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International Journal of Microbiology
Volume 2011 (2011), Article ID 972494, 10 pages
Adhesion of Pathogenic Bacteria to Food Contact Surfaces: Influence of pH of Culture
1Food Research and Development Centre, Agri-Food and Agriculture Canada, 3600 Casavant Boulevard-West, St-Hyacinthe, QC, Canada J2S 1A2
2Department of Science and Nutrition, Laval University, Quebec, QC, Canada G1K 7P4
Received 26 May 2010; Revised 1 September 2010; Accepted 15 September 2010
Academic Editor: Jorge H. Leitao
Copyright © 2011 Akier Assanta Mafu et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.
The adhesion of Aeromonas hydrophila, Escherichia coli O157:H7, Salmonella Enteritidis, and Staphylococcus aureus to hydrophobic and hydrophilic surfaces in cultures with different pHs (6, 7, and 8) was studied. The results indicated that the type of material had no effect on the attachment capacity of microorganisms, while environmental pH influenced the adhesion of A. hydrophila, E. coli, and S. aureus to both solid substrates. The attachment of S. Enteritidis () was not affected by the type of substrate or the culture pH, whereas E. coli displayed the weakest affinity for both polystyrene and glass surfaces. No correlation was established between the physicochemical properties of the materials, or the bacterial and the rate of bacterial adhesion, except for S. aureus. Photomicrographs have shown that surfaces were contaminated by small clusters of S. Enteritidis while S. aureus invaded the food contact surfaces in the form of small chains or cell aggregates.
In food processing plants, residues of all kinds chemical, biological, organic, or inorganic inevitably accumulate on the surfaces of equipments in contact with food . Attachment of undesirable microorganisms to these surfaces is a source of concern, since this can result in product contamination leading to serious economic and health problems [2–4]. In fact, this microbial contamination has two components: first, the saprophytic flora responsible for food spoilage and second, the pathogenic flora, which cause infections in humans and animals. To adversely affect the sensory, physical, and chemical qualities of food, a large population of spoilage-causing microorganisms is required, while in the case of food pathogens it only takes a few cells to affect product safety and cause food poisoning.
In the phenomenon of bacterial adhesion to inert surfaces, the physicochemical properties (hydrophobicity and charges) and substrates or surface topography are playing important roles [5–7]. Joints such as valves and any other difficult-to-reach spaces are the most favourable areas to bacterial adhesion. The effect of corrosion on solid materials must also be considered since it can lead to the formation and expansion of cavities and grooves . This in turn provides breeding sites for microorganisms, thereby compromising the efficacy of cleaning and disinfection procedures. The surface characteristics of the microorganisms themselves and the various environmental conditions encountered in agri-food industries (organic materials, pH, temperature, water activity, etc.) also influence microbial attachment to inert surfaces [2, 9–12].
Once they have adhered to inert surfaces, the microorganisms may exhibit a greater degree of resistance to the chemical or natural cleaning and disinfecting agents used in the agri-food industries compared to bacteria in suspension [13, 14].
The potential for attachment and development of microorganisms on inert surfaces as well as the resistance of the resulting sessile cells has been and continues to be extensively studied [15–19]. Although an understanding of the parameters that govern the adhesion of these bacteria to solid surfaces could help developing new prevention procedures at the initial stages of microbial adsorption, there are still too many unknown factors concerning the adhesion capacity of the main food pathogens .
The objective of this study was to find out the adhesion capacity of pathogens such as Aeromonas hydrophila, Escherichia coli O157:H7, Salmonella Enteritidis, and Staphylococcus aureus on two commonly used materials in food processing plants (polystyrene and glass). The influence of culture medium pH on the rate of adhesion by these agents at the interfaces was also simultaneously evaluated.
