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Although most chronic wounds possess an underlying pathology, infectious agents also contribute. In many instances, pathogens exist as biofilms forming clusters surrounded by a secreted extracellular substance. We hypothesized that compounds secreted by biofilm bacteria may inhibit normal wound healing events including cell proliferation and migration. Conditioned media from two common bacterial species associated with chronic skin wounds and chronic tympanic membrane perforations, Staphylococcus aureus and Pseudomonas aeruginosa, were evaluated for their capacity to affect keratinocyte proliferation and migration. Additionally, proteomic analysis was performed to identify proteins within the biofilm conditioned media that may contribute to these observed effects. Biofilm conditioned media from both species inhibited proliferation in human tympanic membrane derived keratinocytes, whereas only biofilm conditioned media from S. aureus inhibited migration. Human epidermal keratinocytes were found to be more sensitive to the effects of the conditioned media resulting in high levels of cell death. Heat treatment and microfiltration suggested that S. aureus activity was due to a protein, while P. aeruginosa activity was more likely due to a small molecule. Proteomic analysis identified several proteins with putative links to delayed wound healing. These include alpha hemolysin, alcohol dehydrogenase, fructose-bisphosphate aldolase, lactate dehydrogenase and epidermal cell differentiation inhibitor.
The primary function of the skin is to serve as a barrier to the external environment. Wound healing of the skin is a complex process involving cellular proliferation, migration and tissue remodelling leading to reestablishment of its primary function. Failure of a wound to heal in a timely manner may lead to further complications, including septicemia, chronic pain, prolonged hospitalization, amputations, and mortality1. Chronic wounds in humans include wounds of the lower limb, due to an underlying pathology such as diabetes, pressure or venous hypertension, and chronic tympanic membrane perforations typically caused by chronic suppurative otitis media. Bacteria are present in chronic wounds and are proposed to play a role in delayed tissue repair2,3.
It is considered that the bacteria present in chronic wounds not only exist in a planktonic form, but are also characterized by polymicrobial colonies of bacteria existing in communities known as biofilms4. Biofilms consist of a cluster of bacteria adhering to a surface surrounded by an extracellular polymeric matrix5. The function of the biofilm is varied and includes protection from the environment, nutrient storage and aiding in cell-cell communication. Consequently, gene expression and phenotype of bacteria in biofilm mode is different to that when in free living or planktonic mode6,7. The presence of a biofilm in chronic wounds gives rise to several common features; they render the bacteria virtually impervious to antibiotic treatments8 and affected tissues remain in a persistent inflammatory state1. Additionally, it has been shown that the presence of a biofilm can delay wound healing9. However, the mechanisms of delayed wound healing due to biofilms are poorly understood.
We hypothesize that bioactive compounds secreted by bacteria whilst in biofilm mode inhibit key wound healing mechanisms including cell proliferation and migration. Therefore, the aims of this research were to grow isolates of bacteria in biofilm mode and planktonic mode and produce conditioned media. We have selected perhaps the two most common bacterial species related to chronic wound colonization or infection, Pseudomonas aeruginosa and Staphylococcus aureus. In vitro cell culture was then used to compare the effects of secreted biofilm and planktonic compounds on key wound healing events, cell proliferation and migration. For this purpose we utilized human derived primary keratinocytes from two distinct areas, the tympanic membrane and the normal epidermis of the upper arm. Subsequently, proteomic analysis was undertaken to identify potential protein products responsible for any observed effects.
A 10% dilution of biofilm conditioned media (BCM) and planktonic conditioned media (PCM) from S. aureus and P. aeruginosa were examined for their effect on cell proliferation in vitro. Included controls were a 10% dilution of tryptic soy broth (TSB) plus a positive control of cell culture media (DMEM+) only (Fig. 1). Compared to the TSB media control, PCM of both P. aeruginosa and S. aureus had no significant effect on cell proliferation in human tympanic membrane keratinocytes (hTMks) (Fig. 1a). In contrast, BCM from P. aeruginosa completely inhibited proliferation in hTMks with an absorbance reading equivalent to that of seeded cells with no proliferation period (data not shown). For S. aureus BCM, proliferation in hTMks was significantly reduced to approximately 71±5.4% of the TSB media control (p0.001).
