BioMed Research International

BioMed Research International / 2014 / Article
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New Biomaterials and Regenerative Medicine Strategies in Periodontology, Oral Surgery, and Esthetic and Implant Dentistry

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Research Article | Open Access

Volume 2014 |Article ID 253590 | https://doi.org/10.1155/2014/253590

Antonia Terriza, Jose I. Vilches-Pérez, Emilio de la Orden, Francisco Yubero, Juan L. Gonzalez-Caballero, Agustin R. González-Elipe, José Vilches, Mercedes Salido, "Osteoconductive Potential of Barrier NanoSiO2 PLGA Membranes Functionalized by Plasma Enhanced Chemical Vapour Deposition", BioMed Research International, vol. 2014, Article ID 253590, 10 pages, 2014. https://doi.org/10.1155/2014/253590

Osteoconductive Potential of Barrier NanoSiO2 PLGA Membranes Functionalized by Plasma Enhanced Chemical Vapour Deposition

Academic Editor: David M. Dohan Ehrenfest
Received26 Feb 2014
Accepted01 Apr 2014
Published04 May 2014

Abstract

The possibility of tailoring membrane surfaces with osteoconductive potential, in particular in biodegradable devices, to create modified biomaterials that stimulate osteoblast response should make them more suitable for clinical use, hopefully enhancing bone regeneration. Bioactive inorganic materials, such as silica, have been suggested to improve the bioactivity of synthetic biopolymers. An in vitro study on HOB human osteoblasts was performed to assess biocompatibility and bioactivity of SiO2 functionalized poly(lactide-co-glycolide) (PLGA) membranes, prior to clinical use. A 15 nm SiO2 layer was deposited by plasma enhanced chemical vapour deposition (PECVD), onto a resorbable PLGA membrane. Samples were characterized by X-ray photoelectron spectroscopy, atomic force microscopy, scanning electron microscopy, and infrared spectroscopy (FT-IR). HOB cells were seeded on sterilized test surfaces where cell morphology, spreading, actin cytoskeletal organization, and focal adhesion expression were assessed. As proved by the FT-IR analysis of samples, the deposition by PECVD of the SiO2 onto the PLGA membrane did not alter the composition and other characteristics of the organic membrane. A temporal and spatial reorganization of cytoskeleton and focal adhesions and morphological changes in response to SiO2 nanolayer were identified in our model. The novedous SiO2 deposition method is compatible with the standard sterilization protocols and reveals as a valuable tool to increase bioactivity of resorbable PLGA membranes.

1. Introduction

Cell-biomaterial interaction is a major challenge for tissue engineering, since not only the physic-mechanic-chemical features of the natural extracellular matrix must be mimicked, but also a successful cell to biomaterial adhesion should be achieved in the shortest time. Cell adhesion is critical in the first stages of the tissue engineering methodology where adhesion is the basis and the key process that allows other important cell activities such as migration and growth. In the fields of tissue engineering and guided bone regeneration (GBR), an appropriate cell culture scaffold is required to enhance cell attachment, proliferation, and differentiation in vitro, as cells interact with native or topographically and chemically tailored structures in many ways [15].

The GBR therapeutic approach is based on the concept that regeneration of osseous defects is attainable via the application of occlusive membranes, resorbable or nonresorbable, which mechanically exclude nonosteogenic cell populations from the surrounding soft tissues. Nowadays GBR is subject of growing interest due to the increasing needs for permanent, temporary, or biodegradable orthopaedic devices designed for bone repair and regeneration [611].

A variety of polymeric bioresorbable GBR membranes that permit single-step procedures, thus reducing patient discomfort and costs, and potential surgical complications are currently available. Polymeric coatings for biomedical devices are especially interesting due to the diversity of their chemical and physical properties and natural biopolymers appear promising as biomimetic coatings, as a result of their similarity to human tissues. Although these membranes are biocompatible, nontoxic, or immunogenic and permit mechanical support during bone formation, they do not actually possess bioactive properties to induce osteogenesis [6, 9, 1214].

Poly(lactide-co-glycolide) (PLGA) is among the few synthetic polymers approved for human clinical use due to its biocompatibility, controllable degradability, and relatively good processability and has been used in the design of scaffolds for bone tissue engineering and for drug delivery purposes [15, 16]. However, the polymer itself  is quite bioinert and does not elicit a significant biological response in bone cells [8, 16].

The physicochemical properties of the material at the cell-material interface are decisive for the cell-material interaction, due to its interfacial role between the material and the host tissue, and are able to trigger a wide variety of processes, from the initial inflammatory reaction to ultimate tissue remodelling [13, 17]. Although the bulk properties of materials are important for the overall properties, especially for mechanical strength, a topographical modification of the cell-substrate interface is of utmost importance. Thus, the possibility of tailoring membrane surfaces, in particular in biodegradable devices with bioactive properties, to create modified biomaterials that mimic natural bone extracellular matrix (ECM) and stimulate osteoblast response should make them more suitable for clinical use, hopefully enhancing bone regeneration in the near future [1, 2, 18].