2. Material and Methods
2.1. Bacterial Strains, Media, and Culture Conditions
For this study, Aeromonas hydrophila ATCC 7966, Escherichia coli O157:H7 ATCC 35150, Salmonella Enteritidis E1347, and Staphylococcus aureus ATCC 29213 were selected. Cryotubes of these strains, stored at in TSB-YE (tryptic soy broth supplemented with 1% yeast extract; Difco Laboratories, Detroit, MI) containing 20% glycerol (Difco Laboratories, Detroit, MI), were thawed and the bacterial cultures were revived by two successive precultures in 10 mL of TSB-YE (1% v/v) and then incubated for 24 h at
The harvested bacteria were washed three times and resuspended in buffers at pH 6.0, 7.0, or 8.0. A total viable count was performed for each culture and the total CFUs determined using tryptic soy agar (TSA; Difco Laboratories, Detroit, MI) were between and CFU/mL.
2.2. Selection of Test Surfaces and Preconditioning Procedures
Polystyrene (hydrophobic) and glass (hydrophilic) substrates were selected for the adhesion tests. Polystyrene weighing dishes (no. 25433; VWR International Inc., West Chester, PA) were used to obtain 5- coupons and 5- glass coupons were cut from microscope slides (no. 48300; VWR International Inc., West Chester, PA). Prior to physicochemical characterizations and adhesion tests, these substrates were soaked for 24 h in sodium hydroxide (1 N), washed and rinsed thoroughly eight times with deionized water (Millipore, Billerica, MA). The polystyrene coupons were sterilized for 5 min in boiling distilled water, while the glass coupons were directly autoclaved at for 15 min in bioreactors.
2.3. Surface Contamination
The attachment tests were conducted in sterile bioreactors (BST Model SC60 Suspend Reactor, BioSurface Technologies Corporation, Bozeman, MT). Using a sterile clamp and under a microbiological hood, the sterile coupons were mounted on metal rods (six rods per bioreactor) in pairs, separated by a stainless steel nut. To ensure a sufficient attachment of the bacterial cells, the cultures of the pathogens in the bioreactors were left in contact with the inert surfaces for 24 h at ambient temperature under low agitation (90 rpm). Each experiment (bacterium-culture pH-surface type combination) was repeated three times and the means were used for the statistical analyses.
2.4. Rate of Adhesion of the Pathogens to Inert Surfaces
To recover the sessile cells, two coupons of each material were removed from the rods using a sterile clamp and rinsed twice in tubes containing 10 mL of saline (one tube per rinse, carefully rotating the tubes) in order to eliminate the cells that had not adhered. The substrates were then placed in a tube containing 10 mL of sterile phosphate buffer (Oxoid Ltd, Basingstoke, Hampshire, England) and all of the adhered bacterial cells were detached in a sonication bath (VWR International Inc., West Chester, PA) for 10 min. The tubes were vortexed for 30 s before the microbial counts were performed. After preparation of serial dilutions, the bacterial counts were determined by plating on TSA (tryptic soy agar; Difco Laboratories, Detroit, MI) incubated at for 24 h. The relative adhesion (%) was estimated using the following formula:
2.5. Scanning Electron Microscopy (SEM) Observation
In preliminary work, the two types of noncontaminated sterile materials were gold coated and observed under a scanning electron microscope in order to characterize the microstructure of the substrates.
After two saline rinses, the contaminated coupons were fixed by immersion in 5 mL of 2.5% glutaraldehyde (v/v) in a 0.1 M sodium cacodylate buffer (pH 7.3) and left at room temperature for 2 h. The glutaraldehyde was then removed using a Pasteur pipette and the substrates were rinsed four times by immersing them for 15 min in 0.1 M sodium cacodylate buffer (pH 7.3).
Dehydration was performed through an ascending series of ethanol (approximately 5 mL) concentrations (30%, 50%, 70%, and 80%) for 15 min for each concentration, and then three times for 15 min in 100% ethanol. The duplicates were preserved in 70% ethanol and stored at
Dehydration was completed using in a critical point dryer (Model E3000 CPD, Bio-Rad, Polaron Equipment Ltd., Watford Hertfordshire, England). The samples were then mounted on an aluminum platform and covering with 8 nm of gold using a sputter coater (Cressington 108, Kurt J. Lesker Co., Clairton, PA). The substrates were observed under a scanning electron microscope (Hitachi S300N, Hitachi, Tokyo, Japan).