In hEKs, (Fig. 1b) the BCM was diluted further to 5% due to high levels of cellular death seen with a 10% dilution. At 5% dilution, the PCM of S. aureus produced a significant decrease in proliferation (p=0.0025) to 76% of the TSB control while the PCM from P. aeruginosa showed no significant effect (p=0.7). Additionally, the BCM from S. aureus also significantly reduced proliferation to 30.3±5.7% of the TSB control (p0.01), while BCM from P. aeruginosa significantly (p=0.003) reduced proliferation to 48.3±12.4% of the TSB control.
The effect of diluted PCM and BCM on cell migration was examined (Fig. 2). In hTMks, PCM from S. aureus and P. aeruginosa plus BCM from P. aeruginosa had no significant effect on migration compared to the TSB media control (p=0.27, 0.29 and 0.72 respectively) (Fig. 2a). However, the BCM of S. aureus significantly reduced migration to 9.8±7.2% of the media-only control and approximately 13% of the TSB media control (p0.01) in this cell type.
In hEKs (Fig. 2b), the TSB media and PCM from P. aeruginosa seemed to accelerate migration to over 300% of the media-only control. However, the BCM from P. aeruginosa appeared to be highly cytotoxic.
Under microscopy, control hEKs stained with crystal violet exhibited the characteristic cobblestone appearance of keratinocytes (Fig. 3a). When treated in 5% P. aeruginosa BCM for the duration of the migration experiment (15hours) a large proportion of the cells were killed and appeared contracted (Fig. 3b). The PCM of S. aureus (Fig. 3c) resulted in a reduced number of cells with altered morphology, which appeared to be losing close contact with their neighbours. Treatment with BCM of S. aureus resulted in highly reduced cell numbers (Fig. 3d). In addition, the presence of apoptotic cells appeared to be evident (Fig. 3d, arrow heads). It was therefore not possible to interpret these results in terms of altered migration. However, the observations indicate that hEKs are more sensitive to conditioned media than hTMks.
Only hTM-derived keratinocytes were used for analyses.
As the PCM has no observable effect on hTMks proliferation, it was excluded from this experiment. Heat treatment completely abrogated all anti-proliferative activity of S. aureus BCM, which showed no significant difference to the TSB media control (p=0.97). However, heat treatment had no effect on the anti-proliferative activity of P. aeruginosa BCM (Fig. 4a).
Similar to proliferation, heat treatment of S. aureus BCM removed the ability to inhibit migration (Fig. 4b), which showed no significant difference to the TSB control (p=0.23). Heat treated BCM from P. aeruginosa also demonstrated no significant difference compared to TSB control (p=0.19), similar to its untreated form.
Fractionating the samples using a 3KDa filter showed all the anti-proliferative activity of S. aureus was found in the filtrate (p0.01), with no significant (p=0.45) activity found in the flow through fraction (Fig. 5a). By contrast, P. aeruginosa activity was primarily in the flow through fraction with significant activity (p=0.002) also detected in the filtrate. However, this activity was significantly less than that of the flow through (p0.01).
Only BCM from S. aureus was tested (Fig. 5b) due to lack of activity in P. aeruginosa conditioned media. Similar to the effects on proliferation, the inhibitory effect of S. aureus on cellular migration was found only in the filtrate, which was significantly reduced to 40±26.1% of the TSB control (p=0.019). No significant activity (p=0.255) was recorded for the flow through fraction.
