chemical patterning in biointerface science
TRANSCRIPT
ISSN:1369 7021 © Elsevier Ltd 2010APRIL 2010 | VOLUME 13 | NUMBER 422
Chemical patterning in biointerface science
As society strives towards an improved quality of life, we care
for an ever increasing elderly population and attempt to combat
the increase in life-style associated health conditions, such as
diseases of the cardiovascular system. This drives researchers to
develop innovative biomaterials with new and improved surfaces.
In most cases the materials used to treat and diagnose disease
are in contact with biological fluids that contain proteins, which
spontaneously and irreversibly adsorb to surfaces. It is this surface
that cells contacting the material ‘see’, often triggering material
failure1-6. Cells respond to the biochemical signals contained
within the peptide motifs of the adsorbed proteins through extra
cellular matrix receptors such as integrins7. The consequences of
uncontrolled protein adsorption on man made surfaces can be
very severe indeed, resulting in not only device failure but also
additional health risks to patients8. Examples include:
1) attachment and colonisation of pathogenic bacteria to venous
catheters via adsorbed protein layers that can lead to high
patient mortality9;
2) thrombosis on the surfaces of cardiovascular devices such as
artificial hearts, catheters and prosthetic valves from platelet
adhesion and activation10;
3) fouling of hemodialysis membranes11; and
4) inflammatory responses that lead to restenosis following the
insertion of stents12.
On the other hand, the fields of tissue engineering13, biosensors
and diagnostic arrays14,15 and drug delivery systems16, which
Patterning of surfaces with different chemistries provides novel insights into how proteins, cells and tissues interact with materials. New materials, and the properties that their surfaces impart, are highly desirable for the next generation of implants, regenerative medicine and tissue engineering devices, and biosensors and drug delivery devices for disease diagnosis and treatment. Patterning is thus seen as a key technology driver for these materials. We provide an overview of state-of-the-art fabrication tools for creating chemical patterns over length scales ranging from millimeters to micrometers to nanometers. The importance of highly sensitive surface analytical tools in the development of new chemically patterned surfaces is highlighted.
Ryosuke Ogaki1, Morgan Alexander2, and Peter Kingshott1*1 The Polymer NanoInterfaces Group, Interdisciplinary Nanoscience Centre (iNANO), Faculty of Science, Aarhus University, 8000 Aarhus C,
Denmark.2 Laboratory of Biophysics and Surface Analysis, School of Pharmacy, The University of Nottingham, Nottingham, NG7 2RD, UK.
*E-mail: [email protected]
MT1304p22_35.indd 22 12/03/2010 14:58:12
Chemical patterning in biointerface science REVIEW
APRIL 2010 | VOLUME 13 | NUMBER 4 23
aim to regenerate, diagnose and treat diseased tissues, rely on
proteins and biomolecules being presented either to attach cells in
the aqueous environment in the correct conformation and spatial
configuration in 1, 2 and 3D to optimize bioactivity and minimize
adverse reactions.
The realization that interfacial phenomena were important
to biomaterials came after World War II when the concept of
‘biocompatibility’ emerged17. This lead to acceleration in the field of
surface and interface research targeted at biology and medicine. The
progress made has encouraged scientists and engineers to pursue
these goals further with the development of chemically patterned
surfaces with nanometer-scale precision, with a vision of ultimately
fabricating and controlling the biological system as desired through
the interface with the man made materials. The birth of a new
field, termed ‘nanobiotechnology’ arose, which utilizes biological
systems to fabricate functional nanostructured and mesoscopic
architectures comprised of organic and inorganic materials18. One of
the fundamental biological phenomena that has driven and continues
to underpin this field is the fact that cells respond to topographical and
chemical cues from their environment by interacting with extracellular
matrix (ECM) and other cells in vivo, and mechanical and chemical
properties of material-surface interface in vitro. The subsequent cell
signaling events ultimately influences cell function, shape, migration,
adhesion, survival, proliferation and differentiation19-24.
To understand the complex relationship between the surface
chemistry and biological systems, there has been a focus on combining
topographical and chemical modification to create multi-functional
surfaces. Highly defined topographical and chemical features from the
mm to nm range are intended to span the length scales of tissues to
cells to proteins and other biomolecules – these synthetic ‘models’ of
biology will allow us to rationally study and comprehend the complex
interfacial behavior possessed by the biological system in 2- and 3D.
The ability to mimic biological surfaces permits us to unravel the
essential controlling factors in biology by studying the interaction
between the mimicked surface and biological components.
Early developments of surface fabrication were inspired by the
‘top down’ approaches, traditionally used in microelectronics such as
photolithography and electron beam (e-beam) lithography25-27 for
devices such as microprocessors28, MEMS29 and NEMS30. Typically
it is possible to obtain a surface topographical feature of down to
~10 nm with e-beam lithography. Techniques such as Transmission
Electron Beam Ablation Lithography (TEBAL)31 have been recently
developed in an attempt to conquer the challenge of reaching the
sub-10 nm resolution limit. TEBAL is carried out by controllably
ablating evaporated metal films, pre-patterned with e-beam
lithography on silicon nitride membrane substrates, to produce a
variety of intricate nano-features such as gaps, rings, channels and
wires. Many technological methods for surface fabrication have been
inspired by the techniques from the printing industry; for instance,
ink-jet technology has a number of potential life science applications
such as genomics, combinatorial chemistry, drug discovery and tissue
engineering32-34. Current jet printer technology has reached the limit
of printing high resolution features on a surface down to ~ 1 μm in a
parallel manner35.
Surfaces can be fabricated by ‘bottom up’ approaches, for example,
molecular self-assembly such as alkane thiols on gold is a commonly
used method to form well ordered surfaces. A range of surface
functionalities can be presented on the surface by introducing different
chemical terminal groups either as a single component or multiple
components36-40. Certain types of polymers such as block copolymers,
and particulate systems, can self assemble into a variety of nanoscopic
structures with topographical scales of 5 to 50 nm41-43. Examples of
how dimensions influence cellular behavior come from the Spatz group.
They have identified critical surface spacing ranges for the cell-adhesion
peptide sequence RGD, which influence the structure of integrin
receptors on cell surfaces. A spacing on 58 nm vs 108 nm showed
large variations in integrin mediated cell behaviour. On 58 nm RGD
patterns cell spreading was delayed and motility was erratic, whereas
on 108 nm patterns cell adhesion sites exhibited rapid turnover
indicating a critical RGD density was necessary for develop stable
integrins, and efficient cell spreading and focal adhesion formation44.
Furthermore, disordered patterns of > 70 nm cyclic RGD were found to
be necessary to ‘turn-on’ cell attachment compared to ordered 70 nm
patterns that ‘turned off’ attachment45. These nano dimensions have
been related to the size of the integrin structural elements indicating
that cell adhesion is sensitive to dimensions much smaller than the
size of an individual cell. Another emerging ‘bottom up’ fabrication
method is the implementation of micro and nanometer sized colloidal
particles known as ‘colloidal lithography’. Recent advances in colloidal
synthetic methods have enabled highly monodisperse particles to
be produced with good phase stability. Two dimensional structures
with lateral feature sizes in the range of micrometers to nanometers
can be readily assembled simply by selecting different sized particles.
