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Hyperbranched poly(NIPAM) polymers
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bacterial burden in...
Article in Biomaterials · October 2010
DOI: 10.1016/j.biomaterials.2010.08.084 · Source: PubMed
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Biomaterials 32 (2011) 258e267
Contents lists available at ScienceDirect
Biomaterials
journal homepage: www.elsevier.com/locate/biomaterials
Hyperbranched poly(NIPAM) polymers modified with antibiotics for the
reduction of bacterial burden in infected human tissue engineered skin
Joanna Shepherd a, b, Prodip Sarker c, Stephen Rimmer c, Linda Swanson c, Sheila MacNeil b, Ian Douglas a, *
a
Unit of Oral & Maxillofacial Pathology, School of Clinical Dentistry, University of Sheffield, Claremont Crescent, Sheffield S10 2TA, United Kingdom
Department of Engineering Materials, Kroto Research Institute, North Campus, University of Sheffield, Broad Lane, Sheffield S3 7HQ, United Kingdom
c
Department of Chemistry, University of Sheffield, Sheffield S3 7HF, United Kingdom
b
a r t i c l e i n f o
a b s t r a c t
Article history:
Received 29 July 2010
Accepted 27 August 2010
Available online 8 October 2010
The escalating global incidence of bacterial infection, particularly in chronic wounds, is a problem that
requires significant improvements to existing therapies. We have developed hyperbranched poly(NIPAM)
polymers functionalized with the antibiotics Vancomycin and Polymyxin-B that are sensitive to the
presence of bacteria in solution. Binding of bacteria to the polymers causes a conformational change,
resulting in collapse of the polymers and the formation of insoluble polymer/bacteria complexes. We
have applied these novel polymers to our tissue engineered human skin model of a burn wound infected
with Pseudomonas aeruginosa and Staphylococcus aureus. When the polymers were removed from the
infected skin, either in a polymer gel solution or in the form of hydrogel membranes, they removed
bound bacteria, thus reducing the bacterial load in the infected skin model. These bacteria-binding
polymers have many potential uses, including coatings for wound dressings.
Ó 2010 Elsevier Ltd. All rights reserved.
Keywords:
Bacteria
Hydrogel
Infection
Microbiology
Polymerization
Wound dressing
1. Introduction
Bacterial infection of burns, wounds and ulcers of the skin is
a worldwide challenge, which is increasing with the rise of diabetes
and advancing age of the population. Furthermore, the rise in
bacterial antibiotic resistance is compounding difficulties of wound
management [1].
There is a clear need, therefore, for improving management of
both chronic bacterial skin infections and those which may occur in
areas or situations remote from specialised clinical care, such as on
the battlefield. Chronic infections of ulcers and pressure sores,
which may be compounded by poor circulation and malnutrition,
can delay wound healing for several years. Traditionally, topical
antibiotics have been applied to infected wounds and the wounds
dressed and re-dressed until the infection has diminished. This
approach avoids systemic administration of antibiotics and the
associated side-effects. However it can contribute to antibiotic
resistance particularly when used in the treatment of long-term
recalcitrant infected wounds. Alternatives to antibiotics have
become more widely used because of this problem. For example,
various silver compounds have been used, which although effective
as antibacterial agents, can be toxic to the host tissue at high local
* Corresponding author. Tel.: þ44 114 2717957; fax: þ44 114 2717894.
E-mail address: i.douglas@sheffield.ac.uk (I. Douglas).
0142-9612/$ e see front matter Ó 2010 Elsevier Ltd. All rights reserved.
doi:10.1016/j.biomaterials.2010.08.084
concentrations and treatment can have the effect of delaying
wound healing [2]. In an effort to overcome some of these problems
we have developed stimulus responsive hyperbranched poly
(N-isopropyl acrylamide) (HB-PNIPAM) polymers conjugated with
the antibiotics Polymyxin-B (HB-PNIPAM-pmx) [unpublished data]
and Vancomycin (HB-PNIPAM-van) [3], that are able to selectively
bind Gram-negative and Gram-positive bacteria respectively. In
both cases the conjugated antibiotics do not have bactericidal
activity but they bind bacteria via the latter’s target surface groups.
PNIPAM has garnered increasing interest for use in biological
systems, since as well as being non-toxic to host tissue, it has
thermosensitive properties. At temperatures below 32 C, the
polymer is hydrophilic and remains in a coiled form in solution.
However, on raising the temperature past 32 C, which is its lower
critical solution temperature (LCST), the polymer desolvates and
switches to a globular formation. Since the first described interaction of biomolecules with PNIPAM in 1992 [4], this property has
been exploited in the design of several biological agents [5e7].