2.6. Determination of the Physicochemical Properties of the Solid and Bacteria Surfaces
For the inert material, sterile dried substrates were positioned on a microscope stage for contact angle measurements. A microsyringe (Chromatographic Specialities Inc., Brockville, Ontario, Canada) was used to place a drop (1 L) of each wetting agent—bidistilled water (Barnstead Fistreem GlassStill, England), formamide, and α-bromonaphthalene (Aldrich Chemical Co., Inc., Milwaukee, WI)—on the solid surfaces. The contact angles formed by these liquids were determined using a goniometer coupled with a 100 telescope (Gaertner Scientific Corp., Chicago, Ill.).
In each case, six measurements were taken with each liquid on each substrate to determine the surface charge of the substrates  as well as their hydrophilic-hydrophobic characteristics. The total surface energy of the solid substrates, the Lifshitz-van der Waals contribution to surface energies and the Lewis acid-base bonds were calculated using an extension of the Young-Dupré equation : where θ represents the angle formed by the wetting liquid on the substrate and the surface tension of the wetting liquid. and are, respectively, the Lifshitz-van der Waals dispersion, electron donor (basic) and electron acceptor (acid) components of the wetting liquid and inert surface.
Once these parameters have been determined, for both the solid substrates () and for each bacterium () in an aqueous medium (), the free energy of microbial adhesion, was estimated according to the following formula: In theory, the energy balance is favourable to bacterial adhesion if and unfavourable if
Bacteria physicochemical properties were determined for bacterial cultures grown at pHs 6, 7, and 8. The contact angle measurements were performed on bacterial lawns deposited on filter paper as described by Mafu et al.  and the total surface energy of the bacteria and the Lifshitz-van der Waals contribution to surface energies as well as the Lewis acid-base bonds were determined with the help of Young-Dupré relationship (2). The surface properties of the pathogens were evaluated in term of free energy of aggregation using the van der Mei et al.  approach (4) where and are, respectively, the Lifshitz-van der Waals dispersion, electron donor (base) and electron acceptor (acid) components of the microorganisms studied and those of the water. A preference for the aqueous medium, a characteristic of hydrophilic cell surfaces, is demonstrated by a value while hydrophobic organisms, which tend to agglomerate in aqueous suspensions, are characterized by a
2.7. Statistical Analyses
The data were analysed using the GLM procedure of SAS software Version 8.0 (SAS Institute Inc., Cary, NC). An analysis of variance in the form of a factorial experiment (bacterium culture pH surface type) in complete blocks was chosen for adhesion tests. When the pH-pathogen interaction terms were significant, a one-way analysis of variance (culture pH) was performed for each of the four bacteria. The significant differences for the free energies of adhesion were detected using a one-way analysis of variance. The Duncan multiple ranges test was also used to separate means. A confidence level of was chosen during analyses.
3.1. Surfaces Characterization
Photomicrographs of uncontaminated polystyrene and glass obtained using SEM are shown in Figure 1. The substrates microstructure revealed that glass was a smooth surface (Figure 1(a)), while polystyrene had irregularities, with tiny bumps and hollows (Figure 1(b)).
The results obtained for the surface physicochemical properties of the two substrates, determined from contact angle measurement with three solvents, are detailed in Table 1. The surfaces were characterized by a similar Lifshitz-van der Waals dispersion component and by very low values for the electron acceptor parameter The electron donor and Lewis acid base capacities showed considerable variability from one type of material to the other. The total surface energy measured for the polystyrene was lower than for glass. Water drops spread over the glass surface, demonstrating its hydrophilic character, consistent with the high value of the electron donor parameter. Polystyrene was characterized by extremely weak electrical properties. In addition, the angles formed by the water on the specimen were very obtuse compared with those obtained on glass, enabling us to conclude that the surface is hydrophobic.