By using colloidal patterns as masks, diverse topographical features
and geometrical control can be obtained; either directly by reactive
ion etching (RIE) on single and multi-layered colloidal surface46,47, or
by depositing various organic and inorganic materials on a substrate
surface through the interstitial spaces formed between the particles
via evaporation or sputtering followed by the subsequent removal
of particles48,49. A novel method ‘shadow nanosphere lithography’ is
capable of creating a range of topographical morphologies such as cups,
rods and wires in the nanometer size range on the surface by varying
the position and angle of the substrate with respect to the evaporation
source50,51. Various ‘bottom up’ and ‘top down’ fabrication methods
have been also employed in combination for surface patterning.
Non-photolithographic techniques including various soft lithography
methods52-56, dip pen nanolithography (DPN)57 and nanoimprint
lithography58 have been developed over the last two decades.
MT1304p22_35.indd 23 12/03/2010 14:58:14
REVIEW Chemical patterning in biointerface science
APRIL 2010 | VOLUME 13 | NUMBER 424
Spatially controlling the surface chemistry for selective adhesion of
proteins and cells, while resisting non-specific interactions in passive
surface regions, is essential. Surface scientists have been attempting
to create ‘non-fouling’ surfaces, as unwanted protein adhesion to
implanted devices can encourage bacterial colonization which can
pose serious medical complications to the patients. A significant level
of research has been carried out in order to identify and define the
physical and chemical criteria required by the surface for preventing
bioadhesion.
Since the surface constitutes so little material, and surfaces are
very prone to contamination, by virtue of their location, surface
modification must always be accompanied by surface analysis. The
advent of sophisticated, highly surface sensitive analytical instruments
has certainly aided the technological advancement in lithographical
processes and their applications in biology and medicine.
In this article, we first provide examples of several modern surface
analytical techniques commonly used to study biologically relevant
materials. We then highlight some of the current research, process
and associated limitations for developing non-fouling surfaces and
biological patterning. Current applications and potential uses of such
patterns in the areas of drug discovery, combinatorial chemistry,
regenerative medicine and tissue engineering are also succinctly
discussed. Finally a summary and outlook is given in the areas of
fabrication and surface characterization.
Surface characterization and analysisEmphasis on the technical capability of surface analytical instruments
used in biological surface science has moved from spectroscopic based
analysis of mainly large area samples to include routine spatially
resolved chemical state analysis within the last three decades. This
is driven by the demand for methods to prepare spatially well-
defined surfaces59. Commonly a suite of complementary techniques
is applied to derive a full characterization of complex surfaces. X-ray
photoelectron spectroscopy (XPS)60-62 and time-of-flight secondary
ion mass spectrometry (ToF-SIMS)61,63,64 are routinely used to
elucidate quantitative and qualitative surface chemical information
respectively. Both are sensitive to the uppermost surface and are
routinely capable of achieving spatial resolution in the range of 5 μm
– 50 nm for chemical imaging. XPS provides quantitative elemental
and chemical functional information from the first 10 nm of the
surface for all elements but hydrogen and helium but is limited in
lateral resolution to a few microns on ideal samples. In contrast,
SIMS has excellent spatial resolution and sensitivity but is not readily
quantified. It has been extensively utilized to chemically image a range
of biologically relevant systems at high lateral resolution, including
lipids65,66 with lateral resolution as low as 100 nm in model systems
and biological cells67-69 and tissues with lateral resolution of 200 nm
– 1 μm70-72. Fig. 1 provides an example of how ToF-SIMS is currently
being exploited and developed to study the lateral distribution of
different chemistries in biological tissue samples to differentiate tissue
regions through their chemistry and thereby study disease. Such
an ability to differentiate tissue regions is envisaged as vital for the
guided design of artificial materials for tissue engineered constructs,
for example.
Atomic force microscopy (AFM)73 is a topographical imaging
technique that belongs to the family of scanning probe microscopy
(SPM)74 with the capability of obtaining highly resolved images,
with routine spatial resolutions down to 2-3 nm75. Although AFM
is primarily used for obtaining topographical information, chemical
specific (i.e. between chemical functional groups)76,77 and bio-specific
Fig. 1 ToF-SIMS imaging of mouse embryo. (a) Optical image of a 16-day-old H&E stained mouse embryo section and positive total ion ToF-SIMS image of brain (b), liver (c), rib (d) and heart (e). The secondary ion images contain structural and chemical information capable of identifying different tissue sections. (Reprinted with permission from72).
(b)(a)
(c)
(d)
(e)
MT1304p22_35.indd 24 12/03/2010 14:58:15
Chemical patterning in biointerface science REVIEW
APRIL 2010 | VOLUME 13 | NUMBER 4 25
(e.g. antibody-antigen78,79, ligand-receptor80,81, DNA-DNA82, cell-
cell83) interactions between the tip and the substrate surface can be
studied by functionalizing the probe tip84. Tips can also be modified
with molecules such as carbon nanotubes to decrease the probe size in
order to increase image resolution with added functionality85. Recent
efforts in the development of AFM have lead to atomically resolved
image in non contact (NC) AFM mode with tips functionalized with
CO molecule in vacuum86.
Immobilization and measurement of interactions between proteins
and surfaces, and between cells and surfaces, can be monitored without
labeling and in real-time by using sensing instruments such as quartz
crystal microbalance (QCM)87,88 and surface plasmon resonance
(SPR)89,90. SPR is also capable of imaging surface interactions by
monitoring the refractive index with spatial resolution of 2 μm91,92.
The techniques provide complementary information with recent
examples of successful application including the determination of DNA
hybridization efficiencies in streptavidin-biotinylated DNA complexes93,
estrogen receptor-DNA complexes94, the detection of different Ebola
virus glycoprotein species using monoclonal and polyclonal antibodies95
and monitoring the interactions between various photo-immobilized
biomolecules and specifically bound antibodies96. There are numerous
other important surface analytical techniques that have made a
significant contribution to the life sciences, summarised in Fig. 297.
In addition to the techniques and references listed above, interested
readers should refer to the following references for further reading in
surface analysis techniques97-100.
Fig. 2 Flowchart of the various analytical methods available to the biomedical researcher and their respective analytical features (Adapted from97).
MT1304p22_35.indd 25 12/03/2010 14:58:20
REVIEW Chemical patterning in biointerface science
APRIL 2010 | VOLUME 13 | NUMBER 426
Recent developments in material surface patterning ‘Non-fouling’ surfacesMaterial surfaces that are resistant to bioadhesion have become an
essential platform for creating two dimensional selective patterning of
the biological components. The likelihood that a protein will adsorb to
a particular surface depends on numerous inter-relating physical and
chemical properties of the protein and the surface. So far, numerous
efforts have been made to unravel the relationships between surface
chemistry and protein adsorption. For instance, Whitesides et al.
employed a range of SAMs to produce model chemically functionalized
surfaces and studied the relationships between the surface chemistry
and protein adhesion. They found that surfaces that were hydrophilic,
and acted as hydrogen bond acceptors and were electrically neutral
properties resisted protein adsorption101,102. However, an exception
was observed by Mrksich’s group where the mannitol terminated SAMs
which contains a large number of hydrogen donors also resisted protein
adsorption103. Denis et al.104 has employed a combination of SAMs and
colloidal lithography to study the effect of both surface roughness and
chemistry on the adhesion of collagen. More recently, Roach et al.105
studied and noted the conformational changes and adsorption steps
of bovine serum albumin (BSA) and fibrinogen on hydrophilic and
hydrophobic SAMs by QCM and grazing angle infrared spectroscopy
(GA-FTIR).