Functionalization of the NIPAM monomer with other molecules can
further modify the sensitivity of PNIPAM to the environment. For
example, addition of acrylic acid or methacrylic acid results in
microgels that are pH responsive [8], which have several potential
uses including drug delivery. However, prior to our work, there
have been no studies describing the transitions from coil-globule
on binding to a cellular target. With HB-PNIPAM this is possible
because the location of the ligands at chain ends ensures that they
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J. Shepherd et al. / Biomaterials 32 (2011) 258e267
are available for binding both above and below the LCST: chain end
groups tend not to penetrate the coil of the highly branched polymer [9]. Since the binding interactions involve a large perturbation
of the overall solvation of the polymer, the LCST is reduced. The
reduction of the LCST is observed as a coil-to-globule transition if
the magnitude of the change is sufficient to reduce the LCST to
below ambient temperature. The adhesion of bacteria to PNIPAM
above the LCST and release below the LCST is well-known [10] and
in our previous work [3] we showed that binding followed by the
coil-to-globule transition is accompanied by aggregation of target
bacteria. Linkage of antimicrobial peptides and antibiotics to
other materials, such as titanium surfaces for surgical implants
[11], sepharose beads for LPS decontamination [12], cloths/fibres
[13,14] and membranes [15] have been investigated, but none of
these materials possess the inherently useful responsive properties
of PNIPAM. We have recently shown that at physiologically
relevant temperatures, HB-PNIPAM-van in solution specifically
binds Gram-positive bacteria, an event which induces a coil-toglobule transition resulting in the formation of an insoluble
complex of polymer-bound bacteria [3]. We reasoned therefore,
that our polymers may be able to act as a dressing to actively
remove bacteria from infected tissue.
To evaluate the usefulness of these polymers in a simulated in
vivo environment, we recently developed a three dimensional
tissue engineered model of bacterial infected burnt human skin.
This was infected with either the Gram-positive bacterium Staphylococcus aureus or the Gram-negative bacterium Pseudomonas
aeruginosa [16]. In the current study, we used this human infected
skin model to examine the ability of both the free polymers and
polymers bound to hydrogel membranes to selectively bind and
remove P.aeruginosa or S.aureus from these infected wound beds.
2. Materials and methods
2.1. Materials
HB-PNIPAM-COOH was prepared as previously described [17]. N,N-dimethylformamide (DMF) (Aldrich, sure-seal) and dioxane (Aldrich, sure-seal) were
used as received. N,N-dicylohexylcarbodimide (Aldrich, 99%) and N-hydroxy Succinimide (Aldrich, 98%), 1-Amino anthracene (Aldrich) were used as received. IPA
(isopropyl alcohol) and Ethanol (Fisher) HPLC grade were used. TriseHCl was used as
purchased. Polymyxin-B Sulphate (Fluka), Vancomycin hydrochloride (SigmaeAldrich), polymyxin acylase as enzyme (Sigma), Fmoc-Chloride (Fluka, >98%),
piperidine (Aldrich, 99%) were used as supplied. Ethylene glycol dimethacrylate
(EGDMA) was passed through a column of basic alumina to remove the inhibitor.
Glycidyl methacrylate (GME) was distilled under reduced pressure prior to use.
Ethylene diamine was obtained from Fluka (UK) was used without further purification. Photo initiator, 2-hydroxy-2-methylpropiophenone (Aldrich) was used as
received.
2.2. Modification of polymyxin-B sulphate
FMoC-pmx was prepared in aqueous medium. A mixture of fluorenylmethyloxycarbonyl chloride (200 mg) and 1M Na2CO3 aqueous (5 cm3) was
added to a solution of polymyxin-B sulfate (500 mg in 10 cm3 water) and this was
stirred at room temperature over-night. FMoC-pmx was insoluble in water and it
was filtered off and washed with water several times to remove unreacted reagents.
In FTIR spectra, new bands due to FMoC (9-Fluorenylmethoxycarbonyl) group
appeared at 1450 cm 1 and from 1300 cm 1e1200 cm 1. FMoC-pmx had a melting
point of 236 C and the structure was confirmed by mass spectrometry (observed m/z
2314 Da (FAB-MS), theoretical exact mass 2313.090). To remove the terminal alkyl
chain, a mixture of FMoC-pmx (50 mg in 16 cm3 50 mM TriseHCl, 0.3945 g TriseHCl in
50 cm3 water) and polymyxin acylase (2 cm3, 16 mg polymyxin acylase in 16 cm3
phosphate buffer pH 8.0) was stirred at room temperature over-night. Since the
deacylated product (FMoC-pmx-deacylate) was insoluble in water and common
organic solvents, it was filtered and washed several times to remove the unreacted
reagents. In FTIR, a band at 1100 cm 1 due to the alkyl chain present in the FMoC-pmx
was absent after enzymatic cleavage. The melting point was 277 C and the structure
was confirmed by mass spectrometry (observed m/z 2174 Da (FAB-MS), theoretical
exact mass 2172.97).
259
2.2.1. HB-PNIPAM-COOH with 1-amino anthracene at a fraction of the chain ends
(HB-PNIPAM-A-suc)
HB-PNIPAM-COOH (70 mg) was dissolved in DMF (1.5 cm3) and N,N-dicylohexylcarbodimide (DCC) (17 mg) and N-hydroxy Succinimide (9.5 mg) in DMF
(1 cm3) were added to it. The solution was stirred under N2 over-night and solvent
was removed by rotary-evaporator. The solid was dissolved in acetone/ethanol
mixture (9:1) and concentrated by ultra-filtration over 1 h. The ultra-filtration was
repeated three times; solvent was removed by rotary-evaporation and dried under
vacuum at room temperature. The solid was dissolved in DMF and precipitated in
diethyl ether, polymer filtered off and dried under vacuum at room temperature.
