Synthetic osteogenic extracellular matrix formed by coated silicon dioxide nanosprings
- Jamie L Hass1Email author,
- Erin M Garrison2,
- Sarah A Wicher2,
- Ben Knapp1,
- Nathan Bridges1,
- DN Mcllroy†1 and
- Gustavo Arrizabalaga2
© Hass et al; licensee BioMed Central Ltd. 2012
Received: 11 October 2011
Accepted: 27 January 2012
Published: 27 January 2012
The design of biomimetic materials that parallel the morphology and biology of extracellular matrixes is key to the ability to grow functional tissues in vitro and to enhance the integration of biomaterial implants into existing tissues in vivo. Special attention has been put into mimicking the nanostructures of the extracellular matrix of bone, as there is a need to find biomaterials that can enhance the bonding between orthopedic devices and this tissue.
We have tested the ability of normal human osteoblasts to propagate and differentiate on silicon dioxide nanosprings, which can be easily grown on practically any surface. In addition, we tested different metals and metal alloys as coats for the nanosprings in tissue culture experiments with bone cells.
Normal human osteoblasts grown on coated nanosprings exhibited an enhanced rate of propagation, differentiation into bone forming cells and mineralization. While osteoblasts did not attach effectively to bare nanowires grown on glass, these cells propagated successfully on nanosprings coated with titanium oxide and gold. We observed a 270 fold increase in the division rate of osteoblasts when grow on titanium/gold coated nanosprings. This effect was shown to be dependent on the nanosprings, as the coating by themselves did not alter the growth rate of osteoblast. We also observed that titanium/zinc/gold coated nanosprings increased the levels of osteoblast production of alkaline phosphatase seven folds. This result indicates that osteoblasts grown on this metal alloy coated nanosprings are differentiating to mature bone making cells. Consistent with this hypothesis, we showed that osteoblasts grown on the same metal alloy coated nanosprings have an enhanced ability to deposit calcium salt.
We have established that metal/metal alloy coated silicon dioxide nanosprings can be used as a biomimetic material paralleling the morphology and biology of osteogenic extracellular matrix. The coated nanosprings enhance normal human osteoblasts cellular behaviors needed for improving osseointegration of orthopedic materials. Thus, metal-coated nanosprings represent a novel biomaterial that could be exploited for improving success rates of orthopedic implant procedures.
Keywordsnanosprings nanomaterials osteoblasts osseointegration calcification bone regeneration
The assembly of individual cells into functional, healthy, tissue relies on the structural and morphological integrity of the extracellular matrix (ECM) . Consequently, many efforts to bioengineer the ECM by mimicking its three dimensional structure at the nanoscale have been undertaken [2, 3]. The goal of for these artificial matrixes is to serve as scaffolds upon which tissue development, both in vitro and in vivo, can be promoted and accelerated. Indeed, several nanomaterials, form structural complexes that efficiently allow proliferation and differentiation of various types of cells, including cardiomyocytes, epithelial cells, hepatocytes and osteoblasts .
Special attention has been put into making a prototypical system mimicking the nanostructures of the ECM of bone, as there is a need to find materials that can enhance the bonding between orthopedic devices and this tissue [4, 5]. The most common cause of orthopedic implant failure is a suboptimal bone-implant interface, caused by the lack of integration of the implant into the bone structure (i.e. osseointegration), which leads to aseptic loosening . Consequently, efforts to bioengineer bone ECM by mimicking its three dimensional structure at the nanoscale has been undertaken .
The process of osseointegration involves the bone healing around the orthopedic device. Healing occurs at a nanoscale level as specialized cells, osteoblasts, secrete both the organic and inorganic components of the bone ECM. The efficiency of this process relates to the degree of mineralization that occurs during the healing process . A crystalline organic phase (collagen) makes up 90% of the organic component of the bone matrix while the inorganic component of bone ECM is mainly a crystalline mineral phase, hydroxyapatite crystal (HA), which makes up 65% of the bone matrix and provides the strength property of bone . Besides providing a structural scaffold, the ECM is known to regulate important cellular functions such as proliferation, migration, adhesion and differentiation . Thus, the ideal coating for orthopedic implants is one that mimics the morphology of the natural bone ECM and also contains chemical properties that induce osteoblast growth and development.
A novel approach to the generation of new implant materials takes advantage of the advent of nanomaterials. Foremost, the allure of nanomaterials is the significant increase in surface area they provide. By simply increasing the surface area, the nanomaterials can provide additional points on an implant for the bone to contact, which in turn improve the chances for osseointegration. Osteoblast attachment, growth, proliferation and differentiation have shown to be enhanced by various nanosurfaces. Tantala nanotubes, titanium dioxide (TiO2) nanotubes, carbon nanotubes and hydroxyapatite nanocrystallites have all been investigated for osteogenic properties [2, 5, 9].
