tio2 nanotube surfaces: 15 nm—an optimal length scale of surface topography for cell adhesion and...
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Stem cells
TiO2 Nanotube Surfaces: 15 nm—An Optimal LengthScale of Surface Topography for Cell Adhesion andDifferentiation**
Jung Park, Sebastian Bauer, Karl Andreas Schlegel, Friedrich W. Neukam,
Klaus von der Mark, and Patrik Schmuki*
Studies of biomimetic surfaces in medicine and biomaterial
fields have explored extensively how the micrometer-scale
topography of a surface controls cell behavior, but only
recently has the nanoscale environment received attention as a
critical factor for cell behavior. Several investigations of cell
interactions have been performed using surface protrusion
topographies at the nanoscale; such topographies are typically
based on polymer demixing, ordered gold cluster arrays, or
islands of adhesive ligands at distinct length scales.[1–3] Recent
work has indicated that the fabrication of ordered TiO2
nanotube layers with controlled diameters can be achieved by
anodization of titanium in adequate electrolytes.[4–6] Such
surfaces can almost ideally be used as nanoscale spacing
models for size-dependent cellular response. This is particu-
larly important as these studies are carried out on titanium
surfaces—a material used for clinical titanium implantations
for the purpose of bone, joint, or tooth replacements.
Therefore, principles elucidated from this work can guide
implant surface modifications toward an optimized surface
geometry and profile to best fit and cell interactions for
adequate bone growth.[7,8]
[�] Prof. P. Schmuki, S. Bauer
Department of Materials Science,
Institute for Surface Science and Corrosion (LKO)
University of Erlangen-Nuremberg,
Martensstrasse 7, 91058 Erlangen (Germany)
E-mail: [email protected]
Dr. J. Park, Prof. K. von der Mark
Department of Experimental Medicine I,
Nikolaus-Fiebiger-Center of Molecular Medicine
Friedrich-Alexander-University of Erlangen-Nuremberg,
91054 Erlangen (Germany)
Dr. K. A. Schlegel, Prof. F. W. Neukam
Oral and Maxillofacial Surgery
Friedrich-Alexander-University of Erlangen-Nuremberg,
91054 Erlangen (Germany)
[��] J. P. and S. B. contributed equally to the presented work. Wegratefully thank Mrs. Friedrich for SEM investigations, the Depart-ment of Materials Science, and Mrs. Rummelt, Eye-Hospital,University of Erlangen-Nuremberg. This work was supported bythe Deutsche Forschungsgemeinschaft (SCHM1597/9-1 andMA534/20-1).
: Supporting Information is available on the WWW under http://www.small-journal.com or from the author.
DOI: 10.1002/smll.200801476
� 2009 Wiley-VCH Verl
Previously we showed that vitality, proliferation, and
motility of mesenchymal stem cells (MSCs) and their differ-
entiation to bone-forming cells is critically influenced by
nanoscale TiO2 surface topography with a specific response to
nanotubes with diameters between 15 and 100nm.[9,10] We
demonstrated that adhesion, proliferation, migration, and
differentiation of MSCs was maximally induced on 15-nm
nanotubes, but prevented on 100-nm nanotubes, which induced
cell death. It remained unclear, however, whether this high
sensitivity of cell response—detecting minute differences of
pore size from15nmup to100nm—isa specificphenomenonof
stem cells or reflects a universal cell behavior. Therefore, in the
present work, we explore the nanoscale response of two main
bone cells: osteoblasts and osteoclasts.