PAGE analysis was performed on the BCM and PCM for both bacterial species. No protein bands were detectable in the TSB media control or PCM (gel not shown). In the BCM gel (Fig. 6), raw BCM from P. aeruginosa and S. aureus (Lanes 2 and 5 respectively) produced several discernable bands ranging in size from approximately 12KDa to 80KDa. Samples of flow through following fractionation were also included (lane 3 and 6) along with samples of the filtrate (Lane 4 and 7) for P. aeruginosa and S. aureus respectively. All proteins were retained in the filtrate. Six identifiable bands from S. aureus (arrows) were removed from the gel for peptide sequencing and identification. These are summarized in Table 1. Identification of proteins from P. aeruginosa BCM was not performed due to the inability of heat treatment to abrogate its effect and lack of activity in the protein fraction. These results suggest that activity was not due to a protein.
In this study, conditioned media derived from P. aeruginosa and S. aureus cultured as biofilms were examined for their ability to disrupt the normal wound healing processes of cell proliferation and migration. Keratinocytes from the tympanic membrane (TM) and the normal skin epidermis from the upper arm were chosen for the in vitro analysis due to their different healing patterns. When the dermis heals in response to injury, it undergoes sequential phases of haemostasis, inflammation, cellular proliferation, and finally cellular migration. In TM wound healing, the first two stages remain, but migration precedes proliferation10.
For hTMks, at the 10% dilution tested, BCM from S. aureus was capable of a modest reduction in proliferation, while it completely inhibited cellular migration. Conversely, the BCM of P. aeruginosa appeared to only affect proliferation with no significant effect on migration. However, the PCM from both species had no significant effect on either proliferation or migration. The hEKs appeared to be far more sensitive to the conditioned media. At 10% dilution, BCM from both species was highly toxic, effectively killing the hEKs in both migration and proliferation tests. However, when reduced to 5% dilutions a clear inhibitory effect on proliferation was seen. The BCM of both species significantly reduced the level of proliferation compared to the TSB control, with S. aureus BCM appearing to have a larger effect than that of P. aeruginosa. However, a comparison between S. aureus and P. aeruginosa BCM was found to be not significant (p=0.083). In addition, the PCM of S. aureus also caused a significant decrease in proliferation, but was much less potent than the BCM. On the other hand, migration was more difficult to interpret. Both the PCM and BCM of S. aureus had a toxic effect on hEKs in addition to the BCM of P. aeruginosa (Fig. 3a–d). Therefore, meaningful migration results could not be firmly established. However, it should be noted that the PCM of P. aeruginosa had no significant effect compared to the TSB control, although both seemed to increase the rate of migration compared to the cell culture media only control.
Previous studies using cultured cells have examined the effects of PCM and BCM derived from S. aureus. Using wound scratch assays, both were found to significantly reduce gap closure in keratinocytes and fibroblast cells11,12. However, a difference in cell morphology was noted between PCM and BCM treated cells indicating potentially different mechanisms of action. Similarly, both PCM and BCM resulted in reduced viability in both cell types with the BCM being significantly more potent than PCM, which was also reflected in our studies using hEKs, but this did not seem the case in hTMks. For apoptosis, BCM and PCM possessed equal potency in fibroblasts12. However, in keratinocytes, BCM treatment caused significantly higher levels of apoptosis than PCM11, which was also suggested in our experiments. In the case of P. aeruginosa, much exists in the literature regarding the presence of biofilm in wounds and their effects. However, no similar in vitro studies into effects on proliferation and migration have been performed.
In an effort to determine which components of the BCM were exerting the effects seen, further analyses were performed on hTMks. Heat treatment and microfiltration on the BCM revealed the most likely cause for the effects seen for S. aureus was a secreted protein. This was based on heat treatment completely abrogating all S. aureus BCM effects, presumably due to denaturation. Similarly, after filtering the BCM with a 3KDa cut-off, the majority of activity was preserved in the filtrate and not the flow through, which is suggestive of a retained, and relatively large molecular weight protein and not a small molecule. On the other hand, the effects caused by P. aeruginosa BCM appeared to be caused by a small molecule due to the ineffectiveness of heat treatment and the anti-proliferative effect being seen within the flow through fraction following microfiltration.
