The strain of Salmonella enterica subsp. enterica serovar Enteritidis (S. Enteritidis) used in this study was NCTC13349, kindly provided by Matthew McCusker (Centre for Food Safety and Foodborne Zoonomics, Veterinary Sciences Centre, University College, Dublin, Ireland). This strain was transformed with plasmid pBBC129 for permeability experiments in order to generate S. Enteritidis pBBC129 which produces periplasmic β-lactamase and inner β-galactosidase (as S. Enteritidis lacks the corresponding genes).

Plasmid pBBC129 was generated as follows. The lacZ gene of E. coli MG1655 (F⁻, λ⁻, ilvG⁻, rfb-50, rph-1) (Blattner et al., 1997) was amplified by PCR using the Fidelio polymerase (Ozyme, Saint-Cyr-L’Ecole, France), and the primers TAGCTCACTCATTAGGCAC and AATGGATTTCCTTACGCG, according to the manufacturer’s instructions. The amplified lacZ PCR fragment (3,226 bp) was purified using a QIAquick gel extraction kit (Qiagen, Les Ulis, France) and ligated with EcoRV-digested pBR322 plasmid DNA (Bolivar et al., 1977). The ligation mixture was used to transform E. coli DH5α (F⁻, endA1, glnV44, thi-1, recA1, relA1, gyrA96, deoR, nupG, purB20, φ80dlacZΔM15 Δ (lacZYA-argF)U169, hsdR17(rK⁻ mK⁺), λ⁻) (Meselson and Yuan, 1968) by electroporation. Lac⁺ Amp^R transformants were selected on LB agar containing ampicillin (100 μg/mL), 40 μM X-gal and 1 mM isopropyl-β-D-thiogalactopyranoside (IPTG; Sigma, Saint Quentin-Fallavier, France). Plasmid DNA was then extracted (QIAprep Spin Miniprep Kit, Qiagen), and the identity of the isolated plasmid (designated pBBC129) was verified by restriction digestion analysis. S. Enteritidis NCTC13349 was transformed with pBBC129 to generate S. Enteritidis pBBC129. This strain was used to study outer-and inner-membrane permeabilization. The behavior of this strain in the various media used in this study was determined and was found to be comparable to that of S. Enteritidis NCTC13349 (data not shown).

Before each experiment, S. Enteritidis strains were propagated overnight at 37°C in Tryptone Soy Broth (TSB, Biokar diagnostics, Beauvais, France), and then re-propagated for a further overnight period in the same conditions. For S. Enteritidis pBBC129, 100 μg/mL ampicillin (Sigma) was included in the TSB medium.

EW was prepared from eggs obtained from a conventional hen housing system according to Baron et al. (1997). Eggshell surfaces were sanitized with absolute alcohol. Residual alcohol was removed by briefly flaming the eggshell. Eggshells were then broken, under sterile conditions, and the collected EW was aseptically homogenized with an Ultra-Turrax^® Disperser DI25 Basic (Ika, Grosseron, Saint-Herblain, France) for 1 min at 9500 × rpm. The pH of the isolated EW was 9.3 ± 0.1 and its sterility was confirmed by the absence of growth (for 24 h at 37°C) following addition of 1 mL EW into 20 mL of melted Tryptone Soya Agar (TSA; Biokar Diagnostics, Pantin, France) in a Petri dish.

EWF was prepared by ultrafiltration using a pilot unit (TIA, Bollène, France) equipped with an Osmonics membrane (5.57 m², 10 kDa cut-off; PW 2520F, Lenntech BV, Delft, Netherlands), according to Baron et al. (1997). EWF was sterilized by filtration (Nalgene^® filter unit, pore size <0.2 μm, Osi, Elancourt, France) and then stored at 4°C until use. EWF has the same pH and ionic strength as EW but lacks EW macromolecules above 10 kDa. The composition of EWF was determined by Cochet et al. (2021) and is provided in Table 1.