Formaintaining bone homeostasis, the balance between the
bone-forming activity of osteoblasts and the bone-resorbing
activity of osteoclasts is finely regulated by a complex
mechanism involving paracrine and autocrine signals as well
as cellular interactions between these cells and their extra-
cellular matrix. Osteoclasts are originally derived from
hematopoietic stem cells (HSCs) capable of differentiating into
monocytes/macrophages and activated monocytes/macro-
phages, while osteoblasts are derived from mesenchymal
stem/progenitor cells.[11–16] Their differentiation canbe induced
by cytokines such as m-CSF (macrophage colony-stimulating
factor) and by interaction with osteoblasts through the RANK/
RANKL (receptor activator of nuclear factor-kB ligand)
system. Bone-resorbing cells play an important role not only
for daily bone remodeling but also for bone regeneration as
occurring in osseous integration of implant materials.[17,18]
Therefore, we address here the interaction of osteoclasts
with TiO2 nanoscale environments in order to explore i) if the
nanotopography of cell interactions as observed previously
with MSCs[10] is of a universal nature, and ii) if the balance
between bone-forming and bone-resorbing cells can be
affected by nanoscale topography. We show that the cell
response is sensitive to nanoscale surface topography in bone-
forming/resorbing cells as well as stem cells. Our present data
show that this nanoscale surface topography largely affects
bone cell differentiations involving osteoclastic activation and
bone-forming activity, indicating that 15 nm is a universal
geometric constant of surface-topography-supporting cell
adhesion and differentiation.
For this study we used surfaces of vertically aligned TiO2
nanotubes with six different diameters between 15 and 100 nm
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as described previously.[9,10] Synthesis of these self-assembled
TiO2 nanotube layers on titanium in a highly regular
arrangement was achieved by anodizing Ti sheets in a
phosphate-fluoride electrolyte at different voltages ranging
from 1 to 20V, thus precisely controlling tube diameter[9,19]
(Figure 1). On these surfaces we seeded HSCs from human
umbilical cord blood and induced differentiation into multi-
nucleated osteoclast-like cells using standard m-CSF and
RANKL procedures.
As shown in Figure 2, the response of freshly isolated
HSCs from human umbilical cord blood with respect to
differentiation to multinucleated osteoclasts showed the same
size-dependent response to TiO2 nanotubes as described
previously for osteoblastic differentiation,[10] that is, a highly
distinct reaction to the nanoscale spacing distance below
100 nm. On nanotubes below 30 nm differentiation to multi-
nucleated (Figure 2a) and tartrate-resistant acid phosphatase
(TRAP)-positive (Figure 2b) osteoclasts was significantly
stimulated compared to smooth TiO2 surfaces. In contrast,
osteoclast differentiation was severely inhibited on larger pore
sized nanotubes (Figure 2a–c). Differentiation of HSCs
(Figure 2c, left panel) to osteoclasts on 15-nm nanotubes
was evident by the appearance of large, multinucleated cells
(Figure 2c, middle panel, and 2d), which were not observed on
100-nm nanotubes (Figure 2c, right panel). Furthermore,
under the fluorescence microscope, differentiated osteoclasts
on 15-nm nanotubes showed a typical cortical actin ring
(arrows in Figure 2d, left upper panel) commonly observed in
active osteoclasts, and also showed more clearly enhanced
aVb3-integrin expression on 15-nm TiO2 nanotubes as
compared to 100-nm nanotubes (Figure 2d, lower panel).
Scanning electron microscopy (SEM) (Figure 2e) revealed the
Figure 1. Top-view SEM images of self-assembled layers of vertically
oriented TiO2 nanotubes of six different diameters ranging between 15
and 100nm formed in 1 M H3PO4þ0.3 wt% HF at potentials between 1
and 20V for 1 h. Scale bars: 200 nm.
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protrusion of extensive filipodia on 15-nm but not on 100-nm
nanotubes, confirming that HSCs can be actively stimulated to
differentiate into bone-resorbing cells on a TiO2 nanoporous
surface microenvironment with a diameter less than 30 nm.
In bone marrow and circulating blood, activated mono-
cytes/macrophages as well as HSCs are also sources for
osteoclast differentiation. Using blood monocytes we con-
firmed that not only stem cells but also activated monocytes/
macrophages can be induced to osteoclast differentiation
depending on the nanotube diameter (see Supporting
Information, Figure S1).