To further establish possible bioactive components of the conditioned media, SDS PAGE was performed. This revealed a complex pattern of secreted proteins for both P. aeruginosa and S. aureus BCM. As the data suggested only S. aureus activity was due to a protein(s), six of the more prominent S. aureus protein bands were excised from the gel and identified (Table 1). A number of identified proteins including transketolase, triosephosphate isomerase, purine nucleoside phosphorylase and glucosamine-6-phosphate deaminase are typically involved with essential metabolic processes with no known link to wound healing. However, of the proteins identified, several have been previously implicated in delayed wound healing and/or cell death and may be contributors to the effects seen in this study. These proteins include alpha hemolysin, a highly studied S. aureus cytotoxin that is particularly potent in lysing rabbit erythrocytes. In addition, it is also known to be dermonecrotic and neurotoxic13. Alcohol dehydrogenase (AD) may also require further study. Currently, no explicit reports on the direct effects of this enzyme with respect to wound healing have been reported. However, there exists anecdotal evidence that suggests the presence of AD may have a negative impact on wound healing. A transcriptome microarray study on healing tympanic membranes in rats revealed AD to be the most potently downregulated gene in the first 12hours following an induced perforation14. Other studies have shown that ethanol exposure prior to injury may inhibit normal wound healing processes and have suggested the presence of ethanol itself plus its metabolites to be the likely cause15,16. However, the effects of elevated levels of AD were overlooked on these occasions. Therefore, combined with current data it is possible to consider that the presence of AD may also cause a negative impact on early wound healing processes. Fructose-bisphosphate aldolase (ALDOA) is a glycolytic enzyme and has been shown to directly bind to actin filaments of the cytoskeleton and modulate polymerization17. In keratinocytes, endogenous ALDOA is involved in forming actin based lamellipodia, which are structures important for cell migration18. Therefore, its plausible that exogenous ALDOA from S. aureus biofilm may alter the actin polymerisation process leading to a downstream effect in cell migration. Lactate dehydrogenase is an enzyme that reversibly converts lactate into pyruvate. In a healing environment, lactate accumulation stimulates the production of growth factors such as VEGF19 and TGF ß20 and is capable of enhancing cellular migration21. Similar to ALDOA, exogenous lactate dehydrogenase would effectively remove lactate from the wound environment and potentially reduce the pro-healing effects. Another interesting candidate identified was epidermal cell differentiation inhibitor (EDIN) protein. EDINs are able to ADP-ribosylate members of the Rho GTPase family causing their inactivation22. Inhibition of the Rho GTPase Rac1 results in disturbed migration of keratinocytes both in vitro and in vivo23. Additionally, EDIN produces a loss of barrier function in endothelial cells through actin cable disruption leading to the formation of microapertures. This provides direct access of the endothelium basement membrane to S. aureus bacterium24. Furthermore, EDIN genes from S. aureus strains have also been found to correlate to higher grade diabetic foot ulcers25. However, in this instance the presence of biofilm was not established.
In terms of wound healing there is the potential that biofilm secretions from different species may act in synergy. For example, there is a correlation between the in vitro biofilm - producing capacity of P. aeruginosa and S. aureus and unfavourable evolution after endoscopic sinus surgery26. In addition, using a porcine wound model, it was shown that while individual infections with strains of S. aureus and P. aeruginosa were sufficient to delay wound healing, only a co-infection resulted in decreased expression of KGF127. In normal wound healing circumstances KGF1 acts through its receptor to increase migration and proliferation.
There were several limitations inherent in this study, primarily in controlling the many variables. For example, quantifying the amount of total protein present in each sample may have enhanced our results. However, this process was complicated by the presence of the trypsinised soy protein present in the bacterial culture media. Therefore, normalising for protein content was not possible. Similarly, controlling growth conditions of the planktonic and biofilm cultures were difficult to perform equally. This is due to the different growth rates and potential nutrient requirements for the different phases. Also, the process of freeze drying may result in the loss of compounds such as volatile organic chemicals. Additionally, it has also been noted that protein structure may be adversely affected28.