3.2. Prediction of Pathogen Adhesion to Both Surfaces
The free energy of adhesion of the pathogens on bare surfaces, determined by combining the surface characteristics of the selected substrates (Table 1) and the surface properties of the bacteria (Table 4), are shown in Table 2. The values of polystyrene were negative for all microorganism—culture pH—surface combinations, predicting that adhesion would be thermodynamically favourable for the polymer. This approach predicts that conditions would be unfavourable to bacterial attachment in the presence of glass, a hydrophilic surface, since the free energy of adhesion was positive in all cases. Theoretically, A. hydrophila and E. coli should exhibit weaker adsorption on both substrates at pH 6 For S. aureus, the rate of adhered bacteria should be highest in the case of hydrophobic surface at pH 7 and lowest in the case of hydrophilic surface at pH 8 For the two substrates studied, pH of the culture affected the theoretical affinity of S. Enteritidis
3.3. Influence of the Inert Surface and pH of the Culture on the Adhesion of Pathogenic Bacteria
At pH 6, 7, and 8, no interactions were determined between pH of culture and adhesion capability for individual bacterium The effect of each parameter therefore had to be studied independently. The type of substrate did not influence the rate of attachment of pathogens however the effect of pH of the culture varied depending on the type of microorganism considered.
E. coli displayed the lowest relative adhesion, regardless of environmental pH (Table 3). The affinity of E. coli for the solid samples was significantly influenced by pH
A. hydrophila on solid surfaces exhibited the same profile as E. coli (Table 3), however, Aeromonas cell had greater affinity for the two substrates than the enterohemorrhagic bacterium, especially in acid and neutral media, with the number of attached cells ranging from 45% to and from 39% to respectively. The adhesion capacity of A. hydrophila to inert surfaces was lower after being cultivated in an alkaline medium For E. coli and A. hydrophila, neutral pH was the best condition for attachment of these two pathogens, regardless of the type of surface.
Type of substrate and pH had no effect on the adsorption of S. Enteritidis to surfaces The degree of contamination of polystyrene and glass by this enterobacteria was considerably higher than that observed for the other bacteria at pH 8 At pH 6 and 7, S. Enteritidis had been attached to the polymer and glass equally
Also, after the contamination period, adhesion of S. aureus to the two types of coupons (Table 3) was lower compared to the other experimental conditions The number of organisms attached to both substrates decreased by elevating pH. At pH 8, the number of detached S. aureus cells was identical on both polystyrene and glass surfaces
3.4. Influence of the Surface Physicochemical Properties of Pathogenic Bacteria on Their Rate of Adhesion
Figure 2 demonstrates the mean relative adhesion rate of each bacterium as a function of the component of their surfaces. In fact, since the solid surfaces had no effect on the concentration of adhered cells the mean between the relative adhesion to polystyrene and to glass could be calculated in order to obtain an overall adhesion rate. Only an high correlation coefficient between the free energy of aggregation of S. aureus and its mean rate of adhesion to the substrates has been found (Figure 2). The greater the hydrophilic character displayed by this bacterium, the lower its tendency to attach to inert surfaces.
3.5. Scanning Electron Microscopy Observations
On both types of surfaces, porous and nonporous, a very low number of E. coli and dispersed cells of A. hydrophila were observed (data not shown). That is why no photomicrographs of these microorganisms have been provided. S. Enteritidis cells were generally isolated or formed small clusters, regardless of the adhesion conditions (Figure 3). Their dispersion was more uniform at pH 6 than at the other pH values (Figures 3(a) and 3(b)). S. aureus invaded the abiotic surfaces in the form of single cells, small chains, or cell aggregates (Figure 4). It was more difficult to observe staphylococci on polystyrene and glass at pH 8 (Figures 4(e) and 4(f)). As demonstrated by the present results, it becomes clear that in all case, no visible extracellular material was observed on both food contact surfaces.
Bacterial adhesion to surfaces and biofilm formation are complex phenomena influenced by a number of factors. In this study, three of these factors, namely, microbial strains, culture pH, and type of surface, were analysed. Polystyrene and glass were chosen as surfaces, respectively, hydrophobic and hydrophilic, for the attachment and biofilm formation tests.
Scanning electron microscopy observation (Figures 3 and 4) showed that all the pathogens had the capacity to adhere to both types of surface. Although the cavities and distortions of the samples observed under the scanning electron microscope increase the specific contact area for bacteria, the differences in surface irregularities between both solid surfaces had no observable impact on the relative adhesion of the microorganisms. These results are consistent with the findings of Mafu et al. , who found no correlation between the microstructure of the materials and the capacity of bacteria to adhere to surfaces. Also in this study, the attachment of solid surfaces by microorganisms was influenced solely by culture pH, which concurs with the work of Husmark and Ronner  as well as that of Herald and Zottola . The absence of fimbriae and curli [25, 26] might explain the low contamination of E. coli observed in this study as well as in other experiments conducted on the contamination of polymers by serotype O157 [24, 27, 28].