We have recently developed a new type of nanomaterial, silicon dioxide nanosprings (NS) , which showed characteristics that make it a good candidate for an artificial bone ECM and thus as an implant coating. NS are a helical form of silicon dioxide nanowires that form an amorphic mat, where the thickness and density of the mat can be controlled to produce varying degrees of porosity . NS form via vapor-liquid-solid procedure and can be easily grown on a variety of substrates, including metals, ceramic, and even some high temperature plastics [12, 13].
The nanosprings are remarkably similar to bone's collagen fiber type 1 (CF1), the main organic component of bone ECM. The NS are comparable in both size and shape to this protein [8, 10]. The diameter of the average nanospring (191.8 ± 43.6 nm) is comparable to the diameter of extracellular CF1 (191 nm) [15–17]. Because CF1 is a helical crystal of repeating functional sites, of which there are many hydroxyl sites, it provides numerous bonding and attachment sites over its entire length . The NS mimic this behavior because they are a helical structure, which possess uniform repeating chemical makeup of hydroxyls that provide interaction points for the osteoblasts. The addition of coatings provides the surface properties not unlike those of the hexagonal lattice formed by HA, which is bonded to CF1 . Therefore, the coated nanosprings have the potential to mimic the organic and inorganic components of bone ECM and serve as an artificial surface for bone cell growth.
Here we show that NS coated with a variety of chemicals not only allow growth of human osteoblast in tissue culture, but also increase the rate at which they divide. Furthermore, we have discovered that osteoblasts grown on coated NS have a higher rate of differentiating into mature bone cells, which mineralize and potentially form mature bone. These results indicate that NS could be a useful substrate to induce osseointegration of orthopedic implants, which would reduce implant failure.
Results and discussion
Nanosprings can be grown on glass discs and autoclaved
To analyze the compatibility of NS with bone cell growth and development, we established a system that allowed us to easily monitor and analyze cell proliferation and differentiation. Glass cover slips are an ideal material for cell culture as they allow cell adhesion, growth of most cell types and they mount on slides for microscopy analysis. NS grown to our specifications on the glass discs using a vapor-liquid-solid method [10, 11] were purchased from GoNano Inc. (Moscow, Idaho). Visual analysis of the discs after nanospring growth was performed using field emission scanning electron microscopy (FESEM) and allowed us quality control that the silica NS grown on glass formed helical structures characteristic of this nanomaterial. The nanospring density on the cover slips ranged from 0.71 to 1.01 mg/cm2.
Given the relative lack of information available on the interaction between osteoblasts and metal/metal alloy nanosurfaces, we also coated the NS with either of 2 different biocompatible materials, gold nanoparticles (Au), titania (TiO2) or with combinations of them with, or without, zinc oxide (ZnO) (i.e. TiO2/Au, TiO2/ZnO and TiO2/Au/ZnO). Coatings with ZnO or ZnO/Au were not done because of the sensitivity and toxicity of bone cells to zinc oxide. Toxicity of bone cells to ZnO is reported to occur at a blood level of 0.1 μg/cm3 and the density of this coating on the NS, which is the actual surface contact amount, is ~ 3000.0 μg/cm2 [18, 19]. Even with the gold nanoparticles, which covered only 16% of the surface at most (EDS data), the ZnO level would be too high. Nonetheless, we wanted to include ZnO in some samples to examine the response of osteoblasts to the properties of conductivity, piezoelectricity and low thermal expansion that the underlayer of ZnO might provide. For this purpose we first added ZnO to the cover slips and then covered them with the TiO2 layer, which is likely to protect the cells against the effects of the ZnO layer.
Coating densities were calculated to be 0.5 ± 0.05 mg/cm2 for titania, 3.0 ± 0.05 mg/cm2 for zinc oxide and 0.015 ± 0.003 mg/cm2 for gold nanoparticles. An important requirement for the utilization of nanomaterials for any biomedical purpose is the ability to sterilize the material prior to use as to avoid introduction of microbial contamination. Thus, we tested the ability of the NS grown on glass to withstand sterilization temperatures (134°C) and pressures (4 PSI or 207 Torr) for 35 minutes in an autoclave. Attachment of the NS to the glass cover slips was maintained through the autoclaving process and FESEM analysis showed no effect on the integrity or structure of the NS. In addition to FESEM, EDS was also preformed, which showed statistically (p-value < 0.0001, Anova) no change in the atomic content at the surface when evaluated at 15 and 20 kV at magnifications of 50× and 500×. The bare NS and coated NS are fabricated out of robust biocompatible metals, for which the melting temperatures are very high, lowest melting temperature for the materials used is for silicon dioxide and gold, ~1600°C and these metal/metal alloys have been widely reported for their ability to withstand sterilization procedures. Thus, NS are ideally suited for use in both in vitro and in vivo tissue studies as the can be easily sterilized using standard methods.