HB-PNIPAM-succinimide, 300 mg was dissolved in DMF (10 cm3) and a solution
of disopropylamine (3 mg) and 1-aminofluorescene (3 mg) in DMF (6 cm3) were
added to it. The reaction mixture was stirred at room temperature over-night. The
solvent was removed by rotary-evaporation and then the solid was dissolved in
acetone/ethanol mixture (9:1) and concentrated by ultra-filtration over 1 h. The
ultra-filtration was repeated three times; solvent was removed by rotary-evaporation
and dried under vacuum at room temperature. The solid was dissolved in DMF again
and precipitated in diethyl ether, filtered off and dried under vacuum at room
temperature.
2.2.2. Synthesis of HB-PNIPAM-van and HB-PNIPAM-pmx
HB-PNIPAM-A-suc (50 mg) was dissolved in water (2.5 cm3) over ice. Then the
solution transferred to a small reaction tube. A solution of Vancomycin (15 mg) in
water (1 ml) and 0.1 M sodium phosphate buffer (pH 8.5) (1 cm3) were added to the
polymer solution. pH of the total mixture final mixture was maintained at 9.5 and
stirred over-night on ice. The solution was ultra-filtered three times, freeze-dried
and stored at 20 C.
For coupling between activated HB-PNIPAM-A-suc and FMoC-pmx-deacylate-B
DMF was used as a solvent and the reaction mixture stirred for two days at RT. 20%
piperidine aqueous solution was added during ultra-filtration to remove the FMoC
groups. The solution was ultra-filtered three times using de-ionized water and then
freeze-dried and stored at 20 C.
2.2.3. Photopolymerisation
Crosslinked hydrogel membranes were prepared as follows. The monomers,
NIPAM (6.75 g), glycidyl methacrylate (GME) (0.45 g) and ethandiol dimethacrylate
(EDMA) (1.8) were dissolved in Dioxane (5 ml) along with 2-hydroxy-2-methylpropiophenone (90 mg, 1 wt.% of total monomers). The mixture was added to
a polymerization mould and irradiated with a 200 arc 400 W mercury discharge lamp
at a distance of 10 cm in a Dimax model Bondbox on a rotating table for 2 min on each
side. The polymerization mould consisted of two 4 mm thick quartz glass sheets
covered with 100 mm PET film attached by the minimum amount of spray-mount
adhesive (3 M). The plates were separated with a rectangular 500 mm PTFE spacer and
the sheets were 125 mm 70 mm 5 mm when removed from the mould.
2.2.4. Modification of the membrane
Amine-functional membranes (10 g) were produced by soaking freshly prepared
membrane in ethanolic solution containing the 1,2-ethandiamine (250 ml, 5 vol.%)
in large excess for 24 h at room temperature. The operation was conducted in screwtop polypropylene bottles and membranes were washed several times with ethanol
and then IPA to remove excess diamine. HB-PNIPAM-van and HB-PNIPAM-pmx with
residual succinimide end groups were prepared as described below and the residual
succinimide groups were then reacted with the amine-functional membranes.
Functionalized HB-PNIPAM-van (100 mg) was dissolved in 20 cm3 water (this was
carried out over ice for 30e40 min), then the solution was transferred to a screw-top
polypropylene bottle. Pieces of amine-functional membranes (5 g) were added to it,
and then 5 ml of 0.1 M sodium phosphate buffer (pH 8.5) was added to the solution.
The pH of the final mixture was maintained at 9.5 and the mixture was stirred overnight over ice. The modified membranes were washed with water and IPA respectively several times and finally stored in IPA. For coupling between functionalized
HB-PNIPAM-pmx and amino functionalized membranes, IPA was used as a solvent
and the reaction mixture was stirred for two days at RT.
2.2.5. Synthesis of HB-PNIPAM-van or -pmx containing residual succinimide end
groups
Succinimide activated polymer (HB-PNIPAM-suc) (500 mg) was dissolved in
water (10 cm3) over ice and then Vancomycin (24 mg) in water (2 cm3) and sodium
phosphate buffer (0.1 M, pH 8.5, 5 cm3) were added. The pH of the mixture was
maintained at 9.5 and the mixture was stirred at 2e0 C over-night. The solution was
ultra-filtered three times and then freeze-dried and stored in a freezer. For coupling
between activated HB-PNIPAM and FMoC-pmx-deacylate, DMF was used as
a solvent and the reaction mixture was stirred for two days at RT. 20% piperidine
aqueous solution was added during ultra-filtration to de-protect the amine groups.
The solution was ultra-filtered three times using de-ionized water to remove DMF
and unreacted reagents and then freeze-dried and stored at 20 C.
2.2.6. Swelling of the membranes
The equilibrium water contents (EWC ¼ wet weight-dry weight/wet
weight 100) were determined gravimetrically in de-ionized water on cylindrical
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J. Shepherd et al. / Biomaterials 32 (2011) 258e267
samples cut using a cork borer. 6 sample disks per material were cut with a number
2 cork borer (6 mm diameter) and were hydrated over 12 h in ultrapure water.
The equilibrium water contents of the membranes at various stages were:
EWC (wt%)
As polymerized membrane
Amine-modified
VAN-functional
PMX-functional
26
27
33
34
2.2.7. Bacteria
Clinical isolates of S.aureus (S-235) and P.aeruginosa (SOM-1) were used as
representative Gram-positive and Gram-negative strains respectively. Bacteria were
cultured under standard conditions on brain heart infusion (BHI) agar (Oxoid), and
in BHI broth for experimental use. Following over-night incubation in broth, bacteria
were washed and resuspended in PBS to a concentration of 1 1010 cfu/ml.