For applications in biology and medicine, poly(ethylene glycol)
(PEG) and its derivatives continue to be the most promising materials
for creating ‘non-fouling’ surface due to their biocompatibility106.
Theoretical models have been put forward to understand the
effectiveness of PEG against protein and cell adhesion107-109.
Significant effort has been expended in an attempt to understand
the effect of the various oligoEG preparation conditions; grafting
density, molecular weight, chain conformation, hydration, ionic
strength, surface charge and temperature on the effectiveness of PEG
in resisting protein and bacterial adhesion110-119. From the theoretical
and experimental work, the graft density, molecular weight and
hydration have been found to be the most prominent factors in the
effectiveness of PEG to resist protein adsorption118. However the
detailed understanding of the exact parameters required for resisting
protein adsorption and cell adhesion in practice still remains complex
and unsolved, particularly for preventing bacterial adhesion in vitro and
bioadhesion in vivo. A variety of methodologies have been developed
for preparing PEG-modified surfaces. Examples of PEG modified
Fig. 3 The effect of spatially controlled surface modification on protein adhesion and cell growth. (a) Confocal laser scanning microscopy highlighting the preferential binding of collagen I on acetylaldehyde plasma polymer film (AAPP, left) over acetylaldehyde-allylamine plasma polymer film with covalently immobilized PEG (AAPP-ALAPP-PEG, right). (b) The direction of outgrowth on different surface chemistries from a central piece of bovine corneal tissue over an 8 day period. Unrestricted outgrowth on AAPP substrate (1), no outgrowth on AAPP-ALAPP-PEG substrate (2) and controlled outgrowth on chemically patterned substrate with central 13 mm diameter of AAPP and AAPP-ALAPP-PEG on the peripheral (3). (c) Histological analysis of the tissue outgrowth progression over 21 days cultures on chemically patterned substrate. The direction of the tissue migration is depicted as dashed arrows. (1) Migration of epithelial layer (ep) from the corneal disk (cd) onto the supportive AAPP substrate. (2) The central area of the cell supportive (cs) region (AAPP). (3) Boundary point (bp) between cell supportive and the non-supportive (ncs) region (AAPP-ALAPP-PEG) where a disorganized pile up of the cells can be seen behind the boundary point, restricting further migration. (Reprinted with permission from134).
(b)(a)
(c)
MT1304p22_35.indd 26 12/03/2010 14:58:25
Chemical patterning in biointerface science REVIEW
APRIL 2010 | VOLUME 13 | NUMBER 4 27
surfaces include PEG-like coatings via plasma polymerization120-122,
PEG grafting via ‘cloud point’112, co-polymer systems containing
PEG (e.g. poly-l-lysine-grafted-PEG (PLL-g-PEG)123,124, polysulfone-
grafted-PEG (PSf-g-PEG)125, polystyrene-block-PEG (PS-b-PEG)126),
development of poly(oligoethylene glycol methyl methacrylate)
(POEGMA) via atom transfer radical polymerization (ATRP)127,
multi-component cross linked PEG128,129, incorporation of EG to
self assembled monolayer130-132 and poly electrolyte multilayers133.
In recent work, George et al.126 demonstrated that PS-b-PEG block
co-polymer system can self assemble into various controllable
domain morphologies while retaining protein and cell resistance.
Thissen et al.134 used combination of cloud point grafting and plasma
polymerization and demonstrated the controlled deposition of ECM
protein collagen I and the growth of bovine corneal epithelial (BCEp)
tissue in two dimensions (Fig. 3). Multi-component cross linked PEG
has been developed as a single commercial formulation that can be
covalently attached to any substrates without the need of primers129.
Ma et al.135 has demonstrated the effect of surface density of POEGMA
towards the resistivity of fibronectin by controlling the number of ATRP
initiators presented by the mixed SAMs. These novel methodologies
and materials possess diverse physical and chemical characteristics
that facilitate the fabrication of non-fouling backgrounds on which to
accurately pattern biomolecules on surfaces.
Current strategies in biological surface patterningSite specific immobilization of proteins and peptides with nanometer
resolution is of fundamental importance for subsequent recognition
Fig. 4 Self-selective immobilizations of different proteins onto respective surface chemistries from a single mixed solution. (a) Binary protein patterning is carried via a photolithographic method to create a patterned surface contrast of biotin and chloroalkane onto hydrogel substrate. Subsequently this surface is exposed to the mixed solution of streptavidin and HaloTag proteins. (b) Fluorescent images of affinity ligand patterned hydrogel surface after 1 hour exposure to the fluorescently labeled protein conjugates with different excitation wavelengths (streptavidin – excitation/emission 532/557-592 nm, HaloTag – excitation/emission 635/650-690 nm). Methoxy terminated surface chemistry was included as a control. The three binary surface chemical patterns are biotin/methoxy (BM), methoxy/chloroalkane (MC) and biotin/chloroalkane (BC). (Reprinted with permission from139).
(b)
(a)
MT1304p22_35.indd 27 12/03/2010 14:58:27
REVIEW Chemical patterning in biointerface science
APRIL 2010 | VOLUME 13 | NUMBER 428
and adhesion of cells and organization of tissues. While a number of
methodologies have been developed and utilized for the patterning of
biological molecules, recent trends indicate that some techniques are
exploited more extensively, most likely due to limitations posed by
some processes. For example, we have observed significant decrease
in the implementation of photolithographic based techniques for
protein patterning. Although the major limitation associated with
spatial capability has recently been rectified by techniques such
as plasmonic nanolithography136 and scanning near field optical
microscopy (SNOM)137 to reach sub 100 nm resolution, high running
costs and need for a clean room is still a deterring factor. Despite
these limitations, a number of recent studies using photolithographical
techniques are worth mentioning. For instance, Carrico et al.138 has
utilized a recombinant photoreactive protein which exhibits certain
mechanical properties at a given wavelength and demonstrated
Rat-1 fibroblast patterning without the use of traditional chemical
modification that may compromise protein function. Dubey et al.
demonstrated the self-selective patterning of streptavidin and
HaloTag™ into adjacent regions of biotin and chloroalkane respectively
that were prepared onto a PEG based multicomponent hydrogel via
selective photolithographic patterning from the same solution. The
pattern was subsequently characterized by fluorescent microscopy and
ToF-SIMS139 (Fig. 4).
Micron scale protein and cell surface patterning has been
achieved two decades ago by Whitesides’ group using micro contact
printing (μCP)52,140,141 as an alternative method to overcome the
drawbacks associated with photolithographic based techniques and
the popularity of the method still remains today. In μCP, polymer
stamps with features are developed from a master fabricated from
a range of lithographical processes. The stamp is dipped in the ‘ink’
of protein solution and brought to contact with a substrate surface.