Bioactive inorganic materials, such as silica granules, have been suggested to improve the bioactivity of synthetic biopolymers in promoting the osteogenic performance of osteoblast-like cells. It has been strongly suggested that silicon/silica is functionally active during bone formation with a close relationship between silicate and calcium deposition. Silica is a low cost and biocompatible inorganic material having excellent chemical stability with great commercial value and ideal for tailoring surface topographies [1924].

We have designed an in vitro model in order to assess normal human osteoblasts, HOB, response to a series of SiO2 functionalized PLGA membranes intended to be used as barrier membranes for bone guided regeneration.

For the synthesis of the PLGA foils we have followed classical synthesis procedures based on the solution/evaporation method [2527]. A problem encountered by the surface functionalization of these membranes by classical sol-gel or similar wet chemical routes is the degradation of the PLGA when it is exposed to liquid media or treated at relatively high temperatures [2834]. To avoid these problems, we have followed a new approach consisting of the deposition at room temperature by plasma enhanced chemical vapour deposition (PECVD) of a very thin layer of SiO2 on the surface of the PLGA membranes (SiO2/PLGA) [35], in order to achieve a strict control of the deposition conditions without inducing any damage in the PLGA that could efficiently promote the development of bone regenerating cells.

2. Material and Methods

2.1. Cell Culture

HOB human osteoblasts were incubated in Osteoblast Growing Medium with 10% foetal calf serum at 37° and 5% CO2 until the experiments were started. HOB cells did not exceed ten population doublings. Test surfaces were sterilized under ultraviolet (u.v.) light for 20 min each side, in a laminar flow chamber prior to cell seeding. HOB osteoblasts were seeded at a density of 5000 cells/cm2 on test surfaces, that is, bare PLGA or SiO2/PLGA membranes, and immunolabelled after 24, 48, and 72 hours. HOB osteoblasts, media, and sera were obtained from Promocell (Heidelberg, Germany).

2.2. PLGA Membranes

The PLGA membranes used as substrates were prepared from a 1.5 wt% PLGA dichloromethane solution by evaporation of the solvent on a teflon plate. The size of the membranes was  mm2. The thickness of the membranes was of the order of 50 microns.

2.3. Deposition and Characterization of SiO2 Thin Film Layers

SiO2 was deposited onto the PLGA membranes by PECVD in a plasma reactor with a remote configuration. The deposition system consisted of a quartz tube with a funnel shape termination attached to a stainless-steel chamber where the samples were placed. The plasma source is a surfatron (Sairem) launcher that was supplied with a microwave power of 60 W. These conditions provide a typical plasma electron density of about  cm−3. Distance from substrate to the quartz tube was 5 cm. The plasma gas and the precursor used were pure Ar (7.5 sccm) and hexamethyldisiloxane (HDMSO, 5 sccm), respectively. Synthesis of the films was carried out at room temperature, working at a pressure of 0.3 Torr. The gas flow was controlled by mass flow controllers (MKS). Both the stainless steel receptacle which contained the precursor and the dosing line were heated at 323 K to prevent any condensation in the tube walls. Before depositing SiO2, the polymeric substrate was exposed to plasma of pure argon for 2 min, a pretreatment that favours the adhesion of the oxide layer onto the polymer surface. A thin layer of SiO2 of 15 nm, determined by measuring with an adjacent quartz crystal monitor, was deposited on the polymeric substrate. These measurements were calibrated with the data obtained for thicker layer of SiO2 deposited on a silicon substrate that were cleaved and examined by scanning electron microscopy. Before the treatments, Ar or the mixture Ar + HDMSO was kept flowing for at least 30 min to ensure the purity of the plasma gas in the reactor [36]. The nonfunctionalized and SiO2 functionalized membranes will be designated as PLGA and SiO2/PLGA, respectively. The samples were characterized by X-ray photoelectron spectroscopy (XPS) to determine their surface chemical state and composition, atomic force microscopy (AFM) to ascertain their roughness, scanning electron microscopy (SEM) to assess the film microstructure, infrared spectroscopy (FT-IR) to determine the bonding structure, and water contact angle measurements to check the wetting characteristics of their surfaces. XPS spectra were recorded with a SPECS PHOIBOS-100 spectrometer working in the constant pass energy mode fixed at a value of 20 eV. The Mg Ka radiation was used as excitation source. For calibration of  the binding energy scale, a value of 284.6 eV was considered for the C1s component attributed to C–H and C–C bonds. Surface composition was estimated by calculating the area behind the , , and peaks and by correcting the obtained values with the sensitivity factors of these elements. AFM images were taken with a Cervantes AFM microscope driven with a Dulcinea control system (Nanotec, Madrid, Spain) working in tapping mode and using high frequency cantilevers. The images were processed with Nanotec WSxM software. SEM images were acquired in a Hitachi S4800 microscope. FT-IR spectra were collected in attenuated total reflectance (ATR) mode in a JASCO FT/IR6200 spectrometer, performing 64 scans with a resolution of 0.96 cm−1 and a spot size of 1 cm of diameter. Static contact angles of water were determined by the Young method in a SCA20 instrument (Data Physic Instruments, GmbH), with an estimated error of 3%.