2.2.8. Tissue engineered skin constructs
Constructs were produced as previously described [16]. Briefly, human dermal
fibroblasts and keratinocytes were isolated from split-thickness skin biopsies
received from abdominoplasties and breast reductions performed at the Northern
General Hospital, Sheffield. Research Ethics approval was obtained from the Sheffield Research Ethics Committee. Decellularised dermis (DED), (produced by
removing cells using 1 M NaCl as detailed in [16]) also sourced from human skin
biopsies, was used as a base scaffold. Rings of DED 15 mm in diameter were cut and
placed within 12 mm tissue culture inserts with 4 mm pores in the base (Greiner).
Inserts were suspended from the edges of 12 well plates into the wells. Greens’
medium containing 10% foetal calf serum was added to the bottom of the wells so
that it lapped the under surface of the DED. The DED was then seeded with 1 105
fibroblasts and 5 105 keratinocytes, each in 250 ml of 10% Greens medium. Again,
after 24 h incubation at 37 C, seeding medium was removed and replaced with
fresh Greens. After a further 24 h, medium was removed from inside the inserts in
order for the constructs to be at an aireliquid interface. Greens medium in the tissue
culture wells was replaced every 24 h and constructs were used for experimentation
after 14 days at aireliquid interface.
2.2.9. Infection of skin constructs
Constructs were washed in antibiotic-free Greens medium for 72 h prior to
infection. They were then burnt by the application of a heated metal rod, 4 mm in
diameter, for 6 s immediately prior to infection in order to provide the bacteria with
a mode of entry into the dermal tissue. 1 107 P.aeruginosa or S.aureus cells in 100 ml
PBS per construct were pipetted into the inserts covering the epidermal surface.
Infected constructs and non-infected controls were incubated in antibiotic-free
Greens medium at 37 C/5% CO2 for the required time.
2.2.10. Incubation of AMMA-labelled polymer with infected skin
After skin samples had been incubated with bacteria or PBS for 24 h, 100 ml of
AMMA-labelled polymer (5 mg/ml) or PBS was pipetted directly onto the surface of
the skin. Samples were incubated for 1 h at 37 C then imaged under UV light in
a G:Box gel documentation system (Syngene) using Genesnap software (Syngene).
900 ml PBS was then added to each sample and the supernatants aspirated into fresh
wells. Images were captured and processed on a Zeiss Axiovert 200 M inverted
fluorescence microscope using Axiovision Rel 4.6 software.
2.2.11. Histology and viable bacterial counts
Infected and non-infected constructs were bisected with sterile scalpels. Half of
the sample was fixed in 10% formalin for >24 h then processed and paraffin
embedded for histological analysis. The other half was weighed, then the tissue
homogenised in 1 ml BHI broth. The resulting homogenates were diluted serially
and used to perform viable counts of bacteria in the samples. Formalin fixed, paraffin
embedded samples were sectioned to 6 mm thick on a microtome. Sections were
stained with haematoxylin and eosin using standard techniques, and also Gram
stained to visualise bacteria, again using standard techniques.
2.2.12. Bacterial attachment to hydrogel membranes
Circular discs, 6 mm in diameter, of HB-PNIPAM-van hydrogel membrane,
HB-PNIPAM-pmx hydrogel membrane or control HB-PNIPAM-COOH membrane
were incubated with 100 ml S.aureus or P.aeruginosa at 1 1010 cfu/ml in PBS for 1 h
at 37 C. Following incubation, membranes were washed in PBS to remove nonadherent bacteria and viewed under phase-contrast microscopy using a Zeiss
Axiovert 200 M inverted microscope. Images were captured using Axiovision Rel 4.6
software and numbers of visible bacteria adhered to the membranes counted (n 5
images per membrane).
2.2.13. Live/dead staining of bacteria
Membranes were incubated with 1 ml/ml Syto9 (Invitrogen) and 4 ml/ml propidium iodide for 20 min at room temperature, washed 4 times in PBS then viewed
under fluorescence microscopy as above.
2.2.14. Membrane application to skin constructs
Skin constructs were burnt as above and 1 107 cfu S.aureus or P.aeruginosa
pipetted onto this wound, or PBS as control. Constructs were incubated for 45 min
or 24 h at 37 C, then circular discs of HB-PNIPAM-van or epmx-B or eCOOH
hydrogel membrane, 6 mm in diameter, were applied to the surface of the skin
and incubated for 3 h at 37 C. Discs were removed and replaced with a fresh disc
every hour. Bacteria adherent to the membranes were counted, viable bacteria
remaining in the tissue sample quantified and tissue sections Gram stained as
above.
3. Results
3.1. HB-PNIPAM-AMMA-pmx and HB-PNIPAM-AMMA-van
solutions in contact with bacteria in an infected skin model
Burn wounds in tissue engineered human skin were created.
Uninfected controls were burned and incubated with PBS (a,b,c).
Constructs were infected with P.aeruginosa (Fig. 1d, e, f) or
S.aureus (Fig. 1g, h, i) as described previously [16]. After 24 h
infection with bacteria and rinsing in PBS to remove unattached
bacteria, 100 ml of polymer incorporating anthracene as a fluorescent marker (HB-PNIPAM-AMMA-pmx or HB-PNIPAM-AMMAvan) in solution (or PBS control) was pipetted directly onto the
skin surface and incubated at 37 C for 1 h. Skin samples were
then visualised under UV light. In samples which had been
burned (Fig. 1a), infected with P.aeruginosa and incubated with
HB-PNIPAM-AMMA-pmx, bright areas of AMMA fluorescence
were seen in the areas of the burn injury (Fig. 1d), which
microscopy showed to be the location of the highest concentration of bacteria. This was also the case for HB-PNIPAM-AMMAvan incubated with S.aureus infected skin (Fig. 1i). We also tested
burned, uninfected samples to ensure that polymers were not
simply attaching to burn injury-exposed extracellular matrix
components such as fibronectin, which is known to be adhesive.