Osteoblasts exhibit an enhanced proliferation rate when grown on coated nanosprings
Our proliferation studies strongly suggest that osteoblast divide at a faster rate when grown on NS along with either TiO2/Au or TiO2/Au/ZnO coatings. To more precisely explore this phenomenon we added the same number of cells to plain cover slips and cover slips containing NS with those two different coatings and counted the number of live cells after 24, 72 and 120 hrs. (Figure 3B). While the doubling rate between 24 and 120 hours for cells grown on plain glass was every 22.2 hours, cells grown on NS with TiO2/Au and NS with TiO2/Au/ZnO double their numbers every 8.2 and 14.4 hours respectively, during the same time period (Figure 3B). Thus, NS coated with titania and gold nanoparticles accelerated the division of osteoblasts by almost three times of what is observed under normal growth conditions.
The pores and the scaffolding present in bone ECM are known to play a role in differentiation, likely by providing pockets of surface charges in which projections from the osteoblasts can sense the lack of mineralization . Pore size in natural bone varies quite a bit (20-400 μm) depending on location and function needed such as support or a fulcrum point . The nanospring mat can also be fabricated to achieve different levels of porosity and the pores on the samples used for this study ranged between 5-25 μm. Consequently, the porous nature of the NS mat might have contributed to the effect of the coated NS on osteoblasts osteogenic behavior by providing a greater number of gaps that can interact with the osteoblasts and be filled with bone matrix.
The enhanced proliferation with coated NS, confirms our hypothesis that the mats of NS, because of the similar morphology to collagen, provide an excellent material upon which to grow NHOs. Conversely, these findings also indicate that the morphological similarities between NS and collagen alone are not sufficient to enhance proliferation and that surface chemistry and stoichiometry are equally important, as borne out by the lack of enhanced proliferation on uncoated NS. To the best of our knowledge, this is the first study of nanomaterials to definitely demonstrate the equal importance of the nanomaterial's morphology and stoichiometry on osteoblast proliferation.
The bare NS used in this study were completely hydrophilic and thus we hypothesize that a monolayer of water forms around the bare NS, which in turn would block binding of proteins and cells as reported with other completely hydrophilic surfaces . Thus, the decrease in proliferation on hydrophilic NS without coatings might be due to a decrease in attachment as oppose to a direct effect on the NHO proliferation ability. It was noted during incubation, that the NHO stayed rounded up instead of becoming their typical elongated columnar morphology and we did not observe a higher percent of dead cells on cultures grown on plain NS (additional file 2).
The coatings that had the biggest effect on cell proliferation where those that combined TiO2 and Au (Figure 3A). Interestingly, neither of these materials enhanced proliferation over the control when used by themselves to coat the nanosprings. Thus gold and titanium on nanosprings appear to have a synergistic or cooperative effect to enhance the doubling rate of osteoblasts. Why these materials are having such an effect is not understood at this point. One possibility is that together they modify the 3-D structure of the NS array in a way that is more conducive to osteoblast division. It is also possible that these metals are providing additional sites for the osteoblasts to attach to. It has been shown that many proteins found in bone EMC, including fibronectin and osteonectin attach to gold nanoparticles [21, 22]. Thus, it is possible that the addition of gold nanoparticles imparts sites of protein attachment along the length of the nanosprings thus enhancing proliferation. Similarly titania has been shown to be bioactive and biocompatible for osteoblasts and these cells can attach to this metal alloy . Previously, it has been found that titania surfaces have an alternating chemical composition between hydrogen and hydroxyls and do not form a water monolayer . So the titania might be influencing osteoblast proliferation directly by providing sites of attachment or indirectly by eliminating a water shell. Consistent with either of these possibilities, osteoblasts were noted to attach more efficiently to the TiO2 coated nanosprings (data not shown).
The fast propagation rate of cells grown on coated nanosprings is reversible
It is conceivable that when grown on NS, osteoblast are transformed to faster dividing cells, because they either mutated or differentiated into a different type of cell. To determine whether the fast proliferative phenotype of osteoblasts grown on NS constitutes a permanent change in the cells we tested the proliferation rate of cells previously grown on NS. For this purpose, cells grown for 4 days on either normal cell culture conditions, TiO2/Au coated NS, or TiO2/Au/ZnO coated NS were harvested and the same number of cells were added to plain cover slips to monitor their growth. Regardless of how the cells were grown previous to the test, we observed the same number of cells 4 days later. This indicates that the high proliferation rate of the cells grown on NS is a reversible trait and that the NS did not permanently transformed the cells in the time frame tested (Figure 3C).
Coated NS enhance osteoblast development
In terms of differentiation, the presence of TiO2 appears to have an important osteogenic effect. The TiO2 thin coating is expected to be insulative and effectively hold charges. Furthermore, this anatase form of titania is expected to provide a negative charge shell in presence neutral pH cell media . The conductivity of bone and the piezoelectric effects of CF1, which produces negative surface charges, are known to be instrumental in bone healing . Thus, TiO2 may enhance differentiation by affecting the ionic environment, or providing the electrostatic charges that normally promote osteoblast responses during bone growth in vivo.