2.4. Cell Morphology and Spreading

HOB osteoblasts seeded on test surfaces were daily examined with a DM ILLED Leica phase contrast microscope in order to evaluate cell morphology and spreading, cell alignment, and initial adhesion phase to surfaces, prior to fluorescence and CLSM examination.

2.5. Immunolabelling for Actin Cytoskeletal Organization and Focal Adhesion Expression

At the designed experimental time, cells in each group were washed with prewarmed phosphate buffered saline (PBS) and fixed with 3.7% paraformaldehyde at room temperature, permeabilized with 0.1% Triton x-100, preincubated in 1% bovine serum albumin in PBS, and then immunolabelled for actin cytoskeleton with rhodamine-phalloidin and for focal adhesion identification with monoclonal antivinculin FITC conjugate. After 20 min samples were twice PBS rinsed prior to mounting with Vectashield (Vector, CA). All chemicals were obtained from Sigma-Aldrich (St. Louis, Mo) unless noted.

2.6. Immunolabelled Cells Examination

Samples were visualized in a Leica TCS-SL confocal microscope. At least five samples were analysed for each experimental group to assess surface influence on cytoskeletal organization, focal adhesion number and development, and cell morphology. Samples were exposed to the lowest laser power that was able to produce a fluorescent signal, with a pinhole of 1 airy. Images were acquired at a resolution of 512 512, mean voxel size of 209.20 nm.

2.7. Image Analysis

To analyze the differences in focal adhesion number between different sample groups, images were collected and processed. Area, perimeter, roundness, circularity, solidity, and axial ratio were analysed as shape variables. Sample images were collected as frames obtained at 40x magnification and processed using Leica imaging software and Image J software (NIH, http://rsb.info.nih.gov/ij/).

2.8. Statistical Analysis

For the variable number of contacts, we used first the nonparametric contrast Kruskal-Wallis and later a two-way ANOVA contrast with the ranges of this variable [37]. Post hoc contrasts were carried out to detect the differences among the experimental groups. For shape variables, a factor analysis was performed in order to reduce the dimension and a two-way ANOVA with the resulting factors to analyze the influence of the experimental conditions. All the analysis was performed with SPSS program.

3. Results

3.1. PLGA Membranes: Deposition and Characterization of SiO2 Thin Film Layers

The SiO2 thin films prepared by PECVD presented a homogeneous microstructure and a conformal growth on the PLGA membrane. The 15 nm film surface was rather flat as shown in AFM images (Figure 1) of PLGA and SiO2-PLGA samples. In the latter, the deposition of the SiO2 film only increased the RMS roughness from 0.32 to 0.43 nm, while surface topology slightly changed with the formation of finer grains. Even if the SiO2 thickness was rather thin (15 nm), the PLGA surface was totally covered by SiO2, as can be directly retrieved from the XPS spectra (Figure 2).

The C1s spectrum of the PLGA depicts three components at 284.6, 286.4, and 288.6 eV, attributed to C–C/C–H, C–O, and >C=O/COOH species [22, 23]. This complex spectrum transformed when the PLGA membrane was covered by SiO2, where only a C1s component at 284.6 eV, attributed to spurious carbon due to contamination, can be identified. An equivalent modification appears in the O1s spectra, with clearly different widths of PLGA and SiO2 spectra. The Si2p spectra confirms that the PLGA membrane was free from this element, while the SiO2/PLGA samples depict a well-defined Si 2p peak at 103.9 eV, attributed to Si4+ ions in SiO2 [38, 39]. It must be stressed that the deposition by PECVD of the SiO2 onto the PLGA membrane did not alter the composition and other characteristics of the organic membrane as proved by the FT-IR analysis of samples. The spectral regions reported (Figure 3) for the PLGA and SiO2-PLGA samples were very similar and are characterized by the typical shape of the spectra of this polymer. The small increase in the height of the peak at 1050 cm−1 observed for the SiO2/PLGA sample can be attributed to the contribution at this wavenumbers of the Si–O–Si stretching vibration of the silica network in the SiO2 film [36]. The other features in the spectra correspond to well-documented vibrations of PLGA polymers: 2994, 2946, 2840 (CH bend), 1753 (C=O ester), 1460, 1428, 1371 (CH3), 1185, 1080–980 (C–O stretch), and 754 (CH-bend) cm−1 [40]. No significant spectral changes are expected due to the different thickness of the PLGA membrane (50 μm) and the SiO2 films (15 nm) and the typical thickness proved by ATR analysis (a few tens of microns).

Since wetting behavior and surface tension are important parameters for cell development of cells on bioactive materials [41, 42] the water contact angle was measured for both the PLGA and SiO2/PLGA membranes and the values obtained were 99.3° and 93.8°, respectively, indicating no significant differences in wetting between these two surfaces.