In those samples there was no visible fluorescent area (Fig. 1b, c).
Similarly, burned infected samples incubated with PBS rather
than polymer showed no fluorescent areas (Fig. 1e, h).
We then added a further 900 ml of PBS to each sample to
aspirate polymer away from the skin. Examination of the resulting suspensions under a fluorescence microscope revealed that in
eluates from infected samples clusters of fluorescent polymer
were visible, but there were no clusters in eluates from uninfected skin (not shown). These findings, again indicate polymer
collapse only in samples where the polymers had contacted the
bacteria.
We hypothesised that attachment of the polymer to bacteria in
the infected skin model and its subsequent removal could physically debulk the bacterial load from the skin. Consequently,
following infection and incubation with polymers or PBS as above,
each sample was bisected and half examined histologically, while
the other half was assessed for the bacterial viable count. In addition, the PBS wash supernatants were also serially diluted and
counted.
Histological analysis of the skin sections revealed that in
infected samples incubated with PBS alone, a large number of
bacteria were present particularly in the upper layers of the skin
(Fig. 2a, e), in line with previous findings [16]. However, in
samples that had been incubated with the appropriate polymer
and the polymer then removed, there was a striking reduction in
visible bacteria (Fig. 2b, f). Viable counts of bacteria present in the
tissue samples confirmed this, showing a decreased number of
bacteria present in those samples treated with polymer compared
to those incubated with PBS alone (Fig. 2c, g). Also, the washed
supernatants from the skin samples that had been incubated with
polymer showed a higher number of bacteria than the supernatants from non-polymer treated tissue samples (Fig. 2d, h).
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261
Fig. 1. Anthracene-labelled polymer fluoresces on incubation with bacterial infected human tissue engineered skin (a) Gross view of burned skin construct within tissue culture
insert. Arrow indicates injured area of epidermis. (b) and (c) Burned uninfected skin incubated with HB-PNIPAM-AMMA-pmx and HB-PNIPAM-AMMA-van respectively and viewed
under UV light. (d), (e) and (f) Burned skin infected with P.aeruginosa and incubated with HB-PNIPAM-AMMA-pmx, PBS, and HB-PNIPAM-AMMA-van respectively. (g), (h) and (i)
Burned skin infected with S.aureus and incubated with HB-PNIPAM-AMMA-pmx, PBS, and HB-PNIPAM-AMMA-van respectively. Arrow in (d) and (i) indicates bright spot which is
the location of the burn injury.
3.2. Gram-positive and gram-negative bacteria binding to
HB-PNIPAM-van or HB-PNIPAM-pmx hydrogel membranes
Hydrogels were incubated with 100 ml S.aureus or P.aeruginosa at
1 1010 cfu/ml in PBS for 1 h at 37 C. Following incubation,
membranes were washed in PBS to remove non-adherent bacteria
and viewed under phase-contrast microscopy. Images were
captured and numbers of visible bacteria adherent to the
membranes counted (n 5 images per membrane). Visibly more
S.aureus were bound to the HB-PNIPAM-van membrane as
compared to control membrane, or P.aeruginosa bound to
HB-PNIPAM-van membrane (Fig. 3aec). In contrast, P.aeruginosa
bound preferentially to HB-PNIPAM-pmx membrane (Fig. 3f).
Quantification of bacterial numbers demonstrated a significantly
higher number of S.aureus bound to HB-PNIPAM-van membrane,
and P.aeruginosa bound to HB-PNIPAM-pmx membrane, than any
other test group (Fig. 3g). We then investigated whether bacteria
bound to the hydrogel membranes were being killed or were
merely being immobilised by binding to the membranes. To do this
we performed live/dead staining over a 24 h time course, which
differentiates between live and dead bacteria according to uptake
of fluorochromes. Quantification of the percentage of live vs. dead
bacteria revealed that the majority of bacteria were viable even
after being adherent to either polymer for 24 h (Fig. 3h). Viable cells
attached to membranes displayed little (P.aeruginosa) or no
(S.aureus) growth over 24 h after incubation of the membranes at
37 C in optimal growth medium (Fig. 3i), and appeared to form
a biofilm without a substantial release of bacteria into the
surrounding medium, as indicated by the minimal increase in
optical density of the growth medium compared to ‘free’ bacteria
over the same time period (Fig. 3j). In contrast, previous studies
with free antibiotic show that exposure to Vancomycin for 8 h
would normally result in a 1e3 log decrease in viable bacteria, and
at least a 2 log drop in numbers of P.aeruginosa treated with Polymyxin-B for 2 h [18e20] (i.e. >99% decrease).