The possibility existed that the insufficient response of
HSCs to 100-nm nanotubes was due to cellular degeneration
or irreversible loss of differentiation capacity. In Figure 2f we
show, however, that HSCs retain their osteoclastic differ-
entiation potential even though they failed to differentiate into
osteoclasts on 100-nm nanotubes. By harvesting cells from
100-nm nanotubes after culture and replating on tissue culture
dishes, cells differentiated into multinucleated osteoclasts
(OCLs) within 10 days (Figure 2f, left panel). These cells were
TRAP-positive (Figure 2f, middle panel) and showed
osteoclastic resorption pits on bone disks (Figure 2f, right
panel). These findings indicate that osteoclastic differentiation
on large nanoporous structures is only temporarily impaired
on 100-nm nanotubes, but reversible by changing the
nanoscale microenvironment.
These findings show that—apart from this reversible
differentiation block of HSCs on 100-nm nanotubes—the
size-dependent response of HSCs to TiO2 nanotubes with
respect to osteoclast differentiation is very similar to the cellular
response ofMSCs reported previously.[10] MSCs did not spread
properly on nanotube surfaces of pore size larger than 30nm,
and showed unstable filopodia extensions.[10] Further motility
was reduced as shown in a gap-filling cell migration experiment
(see Supporting Information, Figure S2). Interestingly, HSCs
also showedreducedmotilityon100-nmnanotubesas compared
to 15-nm nanotubes as visualized by video microscopy (see
Supporting Information, Movies S1 and S2).
These findings imply that the nanoscale spacing of 15 nm,
which corresponds approximately the diameter of an intergrin
extracellular domain,[10] may represent a universal spacing
constant supporting a maximum of cellular responses to
surfaces. In order to investigate whether differentiation of
osteoblasts (a cell of mesenchymal origin in contrast to the
hematopoietic origin of osteoclasts) also follows a similar size
response to TiO2 nanotubes, we plated primary human
osteoblast-like cells (hOBs) from human iliac bone marrow
on six different sizes of nanotubes and on smooth TiO2
surfaces as a control. As shown in Figure 3, cell proliferation of
hOBs was again highest on 15-nm nanotubes (Figure 3a).
Similar to MSCs,[10] immunofluorescence analysis of hOBs
with antibodies to paxillin and fibronectin indicated a strongly
enhanced formation of focal contacts and a remarkably
stronger deposition of fibronectin fibers on the cell surface on
15-nm nanotubes as compared to 100-nm nanotubes
(Figure 3b). SEM revealed that cells spread out normally
on smaller size nanotubes (15 nm), forming lamellopodia and
wide, thick filopodia, while cell adhesion and spreading was
impaired without stable extension of filopodia on 100-nm
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Figure 2. HSCs can be actively differentiated to multinucleated osteoclasts on nanotubes of
diameter less than 30nm. a) Osteoclast differentiation measured by counting multinucleated
cells; the 100nm value was set as 1. b) Enzymatic assay for TRAP. c) Cell morphology reveals
large osteoclasts only on 15-nm nanotubes. Scale bars: 50, 200, and 200mm. d) Immu-
nofluorescence staining reveals the typical ring of actin cortex (arrows, left upper panel)
shown only in active osteoclasts on 15-nm nanotubes, and enhanced aVb3-integrin
expression on 15-nm nanotubes (lower panels). Scale bars: 100mm. e) SEM analysis of
filopodia formation. Scale bars: 3mm. f) Replating of HSCs that had remained undifferen-
tiated after 10 days on 100-nm nanotube surfaces retained their ability to differentiate toward
bone-resorbing cells on conventional culture dishes. Scale bars: 200, 50, and 50mm.