More recent development in the patterning process has focused
on utilizing a combination of fabrication techniques to produce
nanometer scale protein patterns on the surface in an extremely
parallel fashion. Nanometer scale contact printing (nano contact
printing, nCP) of single142 and multiple108 protein patterning has been
achieved by Delamache’s group (Fig. 5). A number of workers have
highlighted the contact transfer of hydrophobic oligomeric species
from the poly(dimethyl siloxane) (PDMS) stamp as a problem in
many applications143. Csucs et al. have published work illustrating the
utility of an alternative stamp material, polyolefin plastomer (POP),
with improved nanometer scale protein patterning144. To overcome
the issues associated with contact printing such as reproducibility
of the pattern over large areas and transfer contamination, Textor’s
group developed a technique called selective molecular assembly
patterning (SMAP)145. In SMAP, nanometer scale spatially resolved
contrast of hydrophilic (non-fouling) and hydrophobic (fouling) surface
can be created by immobilizing PLL-g-PEG and alkyl phosphates onto
silicon dioxide and titanium dioxide respectively. Nanometer scale
patterns can be created over large areas by combining processes such
as colloidal lithography, hot embossing and template synthesis145.
More recently the same group has demonstrated the improved SMAP
process by combining e-beam lithography into the process and the
incorporation of indium tin oxide into substrate, producing large scale
patterning of streptavidin146.
Another printing based technique is nanoimprint lithography (NIL)
and the first patterning of protein using this method was reported by
Hoff et al. in 200458. NIL typically employs a Si stamp topographically
patterned using conventional lithography which is pressed against
polymer coated substrate heated above the glass transition
temperature of the polymer. The stamp is removed after cooling,
leaving the imprint of the polymer. Residual polymer is removed
further by RIE and the patterned substrate is further modified to create
contrasts of protein adhering / resistant regions. In the recent work,
Fig. 5 μCP for protein surface patterning. (a) Micro-fabrication of a stamp is carried out by pouring liquid polydimethylsiloxane (PDMS) pre-polymer against silicon master mold and cured. (b) The PDMS stamp is released from the master and inked in protein solution. The subsequent rinsing and drying of the inked stamp produces a monolayer of protein and transferred to the target substrate by printing. Multiple proteins can be patterned either by sequential inking and printing (c), parallel inking of stamp followed by a single printing (d) or blocking of certain surface sites by adsorbing blocking agents such as bovine serum albumin (e). (Reprinted with permission from108).
(b)
(a) (c)
(d)
(e)
MT1304p22_35.indd 28 12/03/2010 14:58:32
Chemical patterning in biointerface science REVIEW
APRIL 2010 | VOLUME 13 | NUMBER 4 29
regeneration and reusability of N-nitrilotriacetic acid (NTA) patterned
substrate via NIL was successfully demonstrated by the repeatable
sequential immobilization and rinsing of DsRed protein and Green
fluorescent protein via histidine functionalization147.
A range of AFM based surface patterning methods have been
developed and employed extensively for the surface patterned
immobilization of proteins and cells. AFM based methods allow
immobilization in ambient conditions and enables patterning of
proteins with high spatial resolution and density. Nanoshaving148 and
the extended method of nanografting149 was developed in 1997 and
utilized most commonly on SAMs. The process involves the physical
scraping and removal of the SAM surface by the AFM tip (nanoshaving)
and the molecules with affinity towards the exposed surface are
subsequently grafted on the removed region (nanografting). To date,
SAM feature sizes as low as 2 x 4 nm2 has been demonstrated by
Liu et al.150. For surface protein patterning, EG containing SAMs can
be employed in the resist and immobilization of protein can be carried
out to avoid non specific adsorption of the surrounding unshaved
areas151. The recent development in the extended technique, reversal
nanografting, have overcome the issues associated with the original
nanografting process such as difficulty in maintaining the designed
geometry due to thermal drift, thiol in solution may exchange with
the chemisorbed thiol on substrate due to prolonged soaking, and
tip wear152. In general, reversal nanografting is almost the same
process as the original nanografting procedure, except that the protein
binding terminal containing thiols are bound to the substrate while
protein resistant thiols are in solution. Tan et al.152 demonstrated
the regulation in the coverage and immobilization of antibiotin IgG
by controlling the shaving size and spacing between the shaving lines
on reversal nanografted array of biotin with individual dot size of
25 – 300 nm2 (Fig. 6).
Out of the AFM based surface patterning methods available to
date, DPN has been attracting most attention since the technique was
pioneered by Mirkin’s group in 199957. DPN is a scanning probe based
technique where AFM cantilever tip is ‘inked’ in solution containing
particular molecules of choice and these are transferred from the tip
Fig. 6 Nanografting for protein patterning. (a) Reversal nanografting is carried out by (1) imaging the target surface immobilized with self assembled monolayer containing protein binding termini (2 and 3) shaving of the surface is carried out by AFM tip and shaved areas are immobilized with protein resisting thiols in solution (4) the resulting surface is imaged. (b) 1500 x 1500 nm area of thiolated biotin nanoarrays fabricated by reversal nanografting. (c) Same area as (b) after anti biotin Ig G protein immobilization. (d) The combined cursor plot in (b) and (c) revealing the local height change before and after Ig G immobilization. (e) 300 x 300 nm AFM image of area 1 in (b) containing 1089 biotin nanofeatures with 5.2 x 5.2 nm (f) 300 x 300 nm AFM image of area 2 in (b) containing 288 biotin nanofeatures with 12.7 x 12.7 nm. (g) 300 x 300 nm AFM image of area 3 in (b) containing 144 biotin nanofeatures with 10.3 x 31.9 nm. (Reprinted with permission from152).
(b)
(a)
(c) (d)
(e) (g)(f)
MT1304p22_35.indd 29 12/03/2010 14:58:38
REVIEW Chemical patterning in biointerface science
APRIL 2010 | VOLUME 13 | NUMBER 430
to the substrate surface via capillary transport. Direct and indirect
DPN methods have been developed; the direct method utilizes inks of
protein solution for single-step immobilization of protein onto surface
whereas the indirect method is carried out in a two-step process where
organic molecules such as alkanethiol are deposited first and proteins
are subsequently immobilized onto the surface from solution. The first
indirect DPN for protein patterning was demonstrated by Lee et al.153,
who has successfully immobilized lysozyme and immunoglobulin G
(IgG) onto arrays of 16-mercaptohexadecanoic acid (MHA) surrounded
by the protein resistant area of 11-mercaptoundecyl-tri(ethylene
glycol). The same group has also demonstrated direct DNP writing of
IgG onto base treated and aldehyde modified SiO2 substrates using
PEG modified tip to facilitate transport of protein to the surface
with sub-100 nm resolution154. Hyun et al. utilized indirect DPN and
produced ~ 230 nm array of biotinylated BSA mediated by specific
molecular recognition with streptavidin-biotin complex via covalent
attachment onto MHA155. More recent work in this area has attempted
to overcome some drawbacks associated with the technique, such
as retaining the biological activity of protein, the limited size of the
pattern that can be written and the amount of protein deposited.
Mirkin’s group has recently rectified the issue associated with the
limited fabrication area by utilizing 26 cantilever tips and successfully
immobilized biologically active IgG proteins in array format covering
~ 1 cm156. They have also demonstrated the capability of the parallel
DPN by using arrays of up to 55 000 cantilever tips simultaneously157
(Fig. 7). Wu et al.158 have developed layer-by-layer tip modification
method to form hydrophilic porous structures on the surface. The
modification increases the amount of ink that the tip can hold while
retaining biological activity of protein. Bellido et al.159 recently
demonstrated the possibility of controlling the number of proteins
deposited onto surface by direct DPN. Nanoarrays of ferritin were
fabricated directly on TEM grid and the number of molecules deposited
was controlled by the initial protein concentration, array dot diameter
and the contact angle between the ink solution and the substrate
(Fig. 8).