From the above findings we reasoned that physical binding of
superficial bacteria in the wounded, infected skin model to the
membrane might result in removal of bacteria when the membrane
was removed. Consequently, after 45 min incubation at 37 C with
1 107 cfu S.aureus or P.aeruginosa to allow attachment to burn
wounded models but not invasion of the tissue, circular discs of
HB-PNIPAM-van or -pmx hydrogel membrane were applied to the
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J. Shepherd et al. / Biomaterials 32 (2011) 258e267
Fig. 2. Bacterial numbers are reduced in infected skin samples after incubation with HB-PNIPAM-AMMA-pmx or HB-PNIPAM-AMMA-van Gram stained sections of paraffin
embedded burned skin were infected with P.aeruginosa, and incubated with either (a) PBS (control) or (b) HB-PNIPAM-AMMA-pmx polymer. Arrows in (a) indicate large numbers of
Gram-negative bacteria present in upper layers of skin. Scale bar ¼ 200 mm. (c) Numbers of viable bacteria cultured from P.aeruginosa-infected skin tissue (n ¼ 7). (d) Numbers of
viable bacteria cultured from supernatant of infected skin samples (n ¼ 5). Error bars ¼ SEM. (eef) Gram stained sections of paraffin embedded burned skin infected with S.aureus,
and incubated with either (e) PBS (control) or (f) HB-PNIPAM-AMMA-van polymer. Arrows in (e) indicate large numbers of Gram-positive bacteria present in upper layers of skin.
Scale bar ¼ 200 mm. (g) Numbers of viable bacteria cultured from S.aureus infected skin tissue (n ¼ 5). (h) Numbers of viable bacteria cultured from supernatant of infected skin
samples (n ¼ 4). Error bars ¼ SEM.
surface of the skin and incubated for 3 h at 37 C. The discs were then
replaced hourly for 3 h. As shown in Fig. 4a numbers of S.aureus
adherent to HB-PNIPAM-van membranes were significantly higher
than those adherent to control membranes, or P.aeruginosa adherent
to HB-PNIPAM-van membranes. Also, numbers of S.aureus adherent
to HB-PNIPAM-van membranes increased with each application of
membrane (Fig. 4a). Numbers of P.aeruginosa bound to HB-PNIPAM-
pmx membranes were also higher than those bound to control
membranes, but less bacteria were found bound with each application of fresh membrane (Fig. 4b). We suspect that this is due to the
superior ability of P.aeruginosa to penetrate into the dermis out of
reach of the membranes at the surface, thus P.aeruginosa was clearly
visible within the dermis (Fig. 4e, f) Fig. 4cef show corresponding
sections of skin models stained for bacteria.
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J. Shepherd et al. / Biomaterials 32 (2011) 258e267
263
Fig. 3. Bacteria adhere to HB-PNIPAM-van and -pmx on a hydrogel membrane and remain viable over 24 h Phase-contrast microscopy images of (a) S.aureus adhered to HBPNIPAM-van hydrogel membrane and (b) control membrane, (c) HB-PNIPAM-pmx hydrogel membrane, and P.aeruginosa adhered to HB-PNIPAM-van (d), HB-PNIPAM-COOH (e) and
HB-PNIPAM-pmx (f) hydrogel membranes. Numbers of adherent bacteria to each type of membrane are quantified in (g). Percentages of dead cells adhered to membrane at time
points up to 24 h incubation are quantified in (h). Viable cells attached to membranes displayed a greatly reduced growth rate over 24 h (i), and were not released into the growth
medium as evidenced by the negligible increase in optical density of the medium (j). Scale bars ¼ 20 mm. Error bars ¼ SEM.
The number of viable bacteria remaining in the tissue samples
following membrane treatment was also quantified (Fig. 4g). In this
case, numbers of S.aureus were much lower in HB-PNIPAM-van
membrane-treated samples compared to those treated with control
membranes. Conversely, numbers in tissue samples treated with
control membrane did not decrease with time. P.aeruginosa-infected
skin treated with HB-PNIPAM-pmx membranes also contained less
bacteria than control treated models, and the number of viable
bacteria remained stable with each round of HB-PNIPAM-pmx
membranes (Fig. 4h), whereas high numbers of bacteria were
present at 3 h in the models treated with the control membranes.
Again, we believe that this is due to the penetration of P.aeruginosa
into the dermis. Gram stained paraffin sections of the infected skin
samples showed less visible bacteria in skin treated with HB-PNIPAM-van membranes than those with control membranes (Fig. 4c,d).
In order to observe the effects of the HB-PNIPAM-van
membranes on skin constructs with a more established bacterial
infection, skin constructs were burnt and then infected with
1 107 cfu S.aureus or P.aeruginosa as above. After 24 h incubation
at 37 C to allow infection of the skin, circular discs of HB-PNIPAMvan or eCOOH control hydrogel membrane were applied to the
surface of the skin as before and incubated for 3 h at 37 C. Discs
were replaced hourly. Again, numbers of S.aureus adherent to HBPNIPAM-van membranes were significantly higher than those
attached to control membranes or P.aeruginosa attached to
HB-PNIPAM-van membranes (Fig. 5a). In this case however, the
number of S.aureus adherent to HB-PNIPAM-van membrane
decreased with each sequential application. We propose that this is
due to the longer infection period (24 h vs. 45 min), which allows
a higher proportion of the bacteria to penetrate into the dermis
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J. Shepherd et al. / Biomaterials 32 (2011) 258e267
Fig. 4. S.aureus and P.aeruginosa are reduced in infected skin after application of HB-NIPAM-van or epmx-B on a hydrogel membrane (a) Numbers of bacteria adherent to the HBPNIPAM-van membrane (n ¼ 5), (b) numbers of bacteria adherent to the HB-PNIPAM-pmx membrane (n ¼ 5), (c) Gram stained section of S.aureus infected tissue after two 1-h
applications of HB-PNIPAM-van membrane, (d) Gram stained section of S.aureus infected tissue after two 1-h applications of HB-PNIPAM-COOH control membrane. (e) Gram stained
tissue infected with P.aeruginosa after 3 hourly applications of HB-PNIPAM-COOH control or HB-PNIPAM-pmx membrane (f). (g) Viable S.aureus bacteria remaining in tissue
following membrane treatment (n ¼ 5), (h) viable P.aeruginosa remaining in tissue following membrane treatment (n ¼ 5). Error bars ¼ SEM. Arrows indicate representative
bacteria. Scale bars in c and d ¼ 200 mm, in e and f ¼ 50 mm.