During the experimental time, no clear signs of degradation were observed in the membranes, During the experimental time, no clear signs of degradation were observed in the membranes. FT-IR, AFM, and XPS analysis of the surface of the PLGA and SiO2/PLGA membranes extracted from the PBS and gentled dried in air did not reveal significant changes suggesting any significant degradation. membrane degradation (loss of physical integrity, changes in color, etc.) could only be observed after 20 weeks of immersion in liquid media, although clear signs of degradation (loss of physical integrity, changes in color, etc.) could be observed after 20 weeks of immersion in liquid media. The exposure of PLGA and SiO2/PLGA membranes to u.v. irradiation under similar conditions to those used in the sterilization protocol prior to cell seeding did not produce any detectable change.

3.2. Living Cell Examination: Cell Morphology and Spreading

Living HOB  cells examination revealed a successful cell spreading on silica treated membranes, with cell elongation and marked filopodial emission, and the establishment of clear cell contacts and attachment to the functionalized surface in the first 24 hours. Cells clustered and elongated during the next hours, and after 48 hours in culture, cell spreading evolved to a clear cell packaging, with osteoblasts well adhered to the silica treated surface and to the neighboring cells (Figures 4(b) and 4(d)). Cells grown on bare PLGA membranes spread evenly although clearly adhered to surfaces, showing some lamellipodia in the first 24 hours but without clear cell clustering after 48 hours in culture (Figures 4(a) and 4(c)).

3.3. Actin Cytoskeletal Organization and Vinculin Immunolabelling of Focal Adhesion Sites

Osteoblasts grown on the SiO2 functionalized PLGA membranes showed defined stress fibers formation, with a clear polarization of actin cytoskeleton towards strongly evident vinculin positive sites. Cell polarization was clearly determined by SiO2 functionalized surfaces, with osteoblasts showing extensive lamellipodial emission reinforced with vinculin positive focal adhesion in the leading edge and supported by a highly defined actin network. Focal adhesions appeared to be significantly more numerous and well developed in those cells grown on the SiO2 functionalized membranes HOB grown on bare PLGA randomly orientated and showed a reduced stress fibers and focal adhesion development at the same experimental time. Although some evenly distributed filopodia were observed, cells did not show a well-organized actin network or polarization, and vinculin positive sites appeared randomly distributed in the cell periphery (Figures 5, 6, and 7).

3.4. Image Analysis: Statistical Analysis of Focal Adhesion Behaviour

The high significance obtained after the quantitative analysis of focal adhesion number by Kruskal-Wallis nonparametric contrast for the 4 groups obtained with the combination of the factors silicon and time (H = 23.506, , df = 3) indicates that silicon, time, or both influence focal adhesion number. Using the two-way ANOVA, the analysis of the effects of each factor and their interaction with the ranks of the variable [38], our results indicate that the model is able to explain 58.8% and that silicon is a significant factor (), while time factor is not (). Furthermore, silicon treated groups (post hoc contrast of Scheffé, ) and untreated groups () can be considered homogeneous at any time, and both groups are different from each other () (Figure 8, Table 1).


GroupsN MinimumMaximumMedianMeanSt. dev.

1PLGA CLEAN 48 H1196274143154.2749.601
2PLGA SILICON 48 H11159311229230.7346.866
3PLGA CLEAN 72 H963198145128.8951.163
4PLGA SILICON 72 H10194340241.5250.5046.049

3.5. Image Analysis: Statistical Analysis of the Shape Variables

The descriptive analysis of the shape variables in the osteoblasts grown in the four experimental groups did not establish a clear relationship with the factors silicon or time. Then, an exploratory factor analysis was performed, in the attempt to reduce the number of morphometric indexes (latent factors). The correlation matrix and the factor loadings matrix were obtained first by the method of principal components and later by varimax rotation, which quantify the relationship between the original variables and the indexes achieved. The first index positively related to circularity and solidity and negatively related to perimeter. This first index represents the property of solid roundness (SR) showing higher values in those cells that are circular, without voids, and with a medium perimeter. The second index contrasts roundness and AR, thus representing stretch (ST) or lengthening, with the highest values for the more elongated cells, with high AR, and negative values more circular cells, with AR close to 1. The third index relates to area and perimeter and can, therefore, be interpreted as the cell size, with higher values for larger cells.

Growing cells were scored for the morphometric indices according to the values obtained in each one by each individual cell. The two-way ANOVA contrast performed for these indices showed that the experimental factor silicon significantly increased () the mean score for SR index, estimating this increase by CI95% = (0.94, 1.71), and also caused a decrease in ST index (), estimated by CI95% = (−1.03, −0.11). Moreover, the factor time caused a decrease in the average score for the ST index (), estimated by CI95% = (−1.06, −0.14), while a significant interaction () was obtained for the index size, as cell size decreases in cells grown on bare PLGA surfaces, CI95% = (−1.28, 0.65), and increases in silicon treated ones, CI95% = (0.32, 1.30). These results indicate that silica treatment, independently of time, favors the presence of cells that were circular and solid (without voids). On the other hand, and independently of silica treatment, the experimental factor time favors a lower ST, or roundness, and increases the size in cells grown on silica treated membranes.