Implementation of colloidal lithography for protein and cell
patterning is relatively new. In general, colloidal lithography templating
prior to protein and cell immobilization can be carried out in two ways;
the colloids can be deposited electrostatically onto various substrates
in a geometrically random manner with defined separation distance or
Fig. 7 Massively parallel DPN. (a) Gravity driven alignment method used for parallel DPN with each pen capable of contacting with the substrate under the weight of the whole pen array. The exact position of the pen array is controlled by the AFM scanner head attached to the pen array via epoxy resin. (b) Optical micrograph of part of the two dimensional array of cantilevers. (c) Dot matrix map of the front face of the US five-cent coin. (d) Optical micrograph of a representative region of the substrate with 55,000 duplicates produced by parallel DPN. Each circular feature represents the front face of the US five cent coin made from 1-octadecane thiol dot features as mapped in (c). Inset: AFM image of single circular feature. (Reprinted with permission from157).
(b)
(a) (c)
(d)
MT1304p22_35.indd 30 12/03/2010 14:58:42
Chemical patterning in biointerface science REVIEW
APRIL 2010 | VOLUME 13 | NUMBER 4 31
colloids can be self assembled into a two dimensional hexagonal close
packed structure. In geometrically random templating, Michel et al.160
has combined the SMAP approach and colloidal lithography to create
nanopillers of TiO2 which was made protein adherent with dodecyl
phosphate (DDP) while SiO2 was made protein resistant by PLL-g-PEG
grafting. Streptavidin was patterned on the nanopillers with 50 nm
feature size over a large area. Similar approach was demonstrated by
Agheli et al.161, where electrostatically assembled polystyrene particles
were first made into gold ‘nanodiscs’ via particle annealing and dry
etching with SiO2 background. Alkanethiol was deposited onto gold,
followed by the PLL-g-PEG layer on SiO2. Laminin, BSA and polyclonal/
monoclonal anti-mouse laminin were immobilized and quantitatively
characterized using AFM height histogram and QCM. Cai et al.162
created hexagonally arranged ~ 120 nm nanoarrays of lysozyme over
1cm2. 10-undecenyltrichlorosilane (UTS) was initially deposited onto
Si substrate followed by colloidal template and PEG silane. Colloids
were removed ultrasonically and the lysozyme was deposited on
the UTS exposed surface. Blatter et al.163 has also employed similar
methodology to create submicron protein array. PS particles were
first assembled onto TiO2/SiO2 substrate and combinations of O2/N2
and SF6/O2 etchings were carried out, followed by the lift-off of the
particles to create TiO2 and SiO2 contrast. Protein immobilization onto
TiO2 was carried out by pre-functionalizing the TiO2 and SiO2 with
DDP and PLL-g-PEG, respectively.
Use of programmable self assembly of DNA as a template
for protein patterning has been recently attracting attention.
Two dimensional DNA template for protein patterning was first
demonstrated by Yan et al. in 2003164. Periodic pattern of streptavidin
was achieved by the self assembly of DNA via the reprogrammed
sticky ends into 4 x 4 tiles of nanogrids containing biotinylated
oligonucleotides on each tile junctions separated by ~ 19 nm.
A variety of positioning of streptavidin was achieved further by
selectively modifying each tile with biotin and combining two DNA
tiles together165. Cohen et al.166 demonstrated the use of polyamide-
biotin conjugate to achieve multiple arrangements of streptavidin on a
single DNA tile with ~ 25 nm separations. In a similar manner, human
α-thrombin binding aptamer and platelet derived growth factor (PDGF)
binding aptamers have been incorporated into the DNA template
and the thrombin and PDGF were subsequently patterned167. DNA’s
ability to form an intricate two dimensional geometry with nanometer
precision programmable control makes this technique an attractive
candidate for protein patterning.
3D PatterningIn vivo, cells inhabit a 3D rather than a 2D world. Thus, in regenerative
medicine and the construction of cellular tissue models efforts are
made to achieve this environment using a variety of strategies
including coalesced particles, porous scaffold materials and hydrogels.
Patterning of surface chemistry over long length scales (up to 10s of
millimetres) has been shown to be of great utility in controlling cell
distribution in macroscopic tissue engineering scaffolds168. Gradients
of surface chemistry within porous 3D objects were first exploited to
control fibroblast adhesion in a porous poly(lactic acid) tissue scaffold
formed by super critical CO2 processing by Barry et al.168. Plasma
polymers were deposited to introduce nitrogen functionalities which
enhanced cell adhesion in the centre of a porous 3D object. The
graduated deposition thickness achieved from the periphery to the
centre of the thick disc placed in the plasma was exploited to form
a radial chemical gradient of a second cell resistant plasma polymer
(a hydrophobic hexane plasma polymer). This chemical gradient
achieved a decreasing fibroblast density at the periphery and increase
in the centre, as seen in Fig. 9, thus, counteracting the tendency of
cells to adhere to the periphery of the porous object. This method
achieved a uniform cell distribution in the scaffold, one of the pre-
requisites to tissue formation. Recently a 3D photo patterning method
achieving in hydrogels has been published which allows spatial control
Fig. 8 Controlling the number of protein by direct DPN. (a) Schematic illustration of ferritin pattern produced onto the surface of the TEM grid. (b) TEM images of a ferritin nanoarray (20 x 20 μm, 150 nm feature) generated by direct DPN on a TEM grid. The scale bars are 2 μm, 500 nm and 100 nm for different magnifications. (Reprinted with permission from159).
(b)
(a)
MT1304p22_35.indd 31 12/03/2010 14:58:46
REVIEW Chemical patterning in biointerface science
APRIL 2010 | VOLUME 13 | NUMBER 432
with micrometer scale resolution of biological functionalities such as
RGD (Fig. 10). This exciting new method based on orthogonal click
chemistries shows great promise with the initial report showing control
of cell migration, proliferation and morphological changes169.
High throughput screening approaches to find new materialsPolymer spots of a few hundred microns in diameter formed by micro
array printing are being exploited as material discovery platforms
in high throughput (HT) screening analogous to HT drug discovery.
Anderson and Langer developed an approach to print 576 unique
materials in triplicate on a slide coated with a cell resistant hydrogel170.
They used UV photoinitiated acrylate monomers which provided a
large library of chemical moieties. A convenient combinatorial on-slide
production method was subsequently developed by Bradley et al.
to allow on-slide monomer mixing and thereby potentially further
increasing throughput171. Cell-surface interactions can be studied
on these large micro array libraries of materials (Fig. 11)172,173.
Importantly, as with all materials the surface chemistry must be
well characterised in order to correctly interpret cell response to the
surface, which poses a challenge when dealing with so many samples.
A complementary range of surface analysis techniques, including ToF
SIMS, XPS and sessile drop water contact angle have been developed
to allow high throughput surface characterisation (HT-SC) to be carried
out within the same time frame as the cell culture experiments (a few
days)171. The challenge in HT-SC is automation of the data handling
methods to identify correlations in the large amount of data generated
from this type of combinatorial materials platform174. However, the
method is proving extremely useful at identifying polymers with
application in biotechnology and in understanding the cell response to
materials.