therefore out of reach of the membrane. In this case, over the 3 h
treatment period the membranes remove surface bacteria available
to them, the numbers of which decrease with each application.
After a 45 min infection the numbers of adherent bacteria increase
with each application since they are presumably multiplying at the
skin surface at that early point.
Viable counts of bacteria remaining in tissue following HBPNIPAM-van membrane treatment showed a decreased number of
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J. Shepherd et al. / Biomaterials 32 (2011) 258e267
265
Fig. 5. S.aureus are reduced in infected skin after application of HB-PNIPAM-van on a hydrogel membrane following 24 h infection (a) Numbers of bacteria adherent to membranes
(n ¼ 5), (b) numbers of viable bacteria remaining in tissue after application of membranes (n ¼ 5), c) and d) Gram stained tissue infected with S.aureus for 24 h after 3 hourly
applications of HB-PNIPAM-van (c) or HB-PNIPAM-COOH control (d) membrane. Error bars ¼ SEM, scale bar ¼ 200 mm.
S.aureus within the tissue at all time points compared to control
membrane-treated samples (Fig. 5b). Rather than decreasing with
each sequential application however, the numbers of S.aureus
remained at a similar lowered level throughout the 3 h test period,
as with the P.aeruginosa/HB-PNIPAM-pmx membrane 45 min
incubation experiments. Again we surmise this is due to bacterial
invasion of the dermis away from the membrane at the surface.
Indeed, Gram staining of skin samples reveals that surface bacteria
are removed in samples treated with HB-PNIPAM-van membrane
compared with control membranes, but that some bacteria are
found deeper within the dermis (Fig. 5c,d).
4. Discussion
In this study, we describe the application of HB-PNIPAMs that
are capable of selectively binding to either Gram-positive or Gramnegative bacteria in an in vitro infected human skin model. We
demonstrate that they reduced the bacterial load in the model
when added to the surface and subsequently removed some hours
later. If these were incorporated in dressings they could be
compatible with current wound care management practices.
PNIPAM has an LCST of 32 C, whereas HB-PNIPAM-van has an
LCST of above 60 C [3]. However, the LCST is reduced on binding to
the target bacteria. By modifying the highly branched polymer with
the addition of antibiotic end groups we have successfully altered
the LCST so that binding of the appropriate bacteria at body
temperature causes polymer collapse and consequent aggregation
of bound bacteria. The key feature of these systems is that the
binding-induced coil-to-globule transition converts the PNIPAM
into a substrate to which bacteria are known to adhere. The bacteria
are attached to the polymers by both the specific multiple binding
interactions and the favourable physico-chemical environment
provided by PNIPAM in the globule state. Bacteria are thereby
‘collected’ by binding to the polymer. This polymer could also be
tethered onto diverse surfaces including wound dressings. There is
no need to alter the temperature to induce these modified
polymers in solution to collapse as the trigger is now the binding of
the bacteria, which occurs over a temperature range compatible
with wound management. Although we currently have no direct
evidence for polymer collapse in hydrogel membranes, the modified polymers bound to solid hydrogel supports are also capable of
binding bacteria in the infected wound model as discussed shortly.
Although greatly reduced in number, viable bacteria were left
within the tissue following application of polymer in solution, and
we assume that in its current form the polymer can only debulk the
wound bed at areas where it is in direct contact with bacteria, i.e.
the upper surface layers. However, any reduction in bacterial load is
encouraging. We found that skin samples incubated with soluble
polymer had a significantly higher number of bacteria present
within the washed supernatant than those incubated with PBS
alone. We suggest that this is due to bacterial attachment to polymer, resulting in bacteria being washed away from the surface of
the samples along with the polymer. Since simple washing-off of
the polymer/bacteria complexes is sufficient to remove large
numbers of bacteria from the skin, this supports the potential for
the polymer to be applied as a clinically undemanding wound
dressing.