Calcium salt deposition is enhanced in osteoblasts grown on coated nanosprings
To quantitate the Von Kossa staining results we calculated the percentage of the area covered by black spots on randomly pick fields of view using MetaMorph™ image analysis. In normal growth conditions, we detected 0.104 ± 0.089% coverage of black stain in the areas analyzed, which was not different then what was observed with the same surface in the absence of cells. By contrast, cultures with cells grown on TiO2/ZnO/Au coated NS exhibited 60.18 ± 11.50% coverage by the stain, which represented a 11.51 fold increase over what was detected when the same surface without cells was stained. Thus, consistent with the fact that cells grown on coated NS are differentiating into bone forming cells, these cells exhibit the ability to deposit calcium salts and presumably to induce calcium deposition.
To verify the presence of bone matrix on those samples, we directly visualized them using FESEM at a magnification of 10.00 KX. While normal growth cultures showed some clusters of what appears to be hydroxyapatite crystals (Figure 5B; arrow), it contained dramatically less crystal formations than the cultures grown on NS + TiO2/ZnO/AuNP, which were almost completely covered uniformly in crystals (Figure 5B).
Percent Ca, P and Ag in relation to total% atoms on surface of cultures grown on either plain glass discs or NS coated with TiO2/ZnO/Au as determined by energy dispersion spectroscopy.
NS + TiO2/ZnO/Au
Potential applications of coated nanosprings
Treatment of disorders of the musculoskeletal system, such as skeletal deformities and traumatic injuries that result in fractures, usually involve the use of orthopedic implants. One of the key challenges in this field is assuring that orthopedic implants are permanently and securely set in place. Due to the importance of the nanostructure of the bone ECM in tissue formation and development, significant efforts have been made in the engineering of biomaterials that can mimic its three dimensional characteristics of the ECM. To be of use in the in the enhancement of orthopedic implants these artificial matrixes need to serve as scaffolds for tissue growth, be easy to be grown on a variety of surfaces, able to be sterilized and have the potential for being functionalized with growth factors and proteins. In this respect, the metal-coated NS might represent an ideal nanomaterial to use as a coating on devices that need to integrate into bone.
While silica nanosprings are usually grown on silicon wafers or aluminum foil substrates for industrial uses, they can be mass-produced on a variety of surfaces including glass, titanium and ceramics. The NS grown on glass proved durable in our long-term tissue culture experiments, as we never observed delamination of the NS from the glass surface. Another advantage of the nanosprings we tested over other nanomaterials is their resistance to strong sterilization methods such as high temperature. Autoclavable materials are preferable over ones that require alcohols or ultraviolet light sterilization, since heat sterilization is easier, relatively less expensive and accessible in most medical settings.
Furthermore, the presence of metal alloys increases the versatility of this nanomaterial since the metals can serve as acceptors for the addition of proteins and other functionalizing factors. The use of AuNP as a coating, in particular, would allow us to use established surface functionalizing chemistry that can be exploited to add osteogenic factors or HA to further promote bone formation [29, 30]. Potential candidates to be attached to the NS include the bone morphogenic protein-2 (BMP-2) and HA. BMP-2 is well known to stimulate bone deposition by osteoblast . While BMP-2 has been added directly to the surface of orthopedic implants, it did appear to aid osseointegration, most likely because of loss of the protein from the orthopedic device's surface during implantation . Introducing the protein attached to coated nanosprings may increase the adherence of the BMP-2 to the implant's surface and potentially its stability.
The other coatings we tested also proved beneficial to the propagation and development of human osteoblasts and increased the usability of NS as an implant coating. Titanium is a very common metal for many orthopedic implants because of its strength and non-corrosive ability . The titania coating used in our experiments is in the anatase form, which has been shown to be more bioactive and biocompatible to human osteoblasts . The other metal alloy coating, zinc oxide, which is commonly used in dental cements  provides interesting electrochemical properties to our nanospring coatings, and we hypothesize that this zinc oxide coating has the same crystal hexagonal structure as HA.
The results presented here show that coated nanosprings can enhance the propagation, development and ability to deposit calcium salt of human osteoblasts. Furthermore, our studies allowed us to compare the responses of human osteoblasts to different metal/metal alloys being used as coating for the nanosprings, which showed unique results between proliferation and differentiation/calcium salt deposition behaviors. It is our hypothesis that the nanosprings along with their coatings provided a scaffold for controlled and guided growth as well as additional surfaces and elements for attachment. The ease of the NS to be attached to different surfaces at different densities, autoclaved for sterility and coated with a variety of metal alloys along with its unique morphology are desired traits that can be exploited to enhance osseointegration of biomaterials into living bone.