Summary and outlookChemical manipulation and patterning of material surfaces embrace
exciting opportunities in biology and medicine that aim to improve
the quality of human life. The repertoire of patterning methods and
techniques that has been pioneered over the last several decades,
and their advancement have been significantly helped by scientific
and instrumental progressions made in the field of surface analysis.
This linked progression has provided us with the ability to influence
and control a range of biological components from mm to nm scales.
Control over the length scale allows us to integrate newly patterned
Fig. 9 Controlling cell distribution in tissue engineering scaffolds via surface chemical gradients. Surface chemical contrast were created in the core and sheath of Poly-DL-lactic acid (PDLLA) scaffold by plasma polymer depositions of cell adhesive allyl amine (ppAAm) and cell repulsive hexane (ppHex). (a) Scaffolds cultured with 3T3 fibroblasts for 24 h (the scale bars are 1 mm and cells are color-coded in red): (1) PDLLA, (2) PDLLA/ppAAm, and (3) PDLLA/ppAAm/ppHex. The lower images show X-ray μCT images from approximately 2 mm slices through the centers of the scaffolds. (b) Cumulative cell area in the 0.01 mm slices through the centers of the scaffold within the core and the sheath denoted by the black dotted lines in (a). (Reprinted with permission from168).
(b)
(a) 1 2 3
MT1304p22_35.indd 32 12/03/2010 14:58:48
Chemical patterning in biointerface science REVIEW
APRIL 2010 | VOLUME 13 | NUMBER 4 33
Fig. 10 Cytocompatible, 3D biochemical patterning within preformed click hydrogels. (a) The thiol–ene reaction mechanism provides a means to quantitatively couple sulphhydryls (–SH) with vinyl functionalities (–C=C) in the presence of light. (b) On swelling into the material, relevant thiol-containing biomolecules are covalently affixed to the hydrogel network at varying concentrations by altering the dosage of exposed light (intensity and exposure time). (c) A live/dead stain at 24 h after photolithographic patterning of 3T3s indicates a predominantly viable population (live cells are shown in green, whereas dead cells are shown in red) and that the patterning process is cytocompatible. (d) The thiol–ene reaction is confined to user-defined regions in space using photomasks to introduce three different fluorescently labelled peptide sequences within the gel, a process that can be repeated at desired times and spatial locations to introduce additional biochemical cues. (e) By controlling the focal point of the laser light in three dimensions using a confocal microscope, micrometre-scale spatial patterning resolution is achieved. Values in (b) are reported as mean ± s:d: (n = 5). The image in (c) represents a 200 μm confocal projection. The images in (d )and (e) represent confocal micrographs of fluorescently tagged peptides patterned within the networks. (Reprinted with permission from169).
Fig. 11 Human embryonic stem (hES) cells grown on polymer arrays. (a-c) Six million hES cell embryoid body day-6 cells were added on the polymer array in the presence of retinoic acid for 6 day and then stained for cytokeratin 7 (green) and vimentin (red). Polymer spots can be identified by blue fluorescence. (d) Nuclei were also stained (green) (not shown in other images to simplify presentation). (e) Typical cytokeratin 7 positive spot. (Reprinted with permission from170).
(b)(a) (c)
(d) (e)
(b)(a) (c)
(d)
(e)
MT1304p22_35.indd 33 12/03/2010 14:58:52
REVIEW Chemical patterning in biointerface science
APRIL 2010 | VOLUME 13 | NUMBER 434
chemistries and functionalities onto a variety of medically relevant
device surfaces of various sizes and shapes for resisting protein
adsorption and mammalian and bacterial cell attachment which may
threaten health and well being. Despite these remarkable advances,
each of the chemical and biological patterning processes possess
drawbacks, and improvement of conventional techniques, as well as
the development of new methods can only be made into reality by
overcoming analytical challenges, particularly in 3D where one might,
for example, want to display multiple signals with nanoscale spatial
distribution. The drawbacks associated with the chemical and spatial
sensitivities may hinder meaningful characterization of the patterns.
In addition many of the current surface analytical techniques are
carried out in vacuum environment which is not the representative
of the native state of the biological components. Thus a combined
use of a range of surface analytical techniques is essential for gaining
the thorough characterization of the patterned surface needed to
understand its biological response. The synergy among the surface
engineers and surface scientists in the development of surface
analytical instruments and the patterning processes must continue,
in order to desirably harness the biological components in a range
of scales that are essentially invaluable in progressing materials to
improving human health.
REFERENCES
1. Baier, R. E. and Dutton, R. C., J Biomed Mater Res. (1969) 3 (1), 191.
2. Andrade, J. D., Protein Adsorption. 1985, New York: Plenum.
3. Gray, J. J., Curr Opin Struc Biol (2004) 14 (1), 110.
4. Hlady, V., and Buijs, J., Curr Opin Biotech (1996) 7 (1), 72.
5. Andrade, J. D., and Hlady, V., Plasma Protein Adsorption: The Big Twelve. Annals of the New York Academy of Sciences, (1987) 516 (Blood in Contact with Natural and Artificial Surfaces) 158.
6. Horbett, T. A., and Brash, J. L., Proteins at interfaces II : fundamentals and applications. 1995, Washington, D.C.: American Chemical Society. xiv, pp 561.
7. Keselowsky, B. G., et al., Biomaterials (2004) 25 (28), 5947.
8. Lukashev, M. E., and Werb, Z., Trends in Cell Biology (1998) 8 (11), 437.
9. Costerton, J. W., et al., Science (1999) 284 (5418), 1318.
10. Gorbet, M.B. and Sefton, M. V., Biomaterials (2004) 25 (26), 5681.
11. Lin, W. -C., et al., Biomaterials (2004) 25 (10), 1947.
12. McClean, D. R., and Eigler, N. L., Rev Cardiovasc Med (2002) 3 (suppl 5), S16.
13. Laurencin, C. T. and Nair, L. S., Nanotechnology and tissue engineering : the scaffold. 2008, Boca Raton: CRC Press. xvii, pp 359.
14. Blum, L. J., and Coulet, P. R., Biosensor principles and applications. Bioprocess technology v. 15. 1991, New York: M. Dekker. x, pp 357.
15. Nilsson, K. G. I. and Mandenius, C. F., Nature Biotechnology (1994) 12 (13), 1376.
16. Tao, S. L. and Desai, T, A., Adv Drug Deliver Rev (2003) 55 (3), 315.
17. Ratner, B. D., Biomaterials science : an introduction to materials in medicine. 1996, San Diego: Academic Press. xi, pp 484.
18. Niemeyer, C. M. and Mirkin, C. A., Nanobiotechnology : concepts, applications and perspectives. 2004, Weinheim: Wiley-VCH. xxii, pp 469.
