations of growth factors (VEGF, FGF2, and PDGF) may promote angiogenesis and result in a higher density of blood vessels [43]. It is recognized that growth factors contribute to tissue regeneration at various stages of cell proliferation and differentiation [44]. VEGF and PDGF modulate the glial response to a cortical injury [45]. Endogenous VEGF expression induces glia cell proliferation by autocrine signaling in the brain after injury [46]. VEGF also acts as a proinflammatory cytokine [47] and promotes migration and proliferation of microglia in vitro [48]. PDGF is also expressed in microglia [49] and interacts with the ionized calcium binding adaptor molecule 1 to enhance microglia motility and activation [50]. Increased calcium may also be a potential mechanism underlying the effects of angiogenesis following implantation of CG matrix after surgical brain injury. It has been demonstrated that Orai1 is upregulated in vascular smooth muscle cells (VSMC) during vascular injury and is required for nuclear factor for activated T-cell (NFAT) activity, VSMC proliferation, and neointima formation [51]. In addition, cell proliferation and cell inflammation can be regulated by calcium signaling in different types of cells [5254]. Therefore, increased calcium might also play an important role in the enhanced angiogenesis in L + CG group.

5. Conclusions

Our results indicate that implantation of CG scaffolds leads to a well-developed vasculature. This study verifies the angiogenic effect of a CG used on a surgical brain trauma defect. This opens new opportunities for the clinical use of C-GAG scaffolds for tissue regeneration following brain injuries such as ischemia or trauma.

Conflict of Interests

The authors declare that there is no conflict of interests regarding the publication of this paper.


This study was financially supported in part by Grants from the Ministry of Science and Technology (MOST 103-2321-B-038-002 to JY Wang) and from the Taipei Tzu Chi Hospital, Buddhist Tzu Chi Medical Foundation (TCRD-TPE-101-50 to KF Huang), Taipei, Taiwan, without conflict of interests. The authors would like to thank Life Spring Biotech, Horien Biochemical Technology, and the Core Lab, Taipei Tzu-Chi Hospital, Buddhist Tzu Chi Medical Foundation, for laboratory and technical support of this study.