Cell line and culture
Normal Human Osteoblasts (NHO) supplied by Lonza Inc. (Walkersville, MD) were used for all experiments. We followed the company's instructions for preparing subcultures, calculating cell count, cell viability and seeding density. Cells were grown at 37°C and 5% CO2 on osteoblast growth medium (OGM), which consisted of osteoblast basal medium (Lonza, Inc.) supplemented with Clonetics SingleQuots (Lonza, Inc.) which included fetal bovine serum (FBS), ascorbic acid, and gentamicin/amphotericin B. The OGM was made following the company's specifications.
Production of silicon dioxide nanosprings™ on glass discs
Nanospring mats were grown, to our specifications, via a vapor-liquid-solid (VLS) mechanism and purchased from GoNano Technologies, Inc. A detailed description of the process was previously reported by McIlroy et al.  and Wang et al. . Nanosprings were fabricated on 12 mm diameter microscope cover glass discs (Fisher Scientific) in an atmospheric furnace at a constant O2 flow rate using a gold layer as a catalyst and a proprietary silicon precursor [US Patent application 11/993452 filed, 2010]. The growth time was approximately 15 minutes, which produced an 80-μm thick nanospring mat.
Atomic layer deposition (ALD) was used to coat the nanosprings with zinc oxide (ZnO) and titania (TiO2) [35, 36]. ALD coatings were carried out in a tube furnace maintained at 170°C for diethyl zinc and 300°C for titanium tetrachloride (TiCl4) [35, 37]. Between each pulse of precursor, or water, which was used as a reactant, the system was purged with N2 to ensure that the precursors reacted only at the surface of the growing film . For gold coating, glass discs covered with nanosprings were immersed in a gold tetrachloride (AuCl4) solution in reagent grade ethanol. After air-drying at room temperature, the samples were reduced in an atmosphere of H2 and Ar for 15 minutes at 300°C. The samples were then cooled down to room temperature in Ar atmosphere to avoid oxidation.
Pre and post coating weights along with FESEM dimension of the NS were used to calculate density and determine the% weight of coating/NS for each glass disc. To verify morphology and quality of the NS mat after growth and coating procedures, all samples were analyzed visually with field emission scanning electron microscopy (FESEM).
Cell Culture on Silicon Dioxide Nanosprings™ coated glass discs
NS coated glass discs were rinsed with deionized water and then washed for 10 minutes with 70% ethanol. The NS samples were air dried and placed in autoclave sleeves and conventionally autoclaved for 20 minutes. NS discs were place in wells of tissue culture 24 well plate and rinsed once with OGM. Fresh OGM was then added and plates were incubated at 5% CO2 37°C for 30 minutes before adding osteoblasts.
Quantification of cell proliferation
10, 000 cells were added to each well containing glass cover slips. The plates were incubated at 37°C, 5% CO2 for 5 days. At days 1 and 3, culture media was replaced with 0.2% calcein blue (Molecular Probes, Invitrogen) in OGM and the plates were incubated for 15 minutes at 37°C with 5% CO2. Calcein blue stain was then rinsed twice with N'-2-hydroxyethylpiperazine-N'-Ethanesulfonic Acid (HEPES, pH 7.37, Lonza Inc.) and stained cells, which represent live cells, were counted in 5 views at 200× using a Zeiss Axiovert 40 CFL microscope. After counting, cells were washed 3 times with warm OGM and returned to tissue culture incubator to continue growth; this gives a true proliferation rate for a given culture. At day 5 of the experiment cells were terminally stained with Vybrant Green (Invitrogen) to detect all cells and propidium iodide (PI, Invitrogen) to detect dead cells. In specific, wells were rinsed twice with HEPES followed by addition of 0.06% PI, 0.16% vybrant green in PBS. After 20 min incubation at 37°C, the wells were washed with PBS two times. Cells were visualized at 200× with Zeiss Axiovert 40 CFL microscope, and the number of Vybrant Green positive and PI positive cells on 5 fields of view was counted. For each randomly selected field of view both the total and dead cells were counted before moving to the next viewing field. Images of characteristic fields of view were captured using a Canon Powershot G6 camera. There were a total of 3 testing cover slips for each coating being tested in each independent experiment and the experiment was repeated for a total of 3 independent assays. Thus, for each condition we counted cells in a total of 9 cover slips.
To determine if the NS permanently affected cell proliferation, 2, 000 osteoblasts were allowed to grow on control glass discs and coated NS discs for 4 days. After that point cells were detached and collected from the cover slips using the ReagentPac™ system (Lonza Inc.) according to manufacturer's instructions. 500 cells harvested form each of the different cultures were then added to plain glass cover slips allowing them to grow for 3 days at which time the number of live cells was determined using calcein blue stain.