SM was developed according to the ionic composition of EW and EWF (Table 1) whilst accounting for differences with EWF resulting from chemical elements associated with proteins that are removed during ultrafiltration with a 10 kDa cut-off membrane. As the pH of EW reaches ~9.3 a few days after laying this was an important parameter considered in the design of the SM. Thus, through the inclusion of a 55 mM sodium carbonate/bicarbonate buffer, a pH of 9.3 was obtained. Moreover, this buffer provides a source of sodium and carbonate/bicarbonate ions. This concentration corresponds to the concentration of bicarbonate present in EW, as derived from the hen’s blood and transferred during hydration of EW in the hen’s uterus. In addition, the bicarbonate is also required for the binding of iron to OT (Phelps and Antonini, 1975). Sulfur is the second most abundant element found in EW (50.8 to 56.1 mM), but almost all the sulfur in EW is protein associated, which explains its 78-fold lower concentration in EWF (0.69 mM). Thus, in SM, sulfur was supplied with a concentration of 1 mM in the form of (NH₄)₂SO₄. Chloride is present in EW at a concentration of 49 mM. Thus, KCl, MgCl₂ and CaCl₂ were the three forms of chloride included in the SM for achieving the final concentration of 44 mM. These three chemicals also provide a source of potassium (40 mM), magnesium (2 mM) and calcium (0.25 mM) in SM. In EW, the total nitrogen concentration is very high (1.36 M), but as for sulfur, most of the EW nitrogen is provided in the form of protein. Thus, the ultrafiltration of EW resulted in an ~600-fold reduction in nitrogen concentration in the resulting EWF (to 2.3 mM). For this reason, the nitrogen source in SM was provided by ammonium in the form of 2 mM (NH₄)₂SO₄. The concentration of phosphorus is between 4.2 and 7.1 mM in EW and is partially protein-bound. Thus, a concentration of 2 mM phosphorus in the form of NaH₂PO₄ was included in SM, a concentration that matches that of the EWF. In EW and EWF, the concentration of magnesium is almost the same (between 3 and 4 mM); a source of Mg was provided in SM by the inclusion of 2 mM MgCl₂. The concentration of calcium in EW is between 1.3 and 3 mM, and is 0.96 mM in EWF. Only a 0.25 mM final concentration of calcium was included in SM since precipitation occurred at higher concentrations. This concentration is slightly higher than that of the M9 minimal medium (i.e., 0.1 mM). Iron, zinc, copper and manganese are present in trace amounts in EW (between 1.5 and 1.85 μM) and in EWF (between <0.02 and 0.98 μM), so these elements were not specifically added to SM as they were already present in trace amounts in SM. A source of sugar is essential for bacterial growth. In EWF, like in EW, glucose is the dominant form of carbohydrate with a concentration of ~20 mM. The same quantity was therefore provided in the SM.

SM (pH was 9.3 ± 0.1) was thus prepared by adding the following, in the order given, which were dissolved in ultrapure water: 1 mM (NH4)₂SO₄ (Panreac, Barcelona, Spain), 2 mM Na₂HPO₄ (Merk, Darmstadt, Germany), 40 mM KCl (Merck), 20 mM glucose (Merck), 2 mM MgCl₂ (Merck), 0.25 mM CaCl₂ (Sigma) and 55 mM sodium carbonate buffer (pH 9.3). Finally, the SM was sterilized by filtration (Nalgene^® filter unit, pore size <0.2 μm) (see Table 1).

Apo-OT was purchased from Sigma and is substantially iron free. OT was prepared in EWF or in SM at concentrations ranging from 1.3 to 13 g/L, corresponding to 10 and 100% of the theoretical concentration found in EW. For some experiments, ferric citrate (Sigma) was added to obtain a theoretical OT saturation from 10 (33.4 μM) to 110% (367 μM). The OT solutions were sterilized by filtration, as above.

Salmonella Enteritidis growth was compared after 24 h incubation at 30°C in: EW, EWF, SM or EWF; with or without 10% EW, 1.3 g/L of apo-OT, 13 g/L of OT iron saturated (from 0 to 110% of theoretical saturation) OT. S. Enteritidis NCTC13349 was twice passaged overnight at 37°C in TSB and then centrifuged for 7 min at 5,600 g and 15°C. The cell pellets were washed three times in tryptone salt medium (TS, 8.5 g/L NaCl, 1 g/L Tryptone). Bacterial cells were then diluted and inoculated at 2% of the original volume in a final volume of 800 μL of the corresponding medium, to give 5 log₁₀ CFU/mL. The diluted cultures were then propagated in a 96-well plates of 2.2 mL well volume (Starlab, Bagneux, France) with 800 μL applied per well. Enumeration of S. Enteritidis cells was performed after 24 h of incubation at 30°C in TSA, using a rapid and cost-effective method previously described by Baron et al. (2006). Experiments were performed with three biological replicates and three technical replicates. Statistical analysis was performed using one-way ANOVA followed by a Tukey Contrast test, using R software (version 1.4.1106).