4. Discussion

There are several ways to modify the surface of a material in order to enhance its attractiveness for cell colonization and osteogenic cell differentiation. For biological applications, there is an additional need for versatile deposition methods in the case of devices with potential clinical applications, which should also stand, without alterations, the sterilization processes [13, 16, 18]. We have successfully demonstrated that PECVD TiO2 functionalization methodology employed by our group enhances HOB cells response to nonresorbable PET devices and stands for standard u.v. sterilization [43]. We now herein present a novel design of barrier membrane for GBR purposes, in which HOB cells response to PECVD SiO2 functionalized PLGA membranes has been assessed.

Trace amounts of silicon have been described to substantially contribute to strengthening of bones with promotion of bone formation especially during ageing. Well-dispersed nanosized inorganic particles have been described to enhance the mechanical properties of organic materials [10]. A recent study on biosilica influence on the OPG-RANKL ratio in SaOS-2 cells in vitro suggests both osteoinductive and osteogenic potential of biosilica since it combines an upregulation of the genes required for the differentiation with the potential to increase proliferation of the osteogenic cells [18, 24].

Our PLGA membranes were fabricated by using a conventional resorbable PLGA polymer as substrate and then functionalized by depositing a very thin layer of SiO2, as active layer, by PECVD. A key feature of this method is that it preserved the integrity of the substrate, which remained practically unaltered after the SiO2 as revealed by FT-IR analysis (Figure 3). In comparison with wet chemical routes, which may affect the integrity of this sensitivity substrate, PECVD has been demonstrated to be a quite controllable and friendly procedure for the surface functionalization of resorbable polymers. The absence of a significant damage has been proved here by the AFM analysis of the SiO2/PLGA substrate showing that the surface roughness is not significantly altered after the deposition of SiO2. Stability of these membranes after 72 hours of immersion in a PBS liquid and after UV irradiation sustains that the in vitro cell growth analysis basically refers to the “as prepared” samples without any significant alteration during its manipulation or during their immersion in the culture medium.

Cell adhesion onto a biomaterial surface is a major contributing factor of its cytocompatibility and the host response when implanted, ultimately determining device biocompatibility. Without adhesion, osteoblasts cannot spread or differentiate. A princeps issue in cell adhesion is the development of focal adhesions which, furthermore, are established sites for signal transduction, acting as conveyors of mechanical forces directly to the nucleus via the cytoskeletal network by the complex process of mechanotransduction, where vinculin is required for a strong network formation [1, 4, 44]. Based on the fact that the size and shape of cell spreading area, as well as the number and distribution of  focal adhesion plaques, are decisive for migratory, proliferative, and differentiation behaviour of anchorage-dependent cells, we performed animage-based quantitative feature extraction design in which focal adhesion quantification has been used as marker to assess the osteoconductive potential of the substrata, together with actin cytoskeleton arrangement [2, 17, 20, 45].

The relation between focal adhesion number, functionality, cell movement, and growth of skeletal cells has been described, by our group and others [46], and the formation of super-mature adhesions has also been related to osteogenesis support [47]. Actin polymerization and cytoskeleton rearrangement induced by topographical and chemical cues present in the growing surface are known to serve as driving forces for directional migration and morphological alterations. Of particular interest is the temporal and spatial reorganization of cytoskeleton and the focal adhesion formation in response to SiO2 layer identified in our model, parameters that have been established as important mediators of the mechanotransductive processes, parameters that have been established as important mediators of the mechanotransductive processes [17, 47, 48].

Adherent cells require extracellular matrix anchorage to proliferate and undergo differential function. As shown by our data, HOB cells grown on SiO2 functionalized PLGA membranes actively probe the physical properties of the ECM, with their contractile machinery clearly facilitating the formation of polarized lamellipodia and evenly distributed filopodia, which gather spatial, topographical, and chemical information from the surface. Initial cell tethering and filopodia exploration are followed by lamellipodia ruffling membrane activity and cellular spreading. The results, obtained after a carefully designed in vitro study, are reinforced with a powerful statistical treatment and reveal that in vitro HOB cell morphologies are significantly different and vary greatly depending on the substrata and are consistent with an increased cytoskeletal tension related to focal adhesion increase in SiO2 treated membranes.

5. Conclusions

The methodology described provides a biocompatible and durable functionalization on our PLGA barrier membranes that elicits a significant osteoblast response. Both the morphological changes and the focal adhesion development identified in our model significantly related to SiO2 treated PLGA both the morphological changes and the focal adhesion development identified in our model are significantly related to SiO2 treated PLGA. The novedous SiO2 deposition method reveals as a valuable tool to increase bioactivity of PLGA membranes by combining cell nanotopography cues with the incorporation of bioactive factors, that in addition, stands the standard sterilization protocols.