The data from these experiments are not in agreement with the predictions deduced from the free energies of adhesion of pathogens on polystyrene (Table 2). These energy characteristics demonstrated that conditions for adsorption of all microorganisms were thermodynamically favourable on polystyrene ( 0) and unfavourable on glass () surfaces. The bacterial cultures remained in contact with the inert surfaces for 24 hours. After this contact time, the adhesion stage tends to be irreversible. If the exposure time had been shorter (maximum of four hours, which corresponds to irreversible bacterial adsorption), the predictions for the adhesion, based on , might have proven valid. In fact, the equation used to predict bacterial adhesion to surfaces () does not take into consideration the exopolysaccharides that might be produced for the irreversible attachment of microorganisms.
In another attempt to explain adhesion detection with values we endeavoured to determine whether the surface properties of the infectious agents influenced their adhesion rate. Thus, the free energy of aggregation of S. aureus could be correlated to the degree of attachment of the cocci (Figure 2). Gilbert et al.  also demonstrated that the adhesion of Staphylococcus epidermidis to glass, unlike Escherichia coli, was negatively correlated to the microorganism’s hydrophilicity and surface electronegativity. However, the physicochemical characteristics of the inert surfaces and of the other three pathogens examined throughout this study did not shed any light on their adhesion capacity. The explanation may lie in the composition of the suspension medium of the microorganisms, which was not taken into account in the estimation of PS and glass free energy.
Indeed, conditioning the substrates with compounds from the suspension medium can increase or decrease subsequent bacterial adhesion [23, 30, 31]. These ionic substances located at the microorganism-surface interface can change ionic strength which is a critical factor in adhesion. Some of these elements can reduce the repulsive force between the bacterium and the solid surfaces [32, 33], due to electrostatic interactions, by masking charges of the same sign. Thus, several stress responses are associated with the appearance of macromolecular agents in the medium. Many microorganisms exposed to acidic and alkaline stress synthesize polysaccharides, peptides, or heat-stable proteins [10, 34], which play an active role in induction of tolerance to pH stress. It should also be noted that some bacteria produce biosurfactants that inhibit their attachment. For instance, synthesis by S. aureus of a surfactant, the toxin inhibits the action of D-alanine , limiting cell adhesion to polystyrene .
Previous studies have also demonstrated the important roles played by cell organelles and bacterial mobility in transport and adhesion to various types of surfaces. Pseudomonas fluorescens strains without flagella exhibited a weak capacity to attach to surfaces and develop a biofilm . Flagella apparently play an essential role during the initial reversible stages of attachment by overcoming the repulsive forces. However, the nonmotile bacterium S. aureus adhered to the tested substrates at pH 6 in greater numbers than E. coli O157:H7 and A. hydrophila (Table 3), which are motile microorganisms. The presence of flagella is apparently more important when the velocity of the environmental liquid is high [4, 36]. McClaine and Ford  demonstrated that rotation of the flagellum caused detachment of fixed motile bacteria when flow rates were low (0.02 mLmin-1), while their adhesion was strengthened at high flow rates (2 mL).
Although the irreversible attachment of microorganisms is often associated with the production of exopolysaccharides, no extracellular matrix was detected by scanning electron microscopy, regardless of experimental conditions. This indicates that the presence of polymers is not necessary for permanent adhesion of microorganisms to a surface. The visible filaments attached to the substrates may be dependent on the suspension medium. Maximum polysaccharide production is generally associated with an environment deficient in essential nutrients, such as carbon, nitrogen, calcium, and iron [26, 38]. Contact time and environmental temperature are other factors that influence the formation of a three-dimensional network [39, 40]. However, these appendices are crucial for biofilm consolidation and their resistance to environmental stresses .