Membrane permeabilization was determined spectroscopically using a method adapted from Lehrer et al. (1988) and Derde et al. (2013). As previously described for E. coli ML-35p, β-lactamase and β-galactosidase activities were measured to detect outer-and inner-membrane permeabilization, respectively (Derde et al., 2013; Lehrer et al., 1988). For this experiment, S. Enteritidis pBBC129 was used to allow production of β-lactamase and β-galactosidase.

After propagation as indicated above, the culture was centrifugated at 7,000 x g for 7 min at 15°C, washed three times with TS and then the OD_600nm (Colourwave Colorimeter WPA CO7500, Biochrom, Holliston, United States) was adjusted to 0.35 in the same medium. TS medium (270 μL) containing the β-lactamase substrate, nitrocefin (Sigma), at 30 mM or the β-galactosidase substrate, ortho-nitrophenyl-β-galactopyranoside (ONPG), at 2.5 mM (Sigma), prepared in 10 mM phosphate buffer (pH 7.4), was applied to a 96-well microtiter plate. Then, 30 μL of bacterial suspension were added. Polymyxin B (50 μg/mL) (Sigma), a polypeptide antibiotic, was used as a positive control for the permeabilization of the outer membrane. Melittin (15 μg/mL) (Sigma), an amphipathic cytotoxin derived from bee venom, was used as a positive control for the permeabilization of the inner membrane. The plate was then incubated in a Spectramax M2 spectrophotometer (Molecular Devices, San Jose, United States) at 30°C for 5 h. Absorbance values were read at 490 and 405 nm to measure HP nitrocefin release (for outer-membrane permeabilization) and ONP production (for inner-membrane permeabilization), respectively. According to Derde et al. (2013), the intersection of the baseline and the tangent to the curve at the point where the rate is maximal (defined as “Vmax” here) were used to calculate the lag time (delay between outer-and inner-membrane permeabilization). The enzymatic reaction rate was determined using the following formula, ∆A_nm/30 min*10³, and was expressed in milliA_nm/min. Experiments were performed with three biological and three technical replicates. Statistical significance was determined as indicated above.

A spectrofluorescent method adapted from Epand et al. (2010) was used to detect depolarization of the inner membrane of S. Enteritidis. A change in membrane potential was detected using 3,3′-diopropylthiadicarbocyanine iodide (DiSC₃(5), Sigma), a lipophilic potentiometric dye. Bacteria were grown as previously described, and then ten-fold diluted in TSB and incubated for 3.5 h at 37°C. Bacteria were centrifuged (5,600 g for 7 min at 15°C) and washed three times in HEPES buffer (5 mM HEPES, 5 mM glucose, pH 7.2) before resuspension in the same buffer to give an OD_600nm of 0.5. The cells were then charged using a 20 μM DiSC₃(5) solution and 100 mM KCl, to balance cytoplasmic and external K⁺ concentrations. The mix was incubated for 15 min at 37°C in the dark to stabilize the dye signal. Then, cells charged with DiSC₃(5) were diluted 10 times in various media and incubated for 10 min at 30°C. Fluorescent measurements corresponding to the disruption of the membrane potential gradient (ΔΨ) were made using a spectrofluorometer (Molecular Devices Spectra, MAX Gemini XS) at an excitation and emission wavelengths of 622 and 670 nm, respectively. Three biological and technical replicates were performed. Results are expressed in relative fluorescent units (RFU). Statistical analysis was determined as above.

The cell surface morphologies of S. Enteritidis were compared after 24 h incubation at 30°C in TSB, SM or SM with apo-OT (13 g/L). S. Enteritidis NCTC13349 was twice passaged overnight at 37°C in TSB and then centrifuged for 7 min at 5600 g and 15°C. The cell pellets were washed three times in TS. Bacterial cells were then diluted and inoculated at 2% in SM or in SM with apo-OT (13 g/L) to give an initial inoculum of 7 log₁₀ CFU/mL. After 24 h incubation at 30°C, 2 mL of each cell suspension were placed onto a 0.20 μm pore-size membrane filter (Millipore-Isipore, Merck) and fixed for 1 day in 0.1 M sodium cacodylate buffer (pH) containing 2.5% glutaraldehyde (Sigma-Aldrich). Samples were then washed four times for 15 min in 0.1 M sodium cacodylate buffer and postfixed for 1 h with 0.1 M sodium cacodylate buffer containing 1% OsO₄ (Euromedex). The samples were then dehydrated with a graded ethanol series (10, 25, 50, 75 and 95% ethanol; 15 min at each concentration) followed by treatment with 100% ethanol for 2 h. Samples were then metallized with gold palladium (Sigma-Aldrich). Microscopy was performed with a Jeol-6400F microscope (Olympus) and electron microscopy images were taken at 7 kV. The lengths of 30 cells for each condition (TSB, SM and SM with apo-OT at 13 g/L) were measured and statistical analysis was performed as above.