Conflict of Interests

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

Acknowledgments

The authors thank the Junta de Andalucía (Projects P09-CTS-5189, TEP5283, and FQM-6900) and the Spanish Ministry of Economy and Competitiveness (Projects CONSOLIDER CSD 2008-00023, MAT2010-21228, and MAT2010-18447) and Instituto de Salud Carlos III (FIS PI 09/00508) for financial support (patent P201232018 (Resorbable membrane for guided bone regeneration) PCT pending).

References

  1. M. J. Biggs and M. J. Dalby, “Focal adhesions in osteoneogenesis,” Proceedings of the Institution of Mechanical Engineers H, vol. 224, no. 12, pp. 1441–1453, 2010. View at: Publisher Site | Google Scholar
  2. M. J. P. Biggs, R. G. Richards, and M. J. Dalby, “Nanotopographical modification: a regulator of cellular function through focal adhesions,” Nanomedicine: Nanotechnology, Biology, and Medicine, vol. 6, no. 5, pp. 619–633, 2010. View at: Publisher Site | Google Scholar
  3. E.-J. Lee, S.-H. Teng, T.-S. Jang et al., “Nanostructured poly(ε-caprolactone)-silica xerogel fibrous membrane for guided bone regeneration,” Acta Biomaterialia, vol. 6, no. 9, pp. 3557–3565, 2010. View at: Publisher Site | Google Scholar
  4. T. Orita, M. Tomita, and K. Kato, “Regulation of cellular responses to macroporous inorganic films prepared by the inverse-opal method,” Colloids and Surfaces B: Biointerfaces, vol. 84, no. 1, pp. 187–197, 2011. View at: Publisher Site | Google Scholar
  5. J. A. Sanz-Herrera and E. Reina-Romo, “Cell-biomaterial mechanical interaction in the framework of tissue engineering: insights, computational modeling and perspectives,” International Journal of Molecular Sciences, vol. 12, no. 11, pp. 8217–8244, 2011. View at: Publisher Site | Google Scholar
  6. P. Gentile, V. Chiono, C. Tonda-Turo, A. M. Ferreira, and G. Ciardelli, “Polymeric membranes for guided bone regeneration,” Biotechnology Journal, vol. 6, no. 10, pp. 1187–1197, 2011. View at: Publisher Site | Google Scholar
  7. T.-S. Jang, E.-J. Lee, J.-H. Jo et al., “Fibrous membrane of nano-hybrid poly-L-lactic acid/silica xerogel for guided bone regeneration,” Journal of Biomedical Materials Research B: Applied Biomaterials, vol. 100, no. 2, pp. 321–330, 2012. View at: Publisher Site | Google Scholar
  8. E. Pamula, E. Filová, L. Bačáková, V. Lisá, and D. Adamczyk, “Resorbable polymeric scaffolds for bone tissue engineering: the influence of their microstructure on the growth of human osteoblast-like MG 63 cells,” Journal of Biomedical Materials Research A, vol. 89, no. 2, pp. 432–443, 2009. View at: Publisher Site | Google Scholar
  9. M. Retzepi and N. Donos, “Guided bone regeneration: biological principle and therapeutic applications,” Clinical Oral Implants Research, vol. 21, no. 6, pp. 567–576, 2010. View at: Publisher Site | Google Scholar
  10. J.-H. Song, H.-E. Kim, and H.-W. Kim, “Collagen-apatite nanocomposite membranes for guided bone regeneration,” Journal of Biomedical Materials Research B: Applied Biomaterials, vol. 83, no. 1, pp. 248–257, 2007. View at: Publisher Site | Google Scholar
  11. S.-H. Teng, E.-J. Lee, P. Wang, D.-S. Shin, and H.-E. Kim, “Three-layered membranes of collagen/hydroxyapatite and chitosan for guided bone regeneration,” Journal of Biomedical Materials Research B: Applied Biomaterials, vol. 87, no. 1, pp. 132–138, 2008. View at: Publisher Site | Google Scholar
  12. R. Dimitriou, G. I. Mataliotakis, G. M. Calori, and P. V. Giannoudis, “The role of barrier membranes for guided bone regeneration and restoration of large bone defects: current experimental and clinical evidence,” BMC Medicine, vol. 10, article 81, 2012. View at: Google Scholar
  13. V. Gribova, R. Auzely-Velty, and C. Picart, “Polyelectrolyte multilayer assemblies on materials surfaces: from cell adhesion to tissue engineering,” Chemistry of Materials, vol. 24, no. 5, pp. 854–869, 2012. View at: Publisher Site | Google Scholar
  14. T. Tirri, J. Rich, J. Wolke, J. Seppälä, A. Yli-Urpo, and T. O. Närhi, “Bioactive glass induced in vitro apatite formation on composite GBR membranes,” Journal of Materials Science: Materials in Medicine, vol. 19, no. 8, pp. 2919–2923, 2008. View at: Publisher Site | Google Scholar