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nanotubes (Figure 3b). Mineralization of hOBs as measured
by Alizarin red staining (Figure 4a) and expression of
osteogenic marker proteins such as osteocalcin (Figure 4b)
also reaches a maximum on 15-nm nanotubes as compared to
larger size nanotubes or smooth surfaces. Interestingly,
osteogenic differentiation including mineralization was not
hampered by coculture with osteoclasts on 15-nm nanotubes,
while mineralization was not stimulated in coculture on 100-
nm nanotubes (Figure 4c–e). This indicates that bone cell
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differentiation was largely controlled by the
nanoscale microenvironment even under
the influence through the interaction
between osteoblast and osteoclast via
cell–cell contacts and soluble factors from
each cell type during coculture in vitro.
For both cell types of MSCs and hOBs,
differentiation was severely impaired on
tube diameters larger than 70nm, and cell
proliferation and migration were dramati-
cally reduced, indicating that bone-forming
cells and their progenitor cells have less
osteogenic differentiation potential in that
range of nanoscale spacing. These findings
confirm that both cell types of MSCs and
hOBs react similarly to lateral nanospacing.
This result is consistent with a previous
report on (RGDfK)-coated cell-adhesive
gold nanodots spotted in distinct spacings
of 28, 58, 73, and 85nmdistance, usingblock-
copolymer micelle nanolithography.[20] In
that study a separation of >73nm between
dots resulted in limited cell attachment and
spreading. Our findings support recent
reports on cells reacting sensitively to
nanoscale roughness on silicon or silica
substrates,[21,22] indicating that cell res-
ponses to biomimetic surfaces do not only
depend on the chemistry of the biomaterial
but also on the geometry of the nanoscale
microenvironment. Cell interactions with
extracellular surfaces are mediated by clus-
tering of integrins into focal adhesion
complexes and activation of intracellular
signaling cascades into thenucleus and to the
cytoskeleton.[23] The results presented here
are consistent with our hypothesis that a
spacing of 15–30 nm may be a result of
compact clustering of integrin receptor
molecules with an actual size of the extra-
cellular domain of about 10 nm into focal
contacts by the 15nm spacing of the
nanotubes.[10,24] This may explain why focal
contact formation, cell proliferation, migra-
tion, and differentiation occur at a higher
rate on 15-nm nanotubes than on polished
TiO2 or non-nanoporous surfaces. The
almost identical response of MSCs, HSCs,
andosteoclasts to the15-nmspacing suggests
that this nanoscale spacing may be a
universal scaffold for several cell types, or at least for bone-
remodeling-associated cells.
Bone marrow and surrounding bone are the major
supports for dental implants and total hip replacement
implants.[25] The maintenance of an appropriate balance of
bone resorption and bone remodeling during and after wound
healing, as well as stable integration of the implants have been
a long-standing challenge in the biomaterial implantology
field. Two rather different counteracting cell types of different
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Figure 3. Size-dependent response of primary human osteoblasts to
TiO2 nanotubes. a) Cell proliferation measured by cell counting (100 nm
values were set as 1). b) SEM images show that development of focal
contacts measured by paxillin staining (upper panel) (scale bars:
100mm), extracellular deposition of fibronectin matrix (middle panel)
(scale bars: 50mm), and filopodia formation (lower panel), were highest
on 15 nm nanotubes (scale bars: 10mm).