Studying the antimicrobial impact of a particular EW protein (such as OT) under EW conditions is a challenge largely due to the complex physical and chemical properties of EW, and because of the presence of numerous proteins. One solution to this problem has been the use of EWF, generated by ultrafiltration of EW using a 10 kDa cut-off membrane (Baron et al., 1997) thus removing macromolecules >10 kDa but preserving the pH and ionic composition of EW. However, EWF is not peptide-free and a recent study has highlighted the presence of antimicrobial <10 kDa peptides in this medium (Cochet et al., 2021) which could potentially interfere with OT activity.

Since no suitable EW synthetic medium was available, a medium (designated SM; see Methods and Table 1), closely-matching the ionic composition and pH of EW, was developed using the ionic compositions of EW and EWF as guides (Ciqual, 2024; Cochet et al., 2021; Nau et al., 2010; Nys and Sauveur, 2004; Sauveur, 1988; Stadelman and Cotterill, 1995).

In order to consider the suitability of SM as a model EW medium, S. Enteritidis growth was compared in SM and EWF over a 24 h period at 30°C (a temperature that allows growth in EW and EWF) in SM with/without 10% EW. The egg-based media, EWF and EWF with 10% EW, were used as controls. The results showed that S. Enteritidis growth is similar in EWF and SM (i.e., cell number increased by 3.5 and 3.6 log₁₀ CFU/mL, respectively) (Figure 1). A growth reduction of ~1,000 fold for S. Enteritidis was observed in both media after addition of 10% EW (i.e., cell number increased by only 0.4 and 0.9 log₁₀ CFU/mL for SM and EWF, respectively). These values are similar to those obtained after 24 h incubation in EW at 30°C (i.e., cell number increased by 0.3 log₁₀ CFU/mL, data not shown). A growth reduction of ~100 fold for S. Enteritidis was observed in both media after addition of apo-OT (1.3 g/L; i.e., at 10% of its concentration in EW). S. Enteritidis growth after addition of apo-OT was only slightly, although significantly, higher in SM than to EWF (i.e., cell number increased by 1.6 and 1.1 log₁₀ CFU/mL, respectively). The results thus indicate that the antimicrobial activity of EW and OT are exhibited to similar degrees in both SM and EWF. The antimicrobial effect of EW, and EWF with 10% EW, on S. Enteritidis have been previously reported by Baron et al. (1997, 2017, 2020). The slight difference in the impact of apo-OT (at 1.3 g/L) on growth in SM with respect to that seen in EWF may be caused by the presence of antimicrobial peptides in EWF (Cochet et al., 2021), which are not present in SM. In summary, these results indicate that SM is a suitable medium for studying the impact of OT on S. Enteritidis in conditions mimicking EW (i.e., same pH and ionic composition) and offers an advantage over EWF since it is entirely free of proteins or peptides.

The antibacterial activity of OT is considered to be mediated by the iron deficiency that it imposes upon EW. This view is supported by numerous studies demonstrating that iron supplementation promotes bacterial growth in EW (Baron et al., 1997; Garibaldi, 1970; Lock and Board, 1992). To determine whether OT might have an antibacterial action beyond iron restriction, the contribution of the iron-restriction activity of OT to the antibacterial activity of EW was further investigated in this study. Thus, S. Enteritidis was incubated in SM with 13 g/L of iron-saturated (0 to 110%) OT. After 24 h at 30°C, S. Enteritidis was subject to a substantial growth restriction by provision of OT iron-saturated at 0 to 50% (i.e., cell number increased by just 0.4–0.7 log₁₀ CFU/mL) (Figure 2). However, at above 50% OT iron-saturation, S. Enteritidis growth was little impacted by OT (i.e., cell number increased by between 3.5–3.7 log₁₀ CFU/mL) (Figure 2). These results confirm that the iron-chelating activity of OT is responsible for the restriction of S. Enteritidis growth at 30°C, under EW conditions. It should be noted that OT suppressed growth in SM more severely when supplied at 13 g/L than at 1.3 g/L (growth increased by 0.4 ± 0.06 and 1.6 ± 0.14 log₁₀ CFU/mL, respectively; Figures 1, 2), indicating a clear concentration-dependent effect.