  1. S. Baiguera and D. Ribatti, “Endothelialization approaches for viable engineered tissues,” Angiogenesis, vol. 16, no. 1, pp. 1–14, 2013. View at: Publisher Site | Google Scholar
  2. K.-F. Huang, W.-C. Hsu, W.-T. Chiu, and J.-Y. Wang, “Functional improvement and neurogenesis after collagen-GAG matrix implantation into surgical brain trauma,” Biomaterials, vol. 33, no. 7, pp. 2067–2075, 2012. View at: Publisher Site | Google Scholar
  3. X.-T. Yang, Y.-Y. Bi, and D.-F. Feng, “From the vascular microenvironment to neurogenesis,” Brain Research Bulletin, vol. 84, no. 1, pp. 1–7, 2011. View at: Publisher Site | Google Scholar
  4. Y. Xiong, A. Mahmood, and M. Chopp, “Angiogenesis, neurogenesis and brain recovery of function following injury,” Current Opinion in Investigational Drugs, vol. 11, no. 3, pp. 298–308, 2010. View at: Google Scholar
  5. H. Wu, D. Lu, H. Jiang et al., “Simvastatin-mediated upregulation of VEGF and BDNF, activation of the PI3K/Akt pathway, and increase of neurogenesis are associated with therapeutic improvement after traumatic brain injury,” Journal of Neurotrauma, vol. 25, no. 2, pp. 130–139, 2008. View at: Publisher Site | Google Scholar
  6. B. A. C. Harley, H.-D. Kim, M. H. Zaman, I. V. Yannas, D. A. Lauffenburger, and L. J. Gibson, “Microarchitecture of three-dimensional scaffolds influences cell migration behavior via junction interactions,” Biophysical Journal, vol. 95, no. 8, pp. 4013–4024, 2008. View at: Publisher Site | Google Scholar
  7. W.-C. Hsu, M. H. Spilker, I. V. Yannas, and P. A. D. Rubin, “Inhibition of conjunctival scarring and contraction by a porous collagen-glycosaminoglycan implant,” Investigative Ophthalmology and Visual Science, vol. 41, no. 9, pp. 2404–2411, 2000. View at: Google Scholar
  8. I. V. Yannas, E. Lee, D. P. Orgill, E. M. Skrabut, and G. F. Murphy, “Synthesis and characterization of a model extracellular matrix that induces partial regeneration of adult mammalian skin,” Proceedings of the National Academy of Sciences of the United States of America, vol. 86, no. 3, pp. 933–937, 1989. View at: Google Scholar
  9. W.-C. Wu, C.-C. Lai, H. S.-L. Chen et al., “Efficacy and safety of biodegradable collagen-glycosaminoglycan polymer as a material for scleral buckling,” Investigative Ophthalmology and Visual Science, vol. 49, no. 6, pp. 2673–2678, 2008. View at: Publisher Site | Google Scholar
  10. S. G. Kernie and J. M. Parent, “Forebrain neurogenesis after focal Ischemic and traumatic brain injury,” Neurobiology of Disease, vol. 37, no. 2, pp. 267–274, 2010. View at: Publisher Site | Google Scholar
  11. Y.-J. Peng, C.-Y. Pan, Y.-T. Hsieh, S. Wu, H.-N. Chu, and W.-C. Hsu, “The application of tissue engineering in reversing mitomycin C-induced ischemic conjunctiva,” Journal of Biomedical Materials Research A, vol. 100, no. 5, pp. 1126–1135, 2012. View at: Publisher Site | Google Scholar
  12. W.-C. Hsu, R. Ritch, T. Krupin, and H. S.-L. Chen, “Tissue bioengineering for surgical bleb defects: an animal study,” Graefe's Archive for Clinical and Experimental Ophthalmology, vol. 246, no. 5, pp. 709–717, 2008. View at: Publisher Site | Google Scholar
  13. A. G. Mustafa and O. A. Al-Shboul, “Pathophysiology of traumatic brain injury,” Neurosciences, vol. 18, no. 3, pp. 222–234, 2013. View at: Google Scholar
  14. H. M. Blau and A. Banfi, “The well-tempered vessel,” Nature Medicine, vol. 7, no. 5, pp. 532–534, 2001. View at: Publisher Site | Google Scholar
  15. T. L. Creazzo, R. E. Godt, L. Leatherbury, S. J. Conway, and M. L. Kirby, “Role of cardiac neural crest cells in cardiovascular development,” Annual Review of Physiology, vol. 60, pp. 267–286, 1998. View at: Publisher Site | Google Scholar
  16. W. N. Burnette, ““Western blotting”: electrophoretic transfer of proteins from sodium dodecyl sulfate-polyacrylamide gels to unmodified nitrocellulose and radiographic detection with antibody and radioiodinated protein A,” Analytical Biochemistry, vol. 112, no. 2, pp. 195–203, 1981. View at: Google Scholar
  17. M. I. Góth, E. Hubina, S. Raptis, G. M. Nagy, and B. E. Tóth, “Physiological and pathological angiogenesis in the endocrine system,” Microscopy Research and Technique, vol. 60, no. 1, pp. 98–106, 2003. View at: Publisher Site | Google Scholar
  18. M. Chvapil, R. L. Kronenthal, and W. Van Winkle Jr., “Medical and surgical applications of collagen,” International Review of Connective Tissue Research, vol. 6, pp. 1–61, 1973. View at: Publisher Site | Google Scholar
  19. J. M. Pachence, “Collagen-based devices for soft tissue repair,” Journal of Biomedical Materials Research, vol. 33, pp. 35–40, 1996. View at: Google Scholar
  20. R. L. Jackson, S. J. Busch, and A. D. Cardin, “Glycosaminoglycans: molecular properties, protein interactions, and role in physiological processes,” Physiological Reviews, vol. 71, no. 2, pp. 481–539, 1991. View at: Google Scholar