Alkaline phosphatase measurements
Control glass discs and the respective NS containing discs were placed in 24-well plates and a total of 10, 000 osteoblasts were added to each to the well. Cultures were then incubated at 37°C, 5% CO2 in OGM for 36 days based on published methods . To maintain the pH and nutrient levels, media was changed every 4 days during this incubation period. At the end of the 36 days incubation, discs were carefully removed from the wells and placed into empty wells and then washed with HEPES two times before adding triton X-100 at 1% (500 ul/well) to lyse cells. The plates were incubated for 2 hours at 37°C, 5% CO2 and then lysates were transferred into microcentrifuge tubes and three rounds of freeze/thaw cycles were done at -80°C. QuantiChrom™ Alkaline Phosphatase Assay (BioAssay Systems) was used to test alkaline phosphatase levels according to manufacturer's instructions. As part of this process an EL 808 ultra microplate reader (Biotek Instruments Inc.) spectrometer was used to read emission at 405 nm. Determining total protein level for each sample normalized the readout of alkaline phosphatase activity. Total protein levels were determined using the BCA (bicinchoninic acid) protein assay (Pierce Incorporated) according to manufacturer's instructions.
Calcium deposition studies
For calcium salt deposition experiments, osteoblast growth media was supplemented with hydrocortisone (200 nM) and β-glycerophosphate (2.0 mM). We added 10, 000 cells per sample and incubated the cultures at 37°C, 5% CO2 for 36 days while changing media every 3-4 days. Mineral staining was done with Von Kossa stain system (American MasterTech). In brief, media was removed and 2 mls of 3.7% formaldehyde with PBS (1:9) was added to each well and incubated for 20 minutes. All samples underwent a serial alcohol dehydration process (i.e. 70% ethanol for 10 minutes, 80% for 10 minutes, 90% for 20 minutes, and rinse with absolute alcohol). The serial dehydration process was done at this point to promote better imaging of the biologic material with the FESEM . Each sample was then rinsed three times with deionized water. Staining protocol by the manufacturer was followed. The disks were viewed under light microscopy to see the dark brown or black metallic silver stain positively identifying phosphate anions of the calcium salt deposition while the cells stained red. Imaging was done using a Leica MZ16F fluorescent stereoscope, a Leica DFC420 color digital camera and Leica Application Suite software.
The % coverage of positive Von Kossa stain/area was determined by using MetaMorph™ software. Three areas of the same size on each sample were examined from the tiff image obtained from the Leica DFC420 camera. We set the color threshold to cover half of the gray scale and minimized the red hue to avoid detecting the red color contributed by gold nanoparticles, modifying a Von Kossa quantification method (BD Biosciences, technical bulletin #444). The modified method excludes less developed nodules that stained yellow to light brown. The set parameters allowed pixels to be counted that reached the resorbed part of the histogram, which represented a well-developed calcium mineral nodule. The software attained these counts that reached the set threshold in a total specified area and calculated the% threshold/area.
Scanning Electron Microscopy and Energy Dispersion Spectroscopy
Energy dispersion spectroscopy (EDS) and FESEM was done on the samples taken from the Von Kossa calcium salt deposition study. EDS was first done using 15 kV and 20 kV, in different areas of the discs at 70 X, 300 × and 5 KX. The results of the different magnifications all had very similar quantitative and% atom content for the particular disc. The samples were coated with gold for the FESEM images (SPI-Module™ Sputter Coater; West Chester, PA) for 50 seconds. FESEM images were taken of each disc at 500×, 5 KX, 10 KX and 20 KX using Zeiss SmartSEM, with a Gemini electron gun .
List of abbreviations
silicon dioxide nanosprings
collagen fiber type 1
field emission scanning electron microscopy
normal human osteoblasts
energy dispersion spectroscopy
bone morphogenic protein-2
osteoblast growth medium
fetal bovine serum
atomic layer deposition
We would like to acknowledge Franklin Bailey, Ann Norton and Tom Williams for their technical support. This work was supported by a development grant from the University of Idaho. NIH Grant Number P20 RR016454 from the INBRE Program of the National Center funded J.H. for Research Resources. The laboratory of G.A. is also funded by NIH grant R01 AI 89808-01. This work was also partly funded by funds from the Higher Education Research Council of Idaho and by the University of Idaho BanTech.