origin, osteoblasts and osteoclasts, are responsible for the bone
healing process. In most aspects, osteoblasts and osteoclasts
behave different in vitro and in vivo and underlie different
regulatory mechanisms. Thus, the present findings that the
activities of both bone-forming cells and bone-resorbing cells
on biomimetic surfaces responded almost identically to the
same spacing topography within a narrow range between 15
and 100 nm are quite surprising. Since MSCs also showed the
same size-dependence in their responses to TiO2 nanotubes,
we propose that a surface geometry with a lateral spacing of
approximately 15 nm that corresponds to the dimension of
integrin heads will be preferentially recognized by many more
(at least bone remodeling cells (osteoblast/osteoclast) as well
as MSCs) if not all cell types. Although several facts, such as
the formation of focal contacts, the induction of paxillin,
phosphorylation, and the formation of stress fibers, indicate
the key role of the integrin cluster size in the recognition of
nanoscale surface topography, further work is needed to
ultimately confirm this point. It is, however, noteworthy that
our pilot in vivo experiments also have shown that bone
regeneration on Ti implants with 30-nm nanotubes are
small 2009, 5, No. 6, 666–671 � 2009 Wiley-VCH Verlag Gmb
significantly different from that on rough Ti implants.[26] It
is still elusive how the balance between osteoblastic and
osteoclastic activity can be modulated by controlling the
surface geometry. However, this implies a general change in
our concepts in the design of nanoscale surfaces and
biomaterials used for implantation and other biotechnology
developments.
Experimental Section
Nanotube formation: Titanium foils (99.6% purity, Advent Ltd.)
were used for producing nanoporous surfaces. Coatings consisting
of highly ordered self-assembled TiO2 nanotubes of different
diameters were applied on the foils using an electrochemical cell
with a three-electrode configuration. Platinum gauze served as
a counter electrode and a Haber–Luggin capillary with a Ag/AgCl
(1 M KCl) electrode was used as a reference electrode. Electro-
chemical treatments were carried out according to previous
reported work[9] in 1 M H3PO4 (Merck) with addition of 0.3wt%
HF (Merck) with applied potentials from 1V up to 20 V for 1 h at
room temperature. For smooth, polished surfaces, titanium sheets
(99.99% purity, Alfa Aesar) were mechanically ground, lapped,
and finally polished (New Lam System) followed by anodization in
fluoride free 1 M H3PO4 at 20 V. All electrolytes were prepared from
reagent grade chemicals and deionized water. The samples were
sterilized using an autoclave at 121 8C prior to cell seeding. High
resolution X-ray diffraction (XRD) of the nanotube layers after
autoclaving showed the tubes to be of an amorphous nature. X-ray
photoelectron spectroscopy (XPS) investigations of the tubes
revealed the composition to be approximately 58 at% Ti, 37 at%
O, and 5 at% F prior to the wash with distilled water.[6] For
morphological characterization of sample surfaces, a field
emission SEM (FESEM, S-4800, Hitachi) was used.
Cell culture: For the isolation of HSCs and mononuclear cells
(MNCs), fresh umbilical cord blood samples were collected from
healthy, full-term placentas. The MNC fraction was isolated by
density gradient centrifugation using Ficoll-Paque Plus (Amersham
Biosciences) according to the manufacturer’s protocol. CD133(þ)
cells were obtained by incubating the cells with an anti-CD133-
phycoerythrin antibody (Miltenyi Biotech) followed by separation
on a high-performance flow cytometry cell sorter (MoFlo, DAKO)
with forward-side scatter gating. The resulting fraction of
CD133(þ) cells was sorted again to increase its purity to >98%.
Primary human osteoblast-like cells were isolated from
remaining bone chips of iliac bone marrow obtained after
autologous bone graft with patient consent. After two passages
of primary cell culture with alpha medium (Invitrogen) containing
10% fetal calf serum (FCS), cells were harvested at their
confluency and stored frozen until usage. Rat MSCs were isolated
and expanded from fresh bone marrow from femurs of 4-week-old
wistar rats. Selected clonal cells were further expanded as
described previously.[10,27] For migration assay the cells were
infected with retroviruses containing a green fluorescence protein
(GFP) cDNA. For all studies, stably GFP-expressing cell clones were
used.