  15. Y. Amano, M. Ota, K. Sekiguchi, Y. Shibukawa, and S. Yamada, “Evaluation of a poly-l-lactic acid membrane and membrane fixing pin for guided tissue regeneration on bone defects in dogs,” Oral Surgery, Oral Medicine, Oral Pathology, Oral Radiology, and Endodontics, vol. 97, no. 2, pp. 155–163, 2004. View at: Publisher Site | Google Scholar
  16. M. Vandrovcová and L. Bačáková, “Adhesion, growth and differentiation of osteoblasts on surface-modified materials developed for bone implants,” Physiological Research, vol. 60, no. 3, pp. 403–417, 2011. View at: Google Scholar
  17. C. J. Bettinger, R. Langer, and J. T. Borenstein, “Engineering substrate topography at the Micro- and nanoscale to control cell function,” Angewandte Chemie (International Edition), vol. 48, no. 30, pp. 5406–5415, 2009. View at: Publisher Site | Google Scholar
  18. N. Takeuchi, M. Machigashira, D. Yamashita et al., “Cellular compatibility of a gamma-irradiated modified siloxane-poly(lactic acid)-calcium carbonate hybrid membrane for guided bone regeneration,” Dental Materials Journal, vol. 30, no. 5, pp. 730–738, 2011. View at: Publisher Site | Google Scholar
  19. C. K. Choi, M. T. Breckenridge, and C. S. Chen, “Engineered materials and the cellular microenvironment: a strengthening interface between cell biology and bioengineering,” Trends in Cell Biology, vol. 20, no. 12, pp. 705–714, 2010. View at: Publisher Site | Google Scholar
  20. F. Intranuovo, P. Favia, E. Sardella et al., “Osteoblast-like cell behavior on plasma deposited micro/nanopatterned coatings,” Biomacromolecules, vol. 12, no. 2, pp. 380–387, 2011. View at: Publisher Site | Google Scholar
  21. V. Puddu and C. C. Perry, “Peptide adsorption on silica nanoparticles: evidence of hydrophobic interactions,” ACS Nano, vol. 6, pp. 6356–6363, 2012. View at: Google Scholar
  22. Y. Tang, Y. Zhao, X. Wang, and T. Lin, “Layer-by-layer assembly of silica nanoparticles on 3D fibrous scaffolds: enhancement of osteoblast cell adhesion, proliferation, and differentiation,” Journal of Biomedical Materials Research, 2013. View at: Publisher Site | Google Scholar
  23. M. Vallet-Regí, M. Colilla, and B. González, “Medical applications of organic-inorganic hybrid materials within the field of silica-based bioceramics,” Chemical Society Reviews, vol. 40, no. 2, pp. 596–607, 2011. View at: Publisher Site | Google Scholar
  24. X. Wang, H. C. Schröder, M. Wiens, H. Ushijima, and W. E. G. Müller, “Bio-silica and bio-polyphosphate:applications in biomedicine (bone formation),” Current Opinion in Biotechnology, vol. 23, pp. 570–578, 2012. View at: Google Scholar
  25. H. Shen, X. Hu, J. Bei, and S. Wang, “The immobilization of basic fibroblast growth factor on plasma-treated poly(lactide-co-glycolide),” Biomaterials, vol. 29, no. 15, pp. 2388–2399, 2008. View at: Publisher Site | Google Scholar
  26. Y. Wan, X. Qu, J. Lu et al., “Characterization of surface property of poly(lactide-co-glycolide) after oxygen plasma treatment,” Biomaterials, vol. 25, no. 19, pp. 4777–4783, 2004. View at: Publisher Site | Google Scholar
  27. C. Witt and T. Kissel, “Morphological characterization of microspheres, films and implants prepared from poly(lactide-co-glycolide) and ABA triblock copolymers: is the erosion controlled by degradation, swelling or diffusion?” European Journal of Pharmaceutics and Biopharmaceutics, vol. 51, no. 3, pp. 171–181, 2001. View at: Publisher Site | Google Scholar
  28. J. Gao, L. Niklason, and R. Langer, “Surface hydrolysis of poly(glycolic acid) meshes increases the seeding density of vascular smooth muscle cells,” Journal of Biomedical Materials Research, vol. 42, pp. 417–424, 1998. View at: Google Scholar
  29. A. C. R. Grayson, M. J. Cima, and R. Langer, “Size and temperature effects on poly(lactic-co-glycolic acid) degradation and microreservoir device performance,” Biomaterials, vol. 26, no. 14, pp. 2137–2145, 2005. View at: Publisher Site | Google Scholar
  30. C. E. Holy, S. M. Dang, J. E. Davies, and M. S. Shoichet, “In vitro degradation of a novel poly(lactide-co-glycolide) 75/25 foam,” Biomaterials, vol. 20, no. 13, pp. 1177–1185, 1999. View at: Publisher Site | Google Scholar
  31. H. Kranz, N. Ubrich, P. Maincent, and R. Bodmeier, “Physicomechanical properties of biodegradable poly(D, L-lactide) and poly(D, L-lactide-co-glycolide) films in the dry and wet states,” Journal of Pharmaceutical Sciences, vol. 89, pp. 1558–1566, 2000. View at: Google Scholar