Several molecules from the culture media can contribute to produce a conditioning film at the surface of the substrates . These molecules include proteins, which are block copolymers presenting hydrophobic as well as hydrophilic sections. It is thus possible for such molecules to adhere to hydrophilic substrates such as glass, resulting in an hydrophobization of the surface. This phenomena would lead bacteria presenting the same adhesion trends on both PS and hydrophobically coated glass.
The results of this work indicate that pathogens could adapt to various pH levels of cultural media and adhere indifferently to inert polystyrene and glass surfaces, regardless of their hydrophilic or hydrophobic nature which leads to biofilm formation and increases the possibility of resistance to sanitizing agents. Therefore, to minimize surfaces contaminations, one should be aware of the influence of different environmental conditions which affects survival of bacteria in order to reduce their incidence in food systems. The operations must be carried out promptly and regularly (between two production cycles, for example), since they can effectively detach and eliminate the adhered bacteria when they have not yet formed a biofilm, thereby preventing contamination of raw materials and finished products and protecting consumer health.
The authors would like to thank Claude Laberge for the statistical analyses, Marie-Josée Lemay, Marie-Josée Gagné, Avila Croisetière, François Saint-Germain, and Ali Taherian for their technical assistance and scientific advices.
- G. I. Loeb and R. A. Neihof, “Marine conditioning films,” in Applied Chemistry at Protein Interfaces, R. E. Baier, Ed., vol. 145 of Advances Chemical Series, pp. 319–335, American Chemical Society, 1975.
- B. Carpentier and O. Cerf, “Biofilms and their consequences, with particular reference to hygiene in the food industry,” Journal of Applied Bacteriology, vol. 75, no. 6, pp. 499–511, 1993.
- G. A. McFeters, M. J. Bazin, J. D. Bryers, et al., “Biofilm development and its consequences,” in Microbial Adhesion and Aggregation, K. C. Marshall, Ed., pp. 109–124, Springer, Berlin, Germany, 1984.
- R. F. Mueller, “Bacterial transport and colonization in low nutrient environments,” Water Research, vol. 30, no. 11, pp. 2681–2690, 1996.
- C. Faille, C. Jullien, F. Fontaine, M.-N. Bellon-Fontaine, C. Slomianny, and T. Benezech, “Adhesion of Bacillus spores and Escherichia coli cells to inert surfaces: Role of surface hydrophobicity,” Canadian Journal of Microbiology, vol. 48, no. 8, pp. 728–738, 2002.
- C. Jullien, T. Bénézech, B. Carpentier, V. Lebret, and C. Faille, “Identification of surface characteristics relevant to the hygienic status of stainless steel for the food industry,” Journal of Food Engineering, vol. 56, no. 1, pp. 77–87, 2003.
- D. R. Korber, J. R. Lawrence, B. Sutton, and D. E. Caldwell, “Effect of laminar flow velocity on the kinetics of surface recolonization by Mot+ and Mot-Pseudomonas fluorescens,” Microbial Ecology, vol. 18, no. 1, pp. 1–19, 1989.
- J-C. Cartonné and R. Tournier, “Corrosion et anticorrosion des matériaux métalliques utilisés dans les équipements et les ateliers bio-industriels,” in Nettoyage, Désinfection et Hygiène dans les Bio-Industries, J.-Y. Leveau, M. Bouix, J.-Y. Leveau, and M. Bouix, Eds., p. 84, Tec & Doc, Paris, France, 1999.
- M. Fletcher, “The effects of culture concentration and age, time, and temperature on bacterial attachment to polystyrene,” Canadian Journal of Microbiology, vol. 23, no. 1, pp. 1–6, 1977.
- J. W. Foster and H. K. Hall, “Adaptive acidification tolerance response of Salmonella typhimurium,” Journal of Bacteriology, vol. 172, no. 2, pp. 771–778, 1990.
- I. Giovannacci, G. Ermel, G. Salvat, J. L. Vendeuvre, and M. N. Bellon-Fontaine, “Physicochemical surface properties of five Listeria monocytogenes strains from a pork-processing environment in relation to serotypes, genotypes and growth temperature,” Journal of Applied Microbiology, vol. 88, no. 6, pp. 992–1000, 2000.