19. Curtis, A. and Wilkinson, C., Biomaterials (1997) 18 (24), 1573.
20. Keselowsky, B. G., et al., PNAS (2005) 102 (17), 5953.
21. Lecuit, T. and Lenne, P. -F., Nat Rev Mol Cell Biol (2007) 8 (8), 633.
22. Boyan, B. D., et al., Biomaterials (1996) 17 (2), 137.
23. Craighead, H. G., et al., Curr Opin Solid St M (2001) 5 (2-3), 177.
24. Teti, A., J Am Soc Nephrol (1992) 2 (10), S83.
25. Hubbard, A. T., The Handbook of surface imaging and visualization. 1995, Boca Raton: CRC Press. xv, pp 909.
26. Craighead, H. G., et al., Applied Physics Letters (1983) 42 (1), 38.
27. Ito, T. and Okazaki, S., Nature (2000) 406 (6799), 1027.
28. Thompson, L. F., and Kerwin, R. E., Annu Rev Mater Sci (1976) 6 (1), 267.
29. Romankiw, L. T., Electrochim Acta (1997) 42 (20-22), 2985.
30. Craighead, H. G., Science (2000) 290 (5496), 1532.
31. Fischbein, M. D., and Drndic, M., Nano Letters (2007) 7 (5), 1329.
32. Lemmo, A. V., et al., Curr Opin Biotech (1998) 9 (6), 615.
33. de Gans, B. -J., et al., Adv Mater (2004) 16 (3), 203.
34. Nakamura, M., et al., Tissue Engineering (2005) 11 (11-12), 1658.
35. Park, J. -U., et al., Nat Mater (2007) 6 (10), 782.
36. Bain, C. D., et al., J Am Chem Soc (1989) 111 (18), 7155.
37. Bain, C. D., et al., J Am Chem Soc (1989) 111 (1), 321.
38. Bain, C. D., and Whitesides, G. M., et al., J Am Chem Soc (1989) 111 (18), 7164.
39. Ulman, A., Chemical Reviews (1996) 96 (4), 1533.
40. Love, J. C., et al., Chemical Reviews (2005) 105 (4), 1103.
41. Huang, E., et al., Nature (1998) 395 (6704), 757.
42. Lazzari, M., and López-Quintela, M. A., Adv Mater (2003) 15 (19), 1583.
43. Möller, M., et al., Adv Mater (1996) 8 (4), 337.
44. Cavalcanti-Adam, E. A., et al., Biophysical Journal (2007) 92 (8), 2964.
45. Huang, J., et al., Nano Letters (2009) 9 (3), 1111.
46. Choi, D.-G., et al., J Am Chem Soc (2004) 126 (22), 7019.
47. Zheng, Y., et al., Colloid Surface A (2006) 277 (1-3), 27.
48. Chen, J., et al., ACS Nano (2008) 3 (1), 173.
49. Burmeister, F., et al., Langmuir (1997) 13 (11), 2983.
50. Kosiorek, A., et al., Nano Letters (2004) 4 (7), 1359.
51. Kosiorek, A., et al., Small (2005) 1 (4), 439.
52. Xia, Y. and Whitesides, G. M., Annu Rev Mater Sci (2003) 28 (1), 153.
53. Kumar, A. and Whitesides, G. M., Applied Physics Letters (1993) 63 (14), 2002.
54. Xia, Y., et al., Adv Mater (1997) 9 (2), 147.
55. Zhao, X. -M., et al., Adv Mater (1996) 8 (5), 420.
56. Kim, E., et al., Adv Mater (1997) 9 (8), 651.
57. Piner, R. D., et al., Science (1999) 283 (5402), 661.
58. Hoff, J. D., et al., Nano Letters (2004) 4 (5), 853.
59. Castner, D. G. and Ratner, B. D., Surface Science (2002) 500 (1-3), 28.
60. Briggs, D. and Grant, J. T., Surface analysis by Auger and x-ray photoelectron spectroscopy. 2003, Chichester, West Sussex, U.K.: IM Publications. xi, pp 899.
61. Briggs, D., Surface analysis of polymers by XPS and static SIMS. 1998, Cambridge: Cambridge University Press. xiv, pp 198.
62. Briggs, D. and Seah, M. P., Practical surface analysis. Vol.1, Auger and X-ray photoelectron spectroscopy. 2nd ed. ed. 1996: Chichester : Wiley. xiv, pp 657.
63. Vickerman, J. C. and Briggs, D., ToF-SIMS : surface analysis by mass spectrometry. 2001, Chichester: IM. ix, pp 789.
64. Briggs, D. E. and Seah, M. P. E., Practical surface analysis. Vol 2, Ion and neutral spectroscopy. 2nd ed. 1992, Wiley: Salle + Sauerla\0308nder.
65. Ostrowski, S. G., et al., Science (2004) 305 (5680), 71.
66. Kraft, M. L., et al., Science (2006) 313 (5795), 1948.
67. Fletcher, J. S., et al., Analytical Chemistry (2007) 79 (6), 2199.
68. Parry, S. and Winograd, N., Analytical Chemistry (2005) 77 (24), 7950.
69. Nygren, H., et al., Microsc Res Techniq (2007) 70 (11), 969.
70. Touboul, D., et al., J Am Soc Mass Spectr (2005) 16 (10), 1608.
71. Nygren, H., et al., FEBS Letters (2004) 566 (1-3), 291.
72. Wu, L., et al., Int J Mass Spectrom (2007) 260 (2-3), 137.
MT1304p22_35.indd 34 12/03/2010 14:58:59
Chemical patterning in biointerface science REVIEW
APRIL 2010 | VOLUME 13 | NUMBER 4 35
73. Binnig, G., et al., Phys Rev Lett (1986) 56 (9), 930.
74. Vilarinho, P. M., et al., Scanning probe microscopy : characterization, nanofabrication and device application of functional materials. NATO science series. Series II, Mathematics, physics, and chemistry v. 186. 2005, Dordrecht ; Boston: Kluwer Academic Publishers. xxxvii, pp 488.
75. Vansteenkiste, S. O., et al., Prog Surf Sci (1998) 57 (2), 95.
76. Frisbie, C. D., et al., Science (1994) 265 (5181), 2071.
77. van der Vegte, E. W. and Hadziioannou, G., Langmuir (1997) 13 (16), 4357.
78. Raab, A., et al., Nat Biotechnol (1999) 17, 901.
79. Allen, S., et al., Biochemistry (1997) 36 (24), 7457.
80. Chilkoti, A., et al., Biophys J. (1995) 69 (5), 2125.
81. Allen, S., et al., FEBS Letters (1996) 390 (2), 161.
82. Lee, G., et al., Science (1994) 266 (5186), 771.
83. Thie, M., et al., Hum. Reprod. (1998) 13 (11), 3211.
84. Noy, A., Handbook of molecular force spectroscopy. 2008, New York, NY: Springer. xii, pp 291.
85. Wong, S. S., et al., Nature (1998) 394 (6688), 52.
86. Gross, L., et al., Science (2009) 325 (5944), 1110.
87. Martin, S. J., et al., Anal Chem (1991) 63 (20), 2272.
88. Nienhaus, G. U., Protein-ligand interactions : methods and applications. 2005, Totowa, N.J.: Humana Press. xi, pp 568.
89. Schasfoort, R. B. M. and Tudos, A. J., Handbook of surface plasmon resonance. 2008, Cambridge: Royal Society of Chemistry. xxi, pp 403.
90. Homola, J., Chemical Reviews (2008) 108 (2), 462.
91. Brockman, J. M., et al., Annu Rev Phys Chem (2000) 51 (1), 41.
92. Steiner, G., Anal Bioanal Chem (2004) 379 (3), 328.
93. Su, X., et al., Langmuir (2005) 21 (1), 348.
94. Peh, W. Y. X., et al., Biophys. J. (2007) 92 (12), 4415.
95. Yu, J. -S., et al., J. Virol. Methods (2006) 137 (2), 219.
96. Tsuzuki, S., et al., Biotechnol Bioeng (2009) 102 (3), 700.
97. von Recum, A. F., Handbook of biomaterials evaluation : scientific, technical, and clinical testing of implant materials. 2nd ed. 1999, Philadelphia, Penn. ; London: Taylor & Francis. xix, pp 915.