For osteoclastic differentiation, HSCs at a cell density of
10 000 cm�2 or MNCs at a cell density of 500 000 cm�2 were
cultivated on 15- and 100-nm nanotubes in alpha medium
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Figure 4. a) Mineralization (alizarin red staining) and osteogenic differentiation measured by
osteocalcin expression (b) of primary osteoblasts was highest on 15-nm tube diameters, but
severely impaired on nanotubes with diameters larger than 70-nm. Scale bars: 100mm. c,d)
Mineralization assay of a 2-week coculture (c) and of primary osteoblasts and osteoclasts (d),
showing that overall mineralization in spite of osteoclast differentiation was much enhanced
on 15-nm nanotubes compared to 100-nm nanotubes. d) Alizarin red staining showing
mineralization was consistent with quantitative analysis of mineralization in (c), confirming
that the activity of osteoblastic differentiation dramatically was stimulated on 15-nm
nanotubes. Scale bar: 1 cm. Osteoblastic differentiation in cocultures on 15-nm nanotubes
was further supported by immunofluorescence staining for e) osteocalcin at a similar level as
osteoblasts in the absence of osteoclasts (b). Osteocalcin in red, nuclear stain in blue, scale
bars: 400 and 100mm.
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containing 10% FCS, 50 ng mL�1 human recombinant RANKL, and
20 ng mL�1 m-CSF. The culture medium was replaced every 2 days
in all experiments.
For osteogenic differentiation cells were plated at a cell
density of 50 000 cm�2 in alpha medium (Invitrogen) containing
10% FCS. Five days after cell plating, the culture medium was
changed into a differentiation medium containing 10% FCS,
dexamethasone (100 nM), b-glycerophosphate (10mM), and as-
corbic acid (50mg mL�1). The cells were cultivated for 2 weeks
with differentiation medium and analyzed by immunocytochem-
istry and quantitative mineralization assay.
For the coculture experiment, human primary osteoblasts at a
cell density of 50000 cm�2 and primary MNCs at a cell density of
500000 cm�2 were plated on 15- and 100-nm nanotubes in alpha
medium containing 10% FCS, 50 ng mL�1 human recombinant
RANKL, and 20ng mL�1 m-CSF. From the 5th day of coculture, the
cocultured cells were stimulated for osteoblastic/osteoclastic
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differentiation using differentiation medium
containing dexamethasone (100nM), b-glycer-
ophosphate (10mM), ascorbic acid (50mg
mL�1), 50ng mL�1 human recombinant RANKL,
20ngmL�1m-CSF, and 10% FCS. The cells were
cultivated further for 2 weeks with differentia-
tion medium and analyzed by immunocyto-
chemistry and quantitative mineralization
assay.
TRAP staining and solution assays: To
analyze osteoclastic differentiation, HSCs or
MNCs were cultivated on nanotubes in differ-
entiation medium, and fixed and immunos-
tained after 10 days with 40,6-diamidino-2-
phenylindole (DAPI) and phalloidin as de-
scribed previously.[12] Multinucleated cells
containing more than three nuclei were
considered differentiated osteoclast-like cells,
and 100–300 cells in at least three fields were
counted under the fluorescence microscope
(Zeiss Axiophot).
To quantify TRAP activity, cells after 10 days
culture in differentiation medium were washed
once with phosphate buffer saline (PBS) and
lyzed in 80mL of cold lysis buffer (90mM citrate
buffer, pH 4.8, 0.1% Triton X-100 containing
80mM sodium tartrate) for 10min. After lysis,
80mL of substrate solution (20mM p-nitrophe-
nyl phosphate in the above lysis buffer) was
added and incubated for an additional 3–
5min, and the reaction was stopped by adding
40mL of 0.5 M NaOH. The optical density was
read at a 405-nm wavelength.
To verify the differentiation potential of
HSCs on TiO2 nanotubes, cultivated HSCs on
100-nm tubes were trypsinized and replated on
24-well plastic culture plates for TRAP staining
or BD BioCoatTM OsteologicTM disks for osteo-
clastic resorption tests. Replated cells were
cultivated with the same differentiation med-
ium. Then cells were washed once with PBS and
fixed in 10% formalin for 10min. After washing with PBS, cells were
permeabilized with 0.1% Triton X-100 for 1min, washed once with
PBS, and incubated with substrate solution napthol AS-BI phos-
phate (Sigma) in the presence of 50mM sodium tartrate at 37 8C for
10min. Resulting red-stained TRAP activity Osteoclast resorption
pits were visualized by light microscopy.