  32. M. Källrot, U. Edlund, and A.-C. Albertsson, “Surface functionalization of degradable polymers by covalent grafting,” Biomaterials, vol. 27, no. 9, pp. 1788–1796, 2006. View at: Publisher Site | Google Scholar
  33. J. S. C. Loo, C. P. Ooi, and F. Y. C. Boey, “Degradation of poly(lactide-co-glycolide) (PLGA) and poly(L-lactide) (PLLA) by electron beam radiation,” Biomaterials, vol. 26, no. 12, pp. 1359–1367, 2005. View at: Publisher Site | Google Scholar
  34. H. Tsuji, Y. Tezuka, and K. Yamada, “Alkaline and enzymatic degradation of L-lactide copolymers. II. crystallized films of poly(L-lactide-co-D-lactide) and poly(L-lactide) with similar crystallinities,” Journal of Polymer Science B: Polymer Physics, vol. 43, no. 9, pp. 1064–1075, 2005. View at: Publisher Site | Google Scholar
  35. A. Barranco, J. Cotrino, F. Yubero et al., “Synthesis of SiO2 and SiOxCyHz thin films by microwave plasma CVD,” Thin Solid Films, vol. 401, no. 1-2, pp. 150–158, 2001. View at: Publisher Site | Google Scholar
  36. A. Barranco, F. Yubero, J. Cotrino et al., “Low temperature synthesis of dense SiO2 thin films by ion beam induced chemical vapor deposition,” Thin Solid Films, vol. 396, no. 1-2, pp. 9–15, 2001. View at: Publisher Site | Google Scholar
  37. D. A. Shah and L. V. Madden, “Nonparametric analysis of ordinal data in designed factorial experiments,” Phytopathology, vol. 94, no. 1, pp. 33–43, 2004. View at: Google Scholar
  38. T. L. Barr, “An XPS study of Si as it occurs in adsorbents, catalysts, and thin films,” Applications of Surface Science, vol. 15, no. 1–4, pp. 1–35, 1983. View at: Google Scholar
  39. J. Finster, D. Schulze, F. Bechstedt, and A. Meisel, “Interpretation of XPS core level shifts and structure of thin silicon oxide layers,” Surface Science, vol. 152-153, no. 2, pp. 1063–1070, 1985. View at: Google Scholar
  40. M. M. Stevanovic, B. Jordovic, and D. P. Uskokovic, “Preparation and characterization of poly(D, L-lactide-co-glycolide) nanoparticles containing ascorbic acid,” Journal of Biomedicine and Biotechnology, vol. 2007, Article ID 84965, 8 pages, 2007. View at: Publisher Site | Google Scholar
  41. H. Aita, N. Hori, M. Takeuchi et al., “The effect of ultraviolet functionalization of titanium on integration with bone,” Biomaterials, vol. 30, no. 6, pp. 1015–1025, 2009. View at: Publisher Site | Google Scholar
  42. W. Att, N. Hori, F. Iwasa, M. Yamada, T. Ueno, and T. Ogawa, “The effect of UV-photofunctionalization on the time-related bioactivity of titanium and chromium-cobalt alloys,” Biomaterials, vol. 30, no. 26, pp. 4268–4276, 2009. View at: Publisher Site | Google Scholar
  43. A. Terriza, A. Diaz-Cuenca, F. Yubero et al., “Light induced hydrophilicity and osteoblast adhesion promotion on amorphous TiO2,” Journal of Biomedical Materials Research A, vol. 101, pp. 1026–1035, 2013. View at: Google Scholar
  44. M. J. P. Biggs, R. G. Richards, N. Gadegaard et al., “Interactions with nanoscale topography: adhesion quantification and signal transduction in cells of osteogenic and multipotent lineage,” Journal of Biomedical Materials Research A, vol. 91, no. 1, pp. 195–208, 2009. View at: Publisher Site | Google Scholar
  45. L. Bacakova, E. Filova, F. Rypacek, V. Svorcik, and V. Stary, “Cell adhesion on artificial materials for tissue engineering,” Physiological Research, vol. 53, supplement 1, pp. S35–S45, 2004. View at: Google Scholar
  46. M. Salido, J. I. Vilches-Perez, J. L. Gonzalez, and J. Vilches, “Mitochondrial bioenergetics and distribution in living human osteoblasts grown on implant surfaces,” Histology and Histopathology, vol. 24, no. 10, pp. 1275–1286, 2009. View at: Google Scholar
  47. L. E. McNamara, T. Sjöström, K. E. V. Burgess et al., “Skeletal stem cell physiology on functionally distinct titania nanotopographies,” Biomaterials, vol. 32, no. 30, pp. 7403–7410, 2011. View at: Publisher Site | Google Scholar
  48. M. J. Dalby, “Topographically induced direct cell mechanotransduction,” Medical Engineering and Physics, vol. 27, no. 9, pp. 730–742, 2005. View at: Publisher Site | Google Scholar

Copyright © 2014 Antonia Terriza 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.


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