- M. Gross, S. E. Cramton, F. Götz, and A. Peschel, “Key role of teichoic acid net charge in Staphylococcus aureus colonization of artificial surfaces,” Infection and Immunity, vol. 69, no. 5, pp. 3423–3426, 2001.
- H. Anwar, M. K. Dasgupta, and J. W. Costerton, “Testing the susceptibility of bacteria in biofilms to antibacterial agents,” Antimicrobial Agents and Chemotherapy, vol. 34, no. 11, pp. 2043–2046, 1990.
- H. Park, Y.-C. Hung, and C. Kim, “Effectiveness of electrolyzed water as a sanitizer for treating different surfaces,” Journal of Food Protection, vol. 65, no. 8, pp. 1276–1280, 2002.
- P. Chavant, B. Martinie, T. Meylheuc, M.-N. Bellon-Fontaine, and M. Hebraud, “Listeria monocytogenes LO28: surface physicochemical properties and ability to form biofilms at different temperatures and growth phases,” Applied and Environmental Microbiology, vol. 68, no. 2, pp. 728–737, 2002.
- CDC. 2002, “Preliminary foodnet data on the incidence of foodborne illnesses—Selected sites, United States,” Morbidity and Mortality Weekly Report, vol. 51, no. 15, pp. 325–329, 2002.
- A. A. Mafu, M. Pitre, and S. Sirois, “Real-time PCR as a tool for detection of pathogenic bacteria on contaminated food contact surfaces by using a single enrichment medium,” Journal of Food Protection, vol. 72, no. 6, pp. 1310–1314, 2009.
- A. A. Mafu, D. Roy, and K. Machika, “Efficiency of disinfecting agents to destroy Listeria monocytogenes, Yersinia enterocolitica and Staphylococcus aureus on a contaminated surface,” Dairy, Food and Environmental Sanitation, vol. 16, no. 7, pp. 426–430, 1996.
- A. A. Mafu, D. Roy, J. Goulet, and L. Savoie, “Characterization of physicochemical forces involved in adhesion of Listeria monocytogenes to surfaces,” Applied and Environmental Microbiology, vol. 57, no. 7, pp. 1969–1973, 1991.
- C. J. Van Oss, M. K. Chaudhury, and R. J. Good, “Interfacial Lifshitz-van der Waals and polar interactions in macroscopic systems,” Chemical Reviews, vol. 88, no. 6, pp. 927–941, 1988.
- H. C. van der Mei, R. Bos, and H. J. Busscher, “A reference guide to microbial cell surface hydrophobicity based on contact angles,” Colloids and Surfaces B, vol. 11, no. 4, pp. 213–221, 1998.
- A. A. Mafu, D. Roy, J. Goulet, and P. Magny, “Attachment of Listeria monocytogenes to stainless steel, glass, polypropylene, and rubber surfaces after short contact times,” Journal of Food Protection, vol. 53, no. 9, pp. 742–746, 1990.
- U. Husmark and U. Ronner, “Forces involved in adhesion of Bacillus cereus spores to solid surfaces under different environmental conditions,” Journal of Applied Bacteriology, vol. 69, no. 4, pp. 557–562, 1990.
- P. Herald and E. A Zottola, “Attachment of Listeria monocytogenes to stainless steel surfaces at various temperatures and pH values,” Journal of Food Science, vol. 53, no. 5, pp. 1549–1552, 1988.
- A. L. Cookson, W. A. Cooley, and M. J. Woodward, “The role of type 1 and curli fimbriae of Shiga toxin-producing Escherichia coli in adherence to abiotic surfaces,” International Journal of Medical Microbiology, vol. 292, no. 3-4, pp. 195–205, 2002.
- A. C. L. Wong, “Influence of culture conditions on biofilm formation by Escherichia coli O157:H7,” International Journal of Food Microbiology, vol. 26, no. 2, pp. 147–164, 1995.
- G. Harkes, H. C. van der Mei, P. G. Rouxhet, J. Dankert, H. J. Busscher, and J. Feijen, “Physicochemical characterization of Escherichia coli—a comparison with gram-positive bacteria,” Cell Biochemistry and Biophysics, vol. 20, no. 1, pp. 17–32, 1992.