In this study we have shown that BCM from two of the most common bacterial strains associated with infections have a profound effect on the wound healing processes of migration and proliferation. Additionally, we have shown a differential effect in keratinocytes of different anatomical sites. Furthermore, the data suggests that effects caused by P. aeruginosa BCM were due to a small cytotoxic molecule while the effects from S. aureus BCM were protein based. Proteomics on the PAGE separated S. aureus BCM was able to reveal a potential cocktail of proteins that may act either individually or in synergy to produce the effects seen. Our data would suggest that in addition to identifying which species of pathogens are present in a chronic wound or infection, a more detailed study of biofilm components is also necessary to elucidate how the presence of biofilm may delay wound healing.
P. aeruginosa isolates used in this study were obtained from a clinical case of canine otitis externa from Australia. Swabs were cultured onto 5% Columbia sheep blood agar (SBA) (Thermo Fisher Scientific, Scoresby, Vic, Australia) and incubated at 37°C and 42°C, overnight. Following incubation, cultures were stained by the Gram-method for determination of purity and morphology and an oxidase test was performed. S. aureus ATCC 29213 was routinely streaked out onto SBA and incubated at 37°C overnight. All bacterial isolates were stored at −80°C in brain heart infusion broth (BD Biosciences, Sydney, NSW, Australia) with 20% glycerol (Ajax Finechem (Thermo Fisher)).
Inoculated tryptic soy broth (TSB) (25ml culture concentration of 1.0×107cfu/mL) was incubated in 50ml tubes at 35±2°C for 24hours on a shaking incubator. Biofilms were formed using the MBEC™ high-throughput assay (MBEC™ Innovotech, Canada) according to the manufacturer’s instructions29 with incubation temperature at 35±2°C and times extended to 24hours. In brief, this device consists of a 96-peg-lid (top plate) and a ridged trough (bottom plate). The top plate fits over the trough containing 10ml of TSB. The inoculated device is placed on a rocking platform (Select BioProducts, Model SBS300-2, New Jersey, United States), which allows a shear force to be created forming equivalent biofilms on all the pegs. The inoculum is incubated at 35±2°C for 24hours in the MBEC device before collection.
Planktonic and/or biofilm cultures were centrifuged at 4500rpm for 20minutes at 4°C (MPW-351R centrifuge, Warsaw, Poland), the pellet discarded, the supernatant filtered (Millex, PES 0.22μm, Darmstadt, Germany) and frozen at −80°C. Samples were freeze-dried (Dynavac Freeze Dryer, Model FD12, Australia) and stored at −20°C. The freeze-dried conditioned media was then resuspended in an equivalent volume of DMEM+ (DMEM 4,500mg/l D –glucose, supplemented with 100U/ml penicillin, 100g/ml streptomycin (Invitrogen (Thermo Fisher)), and 10% FBS (Invitrogen)) before further dilutions.
Isolation of human tympanic membrane keratinocytes was performed with approval from the St. John of God Healthcare Ethics Committee (Subiaco, Western Australia). Human normal skin keratinocytes were isolated from upper arm skin with approval from the University of Western Australian Human Research Ethics Committee (Approval # RA/4/1/5489). Patients signed a written, informed consent before intervention and specimens were treated anonymously. All collections and experiments were conducted according to the principles and ethical standards expressed by the Declaration of Helsinki.
Culture of primary human tympanic keratinocytes was performed as previously described30. Briefly, fresh intact hTM tissue was obtained from consenting patients who underwent otological procedures requiring the permanent surgical removal of the tympanic membrane. All hTM tissue received was disease-free and considered morphologically normal. Small pieces of hTM tissue, approximately 0.25mm2, were placed into BD Falcon 6-well culture plates (BD Biosciences) containing DMEM+ (Invitrogen). The derived primary cells were incubated for 20 days in a humidified cell culture incubator at 37°C, with 5% carbon dioxide (CO2). Subsequent cell passages were incubated for 5 days in BD Falcon T-75 culture flasks (BD Biosciences).