  21. S. E. Stringer and J. T. Gallagher, “Heparan sulphate,” International Journal of Biochemistry and Cell Biology, vol. 29, no. 5, pp. 709–714, 1997. View at: Publisher Site | Google Scholar
  22. G. David, “Integral membrane heparan sulfate proteoglycans,” The FASEB Journal, vol. 7, no. 11, pp. 1023–1030, 1993. View at: Google Scholar
  23. C. J. Doillon, F. H. Silver, and R. A. Berg, “Fibroblast growth on a porous collagen sponge containing hyaluronic acid and fibronectin,” Biomaterials, vol. 8, no. 3, pp. 195–200, 1987. View at: Publisher Site | Google Scholar
  24. P. D. Kemp, J. F. Cavallaro, and D. N. Hastings, “Effects of carbodiimide crosslinking and load environment on the remodeling of collagen scaffolds,” Tissue Engineering, vol. 1, no. 1, pp. 71–79, 1995. View at: Publisher Site | Google Scholar
  25. F. J. O'Brien, B. A. Harley, I. V. Yannas, and L. J. Gibson, “The effect of pore size on cell adhesion in collagen-GAG scaffolds,” Biomaterials, vol. 26, no. 4, pp. 433–441, 2005. View at: Publisher Site | Google Scholar
  26. D. Rickert, M. A. Moses, A. Lendlein, S. Kelch, and R.-P. Franke, “The importance of angiogenesis in the interaction between polymeric biomaterials and surrounding tissue,” Clinical Hemorheology and Microcirculation, vol. 28, no. 3, pp. 175–181, 2003. View at: Google Scholar
  27. J. S. Pieper, T. Hafmans, P. B. van Wachem et al., “Loading of collagen-heparan sulfate matrices with bFGF promotes angiogenesis and tissue generation in rats,” Journal of Biomedical Materials Research, vol. 62, no. 2, pp. 185–194, 2002. View at: Publisher Site | Google Scholar
  28. H. Teng, Z. G. Zhang, L. Wang et al., “Coupling of angiogenesis and neurogenesis in cultured endothelial cells and neural progenitor cells after stroke,” Journal of Cerebral Blood Flow and Metabolism, vol. 28, no. 4, pp. 764–771, 2008. View at: Publisher Site | Google Scholar
  29. M. Angels Font, A. Arboix, and J. Krupinski, “Angiogenesis, neurogenesis and neuroplasticity in ischemic stroke,” Current Cardiology Reviews, vol. 6, no. 3, pp. 238–244, 2010. View at: Publisher Site | Google Scholar
  30. Y. Doi, H. Takeuchi, H. Horiuchi et al., “Fingolimod phosphate attenuates oligomeric amyloid beta-induced neurotoxicity via increased brain-derived neurotrophic factor expression in neurons,” PLoS ONE, vol. 8, no. 4, Article ID e61988, 2013. View at: Publisher Site | Google Scholar
  31. A. Yoshii and M. Constantine-Paton, “Postsynaptic BDNF-TrkB signaling in synapse maturation, plasticity, and disease,” Developmental Neurobiology, vol. 70, no. 5, pp. 304–322, 2010. View at: Publisher Site | Google Scholar
  32. M. Sasaki, C. Radtke, A. M. Tan et al., “BDNF-hypersecreting human mesenchymal stem cells promote functional recovery, axonal sprouting, and protection of corticospinal neurons after spinal cord injury,” The Journal of Neuroscience, vol. 29, no. 47, pp. 14932–14941, 2009. View at: Publisher Site | Google Scholar
  33. O. Thau-Zuchman, E. Shohami, A. G. Alexandrovich, and R. R. Leker, “Vascular endothelial growth factor increases neurogenesis after traumatic brain injury,” Journal of Cerebral Blood Flow and Metabolism, vol. 30, no. 5, pp. 1008–1016, 2010. View at: Publisher Site | Google Scholar
  34. L. Tolosa, M. Mir, G. Olmos, and J. Lladó, “Vascular endothelial growth factor protects motoneurons from serum deprivation-induced cell death through phosphatidylinositol 3-kinase-mediated p38 mitogen-activated protein kinase inhibition,” Neuroscience, vol. 158, no. 4, pp. 1348–1355, 2009. View at: Publisher Site | Google Scholar
  35. C. Lee, F. Zhang, Z. Tang, Y. Liu, and X. Li, “PDGF-C: a new performer in the neurovascular interplay,” Trends in Molecular Medicine, vol. 19, no. 8, pp. 474–486, 2013. View at: Publisher Site | Google Scholar
  36. C. Alzheimer and S. Werner, “Fibroblast growth factors and neuroprotection,” Advances in Experimental Medicine and Biology, vol. 513, pp. 335–351, 2002. View at: Google Scholar
  37. M. Komori, Y. Tomizawa, K. Takada, and M. Ozaki, “A single local application of recombinant human basic fibroblast growth factor accelerates initial angiogenesis during wound healing in rabbit ear chamber,” Anesthesia and Analgesia, vol. 100, no. 3, pp. 830–834, 2005. View at: Publisher Site | Google Scholar
  38. P. Lindahl, M. Hellström, M. Kalén, and C. Betsholtz, “Endothelial-perivascular cell signaling in vascular development: lessons from knockout mice,” Current Opinion in Lipidology, vol. 9, no. 5, pp. 407–411, 1998. View at: Publisher Site | Google Scholar
  39. M. Huang, S. N. Vitharana, L. J. Peek, T. Coop, and C. Berkland, “Polyelectrolyte complexes stabilize and controllably release vascular endothelial growth factor,” Biomacromolecules, vol. 8, no. 5, pp. 1607–1614, 2007. View at: Publisher Site | Google Scholar