Detection and quantification of mineralization: For detection of
mineralization, alizarin red staining was performed on three
samples each with 15- and 100-nm nanotubes after 2week
differentiation culture as previously described.[28] Briefly, cocul-
tured cells were fixed in 4% paraformaldehyde (PFA) and treated
with 40mM alizarin red S (pH 4.1, Sigma) for 20min at room
temperature with gentle shaking. After aspiration of the unin-
corporated dye, the samples were washed four times with d-H2O
while shaking for 5min. Stained mineralized nodules were
visualized. For quantification of staining, 10% v/v acetic acid
was added to each sample and incubated for 30min with shaking.
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The monolayer on nanotubes was then scraped from the sample
surfaces with 10% v/v acetic acid and transferred to a
microcentrifuge tube. After vortexing for 30 s, the tube was
heated to 85 8C for 10min and centrifuged at 20 000 � g for
15min. The supernatant was transferred to a new microcentrifuge
tube and 10% v/v ammonium hydroxide was added to neutralize
the acid. Aliquots of the supernatant were read in triplicate at
405 nm in a 96-well format enzyme-linked immunosorbent assay
(ELISA) reader.
Immunocytochemistry: For immunocytochemistry, cells grown
on nanotubes were rinsed in PBS and fixed with 2% PFA in PBS at
room temperature for 10min. After fixation, cells were permeabi-
lized with 0.2% Triton X-100 in PBS for 2min, washed with PBS,
and incubated with antibodies of mouse monoclonal anti-paxillin
(Signal Transduction), anti-aVb3-integrin (Chemicon), and mouse
monoclonal anti-osteocalcin (Takara) for 1 h. The F-actin was
visualized with Alexa488-labeled phalloidin (Biosource). Second-
ary antibodies labeled with Cy5 (Biosource) were used. Cell nuclei
were stained blue with DAPI (Roth). Cell images were taken using
an Axiophot 2000 ApoTome microscope with AxioCam digital
camera and AxioVision software (Zeiss).
For SEM observation cells were fixed with 2.5% glutaraldehyde
solution (Merck) overnight at 4 8C. Samples were rinsed in PBS
solution, dehydrated in a series of acetone solutions (60, 70, 80,
90, and 100%) and critical point dried with a Critical Point Dryer
(CPD 030, Balzers).
Cell proliferation and migration assay: Primary human
osteoblast-like cells and GFP-labeled MSCs were plated on a
titanium surface at a cell density of 5 000 cm�2. Cell proliferation
was analyzed by a cell count 3 days after cell plating. For cell
counting of primary osteoblast-like cells cell nuclei were stained
with DAPI before counting. Adherent cells were counted at three
different areas using 1280�1024 pixels resolution, where each
sample was depicted under a fluorescent microscope (50�magnification).
To analyze cell migration, GFP-labeled MSCs were plated at a
cell density of 50 000 cm�2 and 3 h later cells were removed in a
streak (3.4mm in width) in the center of the field. Thirty-six hours
later the immigration of cells into the cleft was analyzed using
Openlab software (Improvision).
To analyze HSC motility on different sizes of nanotubes, HSCs
were labeled using CM-DiI fluorescence cell tracker (Invitrogen)
before cell plating on nanotubes as previously described.[29] One
day after cell plating, cell migration of HSCs was monitored by
time-lapse video microscopy every 2min during 4 h and analyzed
using Openlab software.
Keywords:biomimetics . nanotubes . stem cells . surface topography .
titanium dioxide
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Received: October 6, 2008Revised: November 7, 2008Published online: February 20, 2009
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