98. Spencer, N.D . and Moore, J. H., Encyclopedia of chemical physics and physical chemistry. Vol. 2. 2001, Bristol ; Philadelphia: Institute of Physics Pub.
99. Vickerman, J. C. and Gilmore, I. S., Surface analysis : the principal techniques. 2nd ed. 2009, Chichester, U.K.: Wiley. xix, pp 666.
100. Rivière, J. C. and Myhra, S., Handbook of surface and interface analysis methods for problem-solving. 2nd ed. 2009, Boca Raton: Taylor & Francis.
101. Chapman, R. G., et al., American Chemical Society (2000) 122 (34), 8303.
102. Ostuni, E., et al., Langmuir (2001) 17 (18), 5605.
103. Luk, Y. -Y., et al., Langmuir (2000) 16 (24), 9604.
104. Denis, F. A., et al., Langmuir (2002) 18 (3), 819.
105. Roach, P., et al., Journal of the American Chemical Society (2005) 127 (22), 8168.
106. Tsukagoshi, T., et al., Colloid Surface B (2007) 54 (1), 82.
107. Szleifer, I., Biophys J. (1997) 72 (2, Part 1), 595.
108. Bernard, A., et al., Adv Mater (2000) 12 (14), 1067.
109. Jeon, S. I. and Andrade, J. D., J Colloid Interf Sci (1991) 142 (1), 159.
110. Pasche, S., et al., J Phys Chem B (2005) 109 (37), 17545.
111. Kingshott, P. and Griesser, H. J., Curr Opin Solid St M (1999) 4 (4), 403.
112. Kingshott, P., et al., Biomaterials (2002) 23 (9), 2043.
113. Wei, J., et al., Colloid Surface B (2003) 32 (4), 275.
114. Kingshott, P., et al., Langmuir (2003) 19 (17), 6912.
115. Norde, W. and Gage, D., Langmuir (2004) 20 (10), 4162.
116. Sofia, S. J., et al., Macromolecules (1998) 31 (15), 5059.
117. Gombotz, W. R., et al., J Biomed Mater Res. (1991) 25 (12), 1547.
118. Hamilton-Brown, P., et al., Langmuir (2009) 25 (16), 9149.
119. Unsworth, L. D., et al., Langmuir (2008) 24 (5), 1924.
120. Ademovic, Z., et al., Plasma Process Polym (2005) 2 (1), 53.
121. Johnston, E. E., et al., Langmuir (2004) 21 (3), 870.
122. Bremmell, K. E., et al., Langmuir (2005) 22 (1), 313.
123. Pasche, S., et al., Langmuir (2003) 19 (22), 9216.
124. Pasche, S., et al., Langmuir (2005) 21 (14), 6508.
125. Park, J. Y., et al., Biomaterials (2006) 27 (6), 856.
126. George, P. A., et al., Biomaterials (2009) 30 (13), 2449.
127. Ma, H., et al., Adv Mater (2004) 16 (4), 338.
128. Saldarriaga Fernández, I. C., et al., Biomaterials (2007) 28 (28), 4105.
129. Harbers, G. M., et al., Chem Mater (2007) 19 (18) 4405.
130. Ostuni, E., et al., Langmuir (2001) 17 (20), 6336.
131. Li, L. Y., et al., J Phys Chem B (2005) 109 (7), 2934.
132. Harder, P., et al., J Phys Chem B (1998) 102 (2), 426.
133. Heuberger, R., et al., Adv Funct Mater (2005) 15 (3) 357.
134. Thissen, H., et al., Biomaterials (2006) 27 (1), 35.
135. Ma, H., et al., Adv Funct Mater (2006) 16 (5), 640.
136. Srituravanich, W., et al., Nano Letters (2004) 4 (6), 1085.
137. Sun, S., et al., J Am Chem Soc (2002) 124 (11), 2414.
138. Carrico, I.S., et al., J Am Chem Soc (2007) 129 (16), 4874.
139. Dubey, M., et al., Adv Funct Mater (2009) 19 (19), 3046.
140. Mrksich, M. and Whitesides, G. M., Annu Rev Bioph Biom (1996) 25, 55.
141. Mrksich, M., et al., Exp Cell Res (1997) 235 (2), 305.
142. Renault, J.P., et al., J Phys Chem B (2002) 107 (3), 703.
143. Yunus, S., et al., Surf Interface Anal (2007) 39 (12-13), 922.
144. Csucs, G., et al., Langmuir (2003) 19 (15), 6104.
145. Michel, R., et al., Langmuir (2002) 18 (8), 3281.
146. Lussi, J. W., et al., Nanotechnology (2005) 16, 1781.
147. Maury, P., et al., Small (2007) 3 (9), 1584.
148. Xu, S. and G. -y. Liu, Langmuir (1997) 13 (2), 127.
149. Xu, S., et al., Langmuir (1999) 15 (21), 7244.
150. Liu, G. -y. and Amro, N. A., PNAS (2002) 99, 5165.
151. Kenseth, J. R., et al., Langmuir (2001) 17 (13), 4105.
152. Tan, Y. H., et al., ACS Nano (2008) 2 (11), 2374.
153. Lee, K. -B., et al., Science (2002) 295 (5560), 1702.
154. Lim, J. -H., et al., Angew Chem Int Edit (2003) 42 (20), 2309.
155. Hyun, J., et al., Nano Letters (2002) 2 (11), 1203.
156. Lee, S. W., et al., Adv Mater (2006) 18 (9), 1133.
157. Salaita, K., et al., Angew Chem Int Edit (2006) 45 (43), 7220.
158. Wu, C. -C., et al., J Am Chem Soc (2009) 131 (22), 7526.
159. Bellido, E., et al., Adv Mater (2009) 22 (3), 352.
160. Michel, R., et al., Langmuir (2002) 18 (22), 8580.
161. Agheli, H., et al., Nano Letters (2006) 6 (6), 1165.
162. Cai, Y. and Ocko, B. M., Langmuir (2005) 21 (20), 9274.
163. Blatter, T. M., et al., Nanotechnology (2008) 19, 75301.
164. Yan, H., et al., Science (2003) 301 (5641), 1882.
165. Park, S. H., et al., Nano Letters (2005) 5 (4), 729.
166. Cohen, J. D., et al., J Am Chem Soc (2007) 130 (2), 402.
167. Chhabra, R., et al., J Am Chem Soc (2007) 129 (34), 10304.
168. Barry, J. J., et al., Adv Mater (2006) 18 (11), 1406.
169. DeForest, C. A., et al., Nat Mater (2009) 8 (8), 659.
170. Anderson, D., et al., Nat Biotechnol Letters (2004) 22 (17), 863.
171. Zhang, R., et al., Chem Commun (2008) 11, 1317.
172. Urquhart, A., et al., Adv Mater (2007) 19, 2486.
173. Mei, Y., et al., Adv Mater (2009) 21, 1.
174. Urquhart, A., et al., Anal Chem (2008) 80, 135.
MT1304p22_35.indd 35 12/03/2010 14:58:59