  40. Y.-I. Chung, S.-K. Kim, Y.-K. Lee et al., “Efficient revascularization by VEGF administration via heparin-functionalized nanoparticle-fibrin complex,” Journal of Controlled Release, vol. 143, no. 3, pp. 282–289, 2010. View at: Publisher Site | Google Scholar
  41. M. W. Laschke, A. Elitzsch, B. Vollmar, P. Vajkoczy, and M. D. Menger, “Combined inhibition of vascular endothelial growth factor (VEGF), fibroblast growth factor and platelet-derived growth factor, but not inhibition of VEGF alone, effectively suppresses angiogenesis and vessel maturation in endometriotic lesions,” Human Reproduction, vol. 21, no. 1, pp. 262–268, 2006. View at: Publisher Site | Google Scholar
  42. A. Pettersson, J. A. Nagy, L. F. Brown et al., “Heterogeneity of the angiogenic response induced in different normal adult tissues by vascular permeability factor/vascular endothelial growth factor,” Laboratory Investigation, vol. 80, no. 1, pp. 99–115, 2000. View at: Publisher Site | Google Scholar
  43. T. Asahara, C. Bauters, L. P. Zheng et al., “Synergistic effect of vascular endothelial growth factor and basic fibroblast growth factor on angiogenesis in vivo,” Circulation, vol. 92, no. 9, pp. II365–II371, 1995. View at: Publisher Site | Google Scholar
  44. D. Gospodarowicz, “3 fibroblast growth factor and its involvement in developmental processes,” Current Topics in Developmental Biology, vol. 24, pp. 57–93, 1990. View at: Publisher Site | Google Scholar
  45. A. Norazit, M. N. Nguyen, C. G. M. Dickson et al., “Vascular endothelial growth factor and platelet derived growth factor modulates the glial response to a cortical stab injury,” Neuroscience, vol. 192, pp. 652–660, 2011. View at: Publisher Site | Google Scholar
  46. J. M. Krum, N. Mani, and J. M. Rosenstein, “Roles of the endogenous VEGF receptors flt-1 and flk-1 in astroglial and vascular remodeling after brain injury,” Experimental Neurology, vol. 212, no. 1, pp. 108–117, 2008. View at: Publisher Site | Google Scholar
  47. S. D. Croll, R. M. Ransohoff, N. Cai et al., “VEGF-mediated inflammation precedes angiogenesis in adult brain,” Experimental Neurology, vol. 187, no. 2, pp. 388–402, 2004. View at: Publisher Site | Google Scholar
  48. F. Forstreuter, R. Lucius, and R. Mentlein, “Vascular endothelial growth factor induces chemotaxis and proliferation of microglial cells,” Journal of Neuroimmunology, vol. 132, no. 1-2, pp. 93–98, 2002. View at: Publisher Site | Google Scholar
  49. R. S. T. J. Nicholas, M. G. Wing, and A. Compston, “Nonactivated microglia promote oligodendrocyte precursor survival and maturation through the transcription factor NF-κB,” European Journal of Neuroscience, vol. 13, no. 5, pp. 959–967, 2001. View at: Publisher Site | Google Scholar
  50. H. Kanazawa, K. Ohsawa, Y. Sasaki, S. Kohsaka, and Y. Imai, “Macrophage/microglia-specific protein Iba1 enhances membrane ruffling and Rac activation via phospholipase C-γ-dependent pathway,” The Journal of Biological Chemistry, vol. 277, no. 22, pp. 20026–20032, 2002. View at: Publisher Site | Google Scholar
  51. W. Zhang, K. E. Halligan, X. Zhang et al., “Orai1-mediated ICRAC is essential for neointima formation after vascular injury,” Circulation Research, vol. 109, no. 5, pp. 534–542, 2011. View at: Publisher Site | Google Scholar
  52. I.-H. Yang, Y.-T. Tsai, S.-J. Chiu et al., “Involvement of STIM1 and Orai1 in EGF-mediated cell growth in retinal pigment epithelial cells,” Journal of Biomedical Science, vol. 20, no. 1, article 41, 2013. View at: Publisher Site | Google Scholar
  53. J.-Y. Wang, B.-K. Chen, Y.-S. Wang et al., “Involvement of store-operated calcium signaling in EGF-mediated COX-2 gene activation in cancer cells,” Cellular Signalling, vol. 24, no. 1, pp. 162–169, 2012. View at: Publisher Site | Google Scholar
  54. M.-F. Hou, H.-C. Kuo, J.-H. Li et al., “Orai1/CRACM1 overexpression suppresses cell proliferation via attenuation of the store-operated calcium influx-mediated signalling pathway in A549 lung cancer cells,” Biochimica et Biophysica Acta—General Subjects, vol. 1810, no. 12, pp. 1278–1284, 2011. View at: Publisher Site | Google Scholar

Copyright © 2014 Kuo-Feng Huang et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

More related articles

1340 Views | 687 Downloads | 5 Citations
 PDF  Download Citation  Citation
 Download other formatsMore
 Order printed copiesOrder

Related articles

We are committed to sharing findings related to COVID-19 as quickly and safely as possible. Any author submitting a COVID-19 paper should notify us at to ensure their research is fast-tracked and made available on a preprint server as soon as possible. We will be providing unlimited waivers of publication charges for accepted articles related to COVID-19. Sign up here as a reviewer to help fast-track new submissions.