- M. A. Assanta, D. Roy, M.-J. Lemay, and D. Montpetit, “Evidence for Escherichia coli O157:H7 attachment to water distribution pipe materials by scanning electron microscopy,” Journal of Food Protection, vol. 65, no. 12, pp. 1970–1975, 2002.
- P. Gilbert, D. J. Evans, E. Evans, I. G. Duguid, and M. R. W. Brown, “Surface characteristics and adhesion of Escherichia coli and Staphylococcus epidermidis,” Journal of Applied Bacteriology, vol. 71, no. 1, pp. 72–77, 1991.
- B. E. Brooker, “Surface coat transformation and capsule formation by Leuconostoc mesenteroides NCDO 523 in the presence of sucrose,” Archives of Microbiology, vol. 111, no. 1-2, pp. 99–104, 1976.
- S. K. Hood and E. A. Zottola, “Adherence to stainless steel by foodborne microorganisms during growth in model food systems,” International Journal of Food Microbiology, vol. 37, no. 2-3, pp. 145–153, 1997.
- M.-N. Bellon-Fontaine, N. Mozes, H. C. van der Mei et al., “A comparison of thermodynamic approaches to predict the adhesion of dairy microorganisms to solid substrata,” Cell Biophysics, vol. 17, no. 1, pp. 93–106, 1990.
- R. Briandet, T. Meylheuc, C. Maher, and M. N. Bellon-Fontaine, “Listeria monocytogenes Scott A: Cell surface charge, hydrophobicity, and electron donor and acceptor characteristics under different environmental growth conditions,” Applied and Environmental Microbiology, vol. 65, no. 12, pp. 5328–5333, 1999.
- R. J. Rowbury, N. H. Hussain, and M. Goodson, “Extracellular proteins and other components as obligate intermediates in the induction of a range of acid tolerance and sensitisation responses in Escherichia coli,” FEMS Microbiology Letters, vol. 166, no. 2, pp. 283–288, 1998.
- C. Vuong, H. L. Saenz, F. Gotz, and M. Otto, “Impact of the agr quorum-sensing system on adherence to polystyrene in Staphylococcus aureus,” Journal of Infectious Diseases, vol. 182, no. 6, pp. 1688–1693, 2000.
- D. R. Korber, J. R. Lawrence, and D. E. Caldwell, “Effect of motility on surface colonization and reproductive success of Pseudomonas fluorescens in dual-dilution continuous culture and batch culture systems,” Applied and Environmental Microbiology, vol. 60, no. 5, pp. 1421–1429, 1994.
- J. W. McClaine and R. M. Ford, “Characterizing the adhesion of motile and nonmotile Escherichia coli to a glass surface using a parallel-plate flow chamber,” Biotechnology and Bioengineering, vol. 78, no. 2, pp. 179–189, 2002.
- C. M. Brown, D. C. Ellwood, and J. R. Hunter, “Growth of bacteria at surfaces: Influence of nutrient limitation,” FEMS Microbioogy Letters, vol. 1, no. 3, pp. 163–166, 1977.
- M. F. A. Bal’a, I. D. Jamilah, and D. L. Marshall, “Attachment of Aeromonas hydrophila to stainless steel surfaces,” Dairy Food and Environmental Sanitation, vol. 18, no. 10, pp. 1240–1247, 1998.
- M. A. Assanta, D. Roy, M.-J. Lemay, and D. Montpetit, “Attachment of Arcobacter butzleri, a new waterborne pathogen, to water distribution pipe surfaces,” Journal of Food Protection, vol. 65, no. 8, pp. 1240–1247, 2002.
- C.-T. Huang, F. P. Yu, G. A. McFeters, and P. S. Stewart, “Nonuniform spatial patterns of respiratory activity within biofilms during disinfection,” Applied and Environmental Microbiology, vol. 61, no. 6, pp. 2252–2256, 1995.
- S. Sardin, J.-J. Morrier, G. Benay, and O. Barsotti, “In vitro streptococcal adherence on prosthetic and implant materials. Interactions with physicochemical surface properties,” Journal of Oral Rehabilitation, vol. 31, no. 2, pp. 140–148, 2004.