Skin was excised from the upper arm and collected in 1ml of Epigrow TM human epidermal keratinocyte complete media (Merck Millipore, Massachusetts, USA). Fatty tissue beneath the dermis was removed using a sterile surgical blade (No.23) and forceps. The skin tissue was then cut into 3–5mm2 pieces. The pieces of skin were placed in 5ml of EpigrowTM human epidermal keratinocyte complete media with 20μl of fungizone (Gibco®, Invitrogen™, Carlsbad, California, USA) and 100μl of kanamycin (Gibco®). Dispase (Life technologies™, Carlsbad, California, USA) was added at 0.0127g per 5ml (2.4U/ml). This solution was incubated for 24hours at 40°C. This method is a modified version of a protocol published by the CELLNTEC company (CellNTEC, 2011).
After 24hours, the epidermis was separated from the dermis using sterile fine tip forceps and the pieces of epidermis transferred to a sterile petri dish with 500μl of TrypLETM Select (Gibco®). The epidermal tissue pieces were spread out flat on the surface of TrypLETM Select and covered with a lid to prevent evaporation. After incubating for 20 to 30minutes at room temperature, the petri dish was tilted at a 300 angle and 2ml of human epidermal keratinocyte complete media was added. Using sterile forceps, epidermal tissue pieces were rubbed gently against the base of the petri dish in order to generate a single cell suspension. The resulting cell suspension was collected in a 15ml centrifuge tube and the previous step repeated to increase the yield of keratinocytes. The second preparation of a single cell suspension was then added to the same 15ml centrifuge tube. The combined cell preparation was then centrifuged at 200g for 3minutes. The cell pellet was resuspended in 5ml of human epidermal keratinocyte complete media. Cells were cultured in a T25 tissue culture flask (Sarstedt Australia Pty Ltd, Belmore, NSW, Australia)
Samples of conditioned media were filtered through Amicon® Ultra-4 (Ultracel® - 3k) Centrifugal filters (Merk Millipore Ltd, Tullagreen, Cork, Ireland) with a 3KDa cutoff. Both flow through and the filtrate were retained for analysis.
Undiluted samples of conditioned media were subjected to heat treatment of 75°C for 20minutes. The samples were allowed to cool to room temperature prior to use in downstream assays.
Cell numbers following proliferation were calculated using a modified cell attachment assay31. This method uses a crystal violet solution to stain cells attached to the culture plate. After solubilizing the stained cells, the intensity of the solution is proportional to the number of cells present.
Cells were seeded into the wells of a 96 well plate (Greiner Bio-One GmbH, Frickenhausen, Germany) at a density of 3000cells/well in 200μl of DMEM+. The plates were incubated as described overnight (approx. 16hours) to equilibrate. The media was then replaced with conditioned media diluted to 10% in DMEM+. Cells were incubated for 48hours. The media was then removed and the cells fixed using 100μl of 10% neutral buffered formalin (NBF). The fixed cells were washed twice in 100μl PBS with gentle shaking. The PBS was aspirated and the cells stained with 100μl of crystal violet solution (0.1% w/v crystal violet in 200μM MES buffer, pH 6.0 filtered through a 0.22μm filter) for 15minutes. The crystal violet solution was removed and the cells washed 3 times in 100μl ddH20 with gentle shaking. All the ddH2O was aspirated and the cells solubilized in 100μl of 10% acetic acid for 10minutes with gentle shaking. Absorbance was read at 570nm on an EPOCH microplate reader (BioTek Instruments Inc., Winooski, VT, USA)
Using IBIDI cell migration culture inserts (Ibidi GmbH, Martinsried, Germany), 5×104 cells in a volume of 70μL of DMEM+ were seeded into adjoining Ibidi insert chambers that had been placed into the wells of a 48-well plate (Greiner). The cells were then incubated overnight at 37°C in a humidified atmosphere with 5% CO2. The inserts were removed after 24hours to reveal a well defined gap approximately 500μm wide. The wells were washed once by gentle shaking with 150μl of PBS before adding 400μl of fresh DMEM+ containing diluted conditioned media. Cells were photographed at 0 and 6hours for hTMts and at 0 and 15hours for hEKs using a Nikon Eclipse TE2000-5 microscope. Multiple photographs were taken to ensure the entire “gap” was captured. The gap was then measured using ImageJ software (NIH, USA) at 20 different points along the gap and averaged to provide the mean gap distance. The relative distance of cell migration is calculated as:
% Gap closure=Test (G-t0 hr – G-t6/15 hr)/Control (G-t0 hr – G-t6/15 hr) X 100%.