- Enderle J, Blanchard S, Bronzino J: Introduction to Biomaterials. 2005, Oxford, UK: Elsevier Academic Press, 2Google Scholar
- Dvir T, Timko BP, Kohane DS, Langer R: Nanotechnological strategies for engineering complex tissues. Nat Nano. 2011, 6: 13-22.View ArticleGoogle Scholar
- Holzwarth JM, Ma PX: Biomimetic nanofibrous scaffolds for bone tissue engineering. Biomaterials. 2011, 32: 9622-9629. 10.1016/j.biomaterials.2011.09.009.View ArticleGoogle Scholar
- Streicher RM, Schmidt M, Fiorito S: Nanosurfaces and nanostructures for artificial orthopedic implants. Nanomedicine. 2007, 2: 861-874. 10.2217/17435822.214.171.1241.View ArticleGoogle Scholar
- Kim J-H, Cho K-P, Chung Y-S, Kim O-S, Chung S-S, Lee K-K, Lee D-J, Lee K-M, Kim Y-J: The effect of nanotubular titanium surfaces on osteoblast differentiation. J Nanosci Nanotechnol. 2010, 10: 3581-3585. 10.1166/jnn.2010.2235.View ArticleGoogle Scholar
- Niehaus AJ, Anderson DE, Samii VF, Weisbrode SE, Johnson JK, Noon MS, Tomasko DL, Lannutti JJ: Effects of orthopedic implants with a polycaprolactone polymer coating containing bone morphogenetic protein-2 on osseointegration in bones of sheep. Am J Vet Res. 2009, 70: 1416-1425. 10.2460/ajvr.70.11.1416.View ArticleGoogle Scholar
- Banks W: Applied Veterinary Histology. 1981, Baltimore, MD: Williams and Wilkins, 1Google Scholar
- Behari J: Biophysical bone behavior principles and applications. 2009, Singapore: WileyView ArticleGoogle Scholar
- Price RL, Haberstroh KM, Webster TJ: Improved osteoblast viability in the presence of smaller nanometre dimensioned carbon fibres. Nanotechnology. 2004, 15: 892-900. 10.1088/0957-4484/15/8/004.View ArticleGoogle Scholar
- McIlroy DN, Alkhateeb A, Zhang D, Aston DE, Marcy AC, Norton MG: Nanospring formation--unexpected catalyst mediated growth. J Phys: Condens Matter. 2004, 16: R415-R440. 10.1088/0953-8984/16/12/R02.Google Scholar
- Wang L, Major D, Paga P, Zhang D, Norton MG, Mcllroy DN: High yield synthesis and lithography of silica-based nanospring mats. Nanotechnology. 2006, 17: S298-S303. 10.1088/0957-4484/17/11/S12.View ArticleGoogle Scholar
- Schilke KF, Wilson KL, Cantrell T, Corti G, Mcllroy DN, Kelly C: A novel enzymatic microreactor with Aspergillus oryzae β-galactosidase immobilized on silicon dioxide nanosprings. Biotechnology Progress. 2010, 26: 1597-1605. 10.1002/btpr.476.View ArticleGoogle Scholar
- Timalsina YP, Oriero D, Cantrell T, Prakash T, Branen J, Aston DE, Noren K, Nagler JJ, Rastogi S, Mcllroy DN, Corti G: Characterization of a vertically aligned silica nanospring-based sensor by alternating current impedance spectroscopy. J Micromech Microeng. 2010, 20: 095005-10.1088/0960-1317/20/9/095005.View ArticleGoogle Scholar
- Beaux MF, Wang L, Zhang D, Gangadean D, Mcllroy DN, Kwon NH, Dziewanowska K, Bohach GA: Fibronectin Bonding to Nanowires and Their Internalization by Epithelial Cells. Journal of Biomedical Nanotechnology. 2006, 2: 23-28. 10.1166/jbn.2006.001.View ArticleGoogle Scholar
- Balasundaram G, Webster TJ: Nanotechnology and biomaterials for orthopedic medical applications. Nanomedicine (Lond). 2006, 1: 169-176. 10.2217/174358126.96.36.199.View ArticleGoogle Scholar
- Coelho MJ, Cabral AT, Fernande MH: Human bone cell cultures in biocompatibility testing. Part I: osteoblastic differentiation of serially passaged human bone marrow cells cultured in alpha-MEM and in DMEM. Biomaterials. 2000, 21: 1087-1094. 10.1016/S0142-9612(99)00284-7.View ArticleGoogle Scholar
- Norowski PA, Bumgardner JD: Biomaterial and antibiotic strategies for peri-implantitis: a review. J Biomed Mater Res Part B Appl Biomater. 2009, 88: 530-543.View ArticleGoogle Scholar
- Brauer DS, Gentleman E, Farrar DF, Stevens MM, Hill RG: Benefits and drawbacks of zinc in glass ionomer bone cements. Biomedical Materials. 2011, 6: 045007-10.1088/1748-6041/6/4/045007.View ArticleGoogle Scholar
- Stewart AK, Magee AC: Effect of zinc toxicity on calcium, phosphorus and magnesium metabolism of young rats. The Journal of Nutrition. 1964, 82: 287-295.Google Scholar
- Cicero G, Grossman JC, Catellani A, Galli G: Water at a hydrophilic solid surface probed by ab initio molecular dynamics: inhomogeneous thin layers of dense fluid. J Am Chem Soc. 2005, 127: 6830-6835. 10.1021/ja042963u.View ArticleGoogle Scholar