We hypothesised that repeated applications of the polymer to
the same infected injury may result in an even more dramatic
reduction in bacterial numbers. This would be the case in real-life
situations, where wound dressings are changed regularly. Unless
a patient is severely immunocompromised, the reduced numbers
of bacteria remaining in the tissue could also be more effectively
targeted by the patient’s own immune system than the larger
numbers present pre-treatment with polymer. To simultaneously
examine whether repeated applications of the polymer would
indeed lead to reduced bacterial numbers within the skin samples,
and to investigate the effectiveness of the polymer after attachment
to a fixed surface, we created solid hydrogel membranes with either
HB-PNIPAM-van, -pmx or control eCOOH attached. To examine
the effect of hydrogel polymer on surface bacteria in a wound,
after a short (45 min) incubation with S.aureus or P.aeruginosa
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post-injury we found that numbers of S.aureus adherent to HBNIPAM-van membrane increased with each application of
membrane, indicating enhanced bacterial removal with each
subsequent round. This was supported by the decreasing numbers
of viable bacteria remaining in the tissue after each application of
HB-NIPAM-van. On the other hand, viable numbers of bacteria
remaining in tissue after application of control membrane
increased over the 3 h time period, indicating uncontrolled bacterial cell division over the course of the experiment. These data
suggest that the hydrogel polymer is effective at removal of bacteria
from the uppermost surfaces of wounds. In addition, specificity for
Gram-positive organisms was confirmed as only low numbers of
Gram-negative P.aeruginosa were adherent to the membrane. The
opposite was true with HB-PNIPAM-pmx membrane, to which only
low numbers of S.aureus adhered.
Conversely, after a longer incubation with S.aureus post-injury,
to simulate an established wound infection, the numbers of
S.aureus adherent to HB-PNIPAM-van membrane decreased with
each sequential application, presumably as each round of
membrane application lowered the numbers of bacteria available
near the surface to bind to the membrane. Numbers of S.aureus
adherent to HB-PNIPAM-van membrane were significantly higher
than those attached to control membrane, or P.aeruginosa attached
to HB-PNIPAM-van membrane, only after 1 h since the total
adhered diminished with each application to become closer to the
control levels. The viable S.aureus remaining in the HB-PNIPAM-van
treated tissue were reduced in number compared to control treated
samples but remained fairly constant throughout. We assume that
the membrane was able to remove the majority of the S.aureus from
the surface of the wound but could not reach bacteria that had
penetrated deeper into the tissue. These results mirrored those
found for skin infected with P.aeruginosa for 45 min, which displays
a greater capability for penetration into the dermis. Our previous
findings with S.aureus infection in our skin model demonstrated
that at 24 h post infection, the bulk of S.aureus remain located in the
upper layers of the skin constructs, so we propose that particularly
in the case of S.aureus infection, the greater part of the bacterial
load could be removed by the polymer. Taken together, the data
from the membrane experiments indicated that the polymer would
be most efficacious if applied as rapidly as possible to the wound
surface after injury, before bacteria are able to infect deeper tissue
layers.
Hydrogels have become increasingly used as wound dressings
since their inception in the 1960s [21] due to their multiple desirable qualities, which include biocompatibility, relative low-cost,
and ability to be applied in various forms such as gels or on gauze
dressings [22,23]. In fact, after 24 h infection and 1 h application of
polymer, HB-PNIPAM-van on hydrogel membranes was slightly
more efficient at clearing viable bacteria from the tissue, leaving
w500 cfu/mg compared to w1250 cfu/mg with the same polymer
in solution (Fig. 5b c.f Fig. 3g).
In previous published studies, other materials employing antibiotics linked to polymers have been developed [24e29]. In these
materials ‘entire’ antibiotics are used and in some cases released,
which could contribute to the development of antibiotic resistance.
In our study Polymyxin-B was modified so that only the part of the
molecule that binds bacteria is present, rendering it non-microbicidal. Data for HB-NIPAM-van indicate that even after 24 h
exposure to the polymer, the majority of bacteria remain alive
suggesting that the antibiotic cannot access sufficient target sites to
kill bacteria presumably because it is tethered to the polymer. Also,
this is likely to reduce markedly any potential contribution to
selection of bacterial resistance and S.aureus growth on the
hydrogel membrane was restricted to a slow-growing biofilm that
did not appear to propagate into the growth medium. These are
important considerations given the rise in antibiotic resistance over
recent years and the natural propensity of bacteria to rapidly evolve
resistance mechanisms.
Ruiz et al. [30] recently described work in which Vancomycin
was loaded onto a PNIPAM-modified polypropylene surface for use
in medical implantation devices, in order to prevent biofilm
formation. In this case, PNIPAM-grafted polypropylene films were
soaked in Vancomycin solutions then dried. Under physiological
conditions of temperature and pH, the PNIPAM mesh shrinks and
releases the antibiotic. Consequently the former acts as a drug
delivery device, similar to commercially available products such as
wound dressings delivering topical polymyxin-B sulphate and
bacitracin zinc to the wound, available without prescription in the
United States of America [31]. These are in contrast to the current
bacterial binding system that we have developed.
5. Conclusions
In this study we demonstrate that stimulus-sensitive polymers
can significantly deplete viable bacteria in a 3D tissue engineered
model of infected human skin, by simple application and subsequent washing-off of the polymer. HB-NIPAM-van and -pmx can
also be effectively immobilised onto the surface of biocompatible
hydrogels, with no loss of the polymers’ wound debulking capabilities. Bacteria-sensitive polymers which have the capability to
physically remove pathogens from infected wounds, without
harming healthy tissue or contributing to selection of antibiotic
resistance have enormous potential. Such polymers could be used
to coat wound dressings, or be used for other topical applications,
as well as for the removal of bacteria from liquid systems or
surfaces.
Acknowledgments
We thank DSTL and EPSRC for funding.
Appendix
Figures with essential colour discrimination. Figs. 1 and 3 in this
article may be difficult to interpret in black and white. The full
colour images can be found in the on-line version, at doi:10.1016/j.
biomaterials.2010.08.084.
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