Where G-t0 hr is the mean gap distance prior to cellular migration immediately following the removal of the Ibidi culture insert (zero hour) and G-t6/15 hr is the mean gap distance at the 6 or 15hour endpoint. The results are expressed as a percentage of the control treatment, which contains no conditioned media or diluted TSB media.
BCM and PCM samples (300μl) were vacuum desiccated and resuspended in 20μl of standard 1 × Laemmli loading buffer. Samples were heated to 95°C for 10minutes and allowed to cool to room temperature for 10minutes. The tubes were centrifuged to collect the contents. Premade 4–12% gradient polyacrylamide gels were used for protein separation (Bio-Rad Laboratories, Hercules, CA, USA). The gel cassette was loaded into a Protean II gel apparatus (BioRad) as per the manufactures instructions with standard 1 × Tris/Glycine running buffer. The protein samples were loaded in the wells along with a sample of Kaleidoscope size marker (Promega Corporation, Sydney, Australia) and the gel run at 130V for 30minutes. After separation, the gel was removed from the cassette into a small dish and stained with 100ml of coomassie blue stain (BioRad) for 2hours with gentle rocking. The stain was decanted and the gel rinsed for several seconds in ddH2O to remove excess stain. 100ml of destain solution (50% ddH2O, 40% methanol, 10% acetic acid) was then added to the gel along with 2–3 small pieces (2cm3) of sponge and gently rocked overnight. The destained gel was then photographed.
Prominent bands in the polyacrylamide gel were excised and submitted to Proteomics International (Perth, Western Australia, Australia) for identification. Protein samples were trypsin digested and peptides extracted according to standard techniques32. Peptides were analysed by electrospray ionisation mass spectrometry using the Agilent 1260 Infinity HPLC system (Agilent Technologies, Santa Clara, CA, USA) coupled to an Agilent 6540 mass spectrometer (Agilent). Tryptic peptides were loaded onto a C18 column 300 SB, 5μm (Agilent) and separated with a linear gradient of water/acetonitrile/0.1% formic acid (v/v). Spectra were analysed to identify proteins of interest using Mascot sequence matching software (Matrix Science Inc., Boston, MA, USA) with Ludwig NR database. A match was considered positive if two or more peptides map to the same protein and were within the predicted size parameters as estimated by the standard on the acrylamide gel.
ANOVA with a post hoc Dunnett’s test was used to analyse migration and proliferation results. Four replicates (n=4) were used for each test. All comparisons were made against the TSB (vehicle) control. Significance was set at p<0.05.
How to cite this article: Jeffery Marano, R. et al. Secreted biofilm factors adversely affect cellular wound healing responses in vitro. Sci. Rep. 5, 13296; doi: 10.1038/srep13296 (2015).
The mass spectrometry analyses were performed in facilities provided by the Lotterywest State Biomedical Facility-Proteomics node and BioPlatforms Australia, at the Harry Perkins Institute of Medical Research. Proteomics data analysis described in this work was supported by the use of the Australian Proteomics Computational Facility based at Walter and Eliza Hall Institute of Medical Research.
The authors declare no competing financial interests.
Author Contributions R.M. designed and executed experiments, analysed data and prepared the manuscript. H.J.W. and M.W. helped design experiments and prepare the manuscript. D.W. performed laboratory experiments and assisted in interpretation of results. HSW and R.O’.H. aided experimental design, established the bacterial cultures, produced the conditioned media, interpreted results and aided in manuscript preparation.