- Zhang Z, Ross RD, Roeder RK: Preparation of functionalized gold nanoparticles as a targeted X-ray contrast agent for damaged bone tissue. Nanoscale. 2010, 2: 582-10.1039/b9nr00317g.View ArticleGoogle Scholar
- Hoefling M, Monti S, Corni S, Gottschalk KE: Interaction of β-sheet folds with a gold surface. PLoS ONE. 2011, 6: e20925-10.1371/journal.pone.0020925.View ArticleGoogle Scholar
- Schmidt M: X-ray photoelectron spectroscopy studies on adsorption of amino acids from aqueous solutions onto oxidised titanium surfaces. Arch Orthop Trauma Surg. 2001, 121: 403-410. 10.1007/s004020100262.View ArticleGoogle Scholar
- Talwar A, James J, Arun K, Thangakumaran S, Sudarsan S: Osteoblast response (initial adhesion and alkaline phosphatase activity) following exposure to a barrier membrane/enamel matrix derivative combination. Indian Journal of Dental Research. 2009, 20: 7-10.4103/0970-9290.49048.View ArticleGoogle Scholar
- Collazos-Castro JE, Cruz AM, Carballo-Vila Mã, Lira-CantÃ Mã, Abad L, del Pino, Fraxedas J, San Juan A, Fonseca C, PÃgo AP, CasaÃ-Pastor N: Neural cell growth on TiO2 anatase nanostructured surfaces. Thin Solid Films. 2009, 518: 160-170. 10.1016/j.tsf.2009.06.048.View ArticleGoogle Scholar
- Boskey AL, Wright TM, Blank RD: Collagen and Bone Strength. Journal of Bone and Mineral Research. 1999, 14: 330-335. 10.1359/jbmr.19188.8.131.520.View ArticleGoogle Scholar
- Wang Y-H, Liu Y, Maye P, Rowe DW: Examination of Mineralized Nodule Formation in Living Osteoblastic Cultures Using Fluorescent Dyes. Biotechnol Prog. 2006, 22: 1697-1701.View ArticleGoogle Scholar
- Kourkoumelis N, Tzaphlidou M: Spectroscopic assessment of normal cortical bone: differences in relation to bone site and sex. Scientific World Journal. 2010, 10: 402-412.View ArticleGoogle Scholar
- Clarke B: Normal Bone Anatomy and Physiology. Clinical Journal Of The American Society Of Nephrology. 2008, 3: S131-S139. 10.2215/CJN.04151206.View ArticleGoogle Scholar
- LaLonde AD, Norton MG, Zhang D, Gangadean D, Alkhateeb A, Padmanabhan R, Mcllroy DN: Controlled growth of gold nanoparticles on silica nanowires. Journal of Materials Research. 2005, 20: 3021-3027. 10.1557/JMR.2005.0368.View ArticleGoogle Scholar
- Hall B: Bone Volume 1: The Osteoblast and Osteocyte. 1990, New Jersey: Telford Press, 1: 1Google Scholar
- Callister W: Materials Science and Engineering An Introduction. 2007, York, PA: Wiley, 7Google Scholar
- Yang Y, Ong J, Bessho K: Plasma-Sprayed Hydroxyapatite-Coated and Plasma-Sprayed Titanium Coated Implantas. Biomaterials in Orthopedics. 2004, New York: Marcel Dekker Inc.Google Scholar
- Markowitz K, Moynihan M, Liu M, Kim S: Biologic properties of eugenol and zinc oxide-eugenol. A clinically oriented review. Oral Surg Oral Med Oral Pathol. 1992, 73: 729-737. 10.1016/0030-4220(92)90020-Q.View ArticleGoogle Scholar
- George SM, Ott AW, Klaus JW: Surface Chemistry for Atomic Layer Growth. J Phys Chem. 2011, 100: 13121-13131.View ArticleGoogle Scholar
- Elam JW, George SM: Growth of ZnO/Al2O3 Alloy Films Using Atomic Layer Deposition Techniques. Chem Mater. 2011, 15: 1020-1028.View ArticleGoogle Scholar
- Elam JW, Groner MD, George SM: Viscous flow reactor with quartz crystal microbalance for thin film growth by atomic layer deposition. Review of Scientific Instruments. 2002, 73: 2981-10.1063/1.1490410.View ArticleGoogle Scholar
- Guziewica E, Godlewski M, Krajewski T, Wachnicki L, Luka G, Paszkowica W, Domagala J, Przezdziecka E, Lusakowska E, Witkowski B: ZnO by ALD- Advantages of the Material Grown at Low Temperature. ACTA Physica Polonica a. 2009, 116: 814-818.Google Scholar
- Stadtländer C: Scanning electron microscopy and transmission electron microscopy of mollicutes: challenges and opportunities. Modern Research and Educational Topics in Microscopy. 2007, 1: 122-131.Google Scholar
This article is published under license to BioMed Central Ltd. This is an Open Access article distributed under the terms of the Creative Commons Attribution License (http://creativecommons.org/licenses/by/2.0), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.