The effect of OT’s iron-restriction impact on the growth of S. Enteritidis is well established in the literature, but this is not the case for any effect that OT may have on the membrane integrity of S. Enteritidis. Thus, to explore whether OT can induce permeabilization of the outer and/or inner membranes of S. Enteritidis, a strain (S. Enteritidis pBBC129) expressing β-lactamase and β-galactosidase was generated and deployed. This enabled measurement of substrate accessibility to β-lactamase and β-galactosidase in the periplasm and cytoplasm, respectively, in response to outer-and inner-membrane permeabilization, respectively (Derde et al., 2013; Lehrer et al., 1988).

The results show that outer-and inner-membrane permeabilization progressed steadily with incubation time as S. Enteritidis was exposed to the different conditions at 30°C (Figures 3A,B). For outer-membrane permeabilization (Figures 3A,C), the peptide-antibiotic polymyxin B was used as a positive control. Within the first few minutes of exposure to polymyxin B, β-lactamase activity increased rapidly (Vmax of 11.2 ± 2.1 milli-A_490nm/min), indicating rapid permeabilization of the outer membrane of S. Enteritidis (Figures 3A,C). β-Lactamase activities were also observed upon EW exposure, but significant differences were observed with respect to the other media employed. In SM, the β-lactamase activity was significantly lower (Vmax of 1.4 ± 0.3 milli-A_490nm/min) than in EW (Vmax of 4.4 ± 0.4 milli-A_490nm/min) or in SM with 13 g/L of apo-OT (Vmax of 7.2 ± 0.6 milli-A_490nm/min) (Figures 3A,C). These results indicate that the S. Enteritidis outer membrane is permeabilized by both EW and apo-OT exposure, and that apo-OT (at the concentration corresponding to that in EW) provokes a more drastic permeabilization than EW with a significant difference between EW and SM containing 13 g/L of apo-OT (Vmax of 4.4 ± 0.4 and 7.2 ± 0.6 milli-A_490nm/min, respectively). This difference may well be explained by the presence of proteins or peptides in EW that could reduce the impact of OT on the S. Enteritidis membrane.

For the inner-membrane permeabilization studies, melittin (an amphipathic cytotoxin derived from bee venom), was used as a positive control. A high β-galactosidase activity was observed in the presence of melittin (Vmax of 15.6 ± 4.2 milli-A_405nm/min) along with a relatively short lag time (13 ± 6 min corresponding to the delay between the outer and inner membrane permeabilization), indicating a major permeabilization of the inner membrane (Figures 3B,D). EW also induced a permeabilization of the inner membrane, but this was 2.5-fold weaker than seen for melittin (Vmax of 6.3 ± 0.9 milli-A_405nm/min; lag time of 127 ± 6 min) (Figures 3B,D). Inner-membrane permeabilization was significantly higher in EW than in SM or in SM with apo-OT at 13 g/L (Vmax of 3.2 ± 0.6 and 3.7 ± 0.7; lag times 122 ± 13 min and 141 ± 20 min, respectively) (Figures 3B,D), and there was no significant difference between SM and SM with apo-OT at 13 g/L. These results indicate that OT does not lead to inner-membrane permeabilization and suggest that other EW-proteins are responsible for the weak inner-membrane disrupting effect observed in EW.

To confirm the impact of apo-OT on the permeabilization of the S. Enteritidis outer membrane and the absence of any effect of apo-OT on the inner membrane, the effect of apo-OT at 0 to 13 g/L was tested in SM (Figures 4A,B). Results show that the β-lactamase activity progressively increased with apo-OT concentration (Figure 4A) whilst β-galactosidase activity remained relatively unchanged as apo-OT concentration increased (Figure 4B). These results thus further support the ability of apo-OT to induce permeabilization of the outer membrane of S. Enteritidis at 30°C. The strongest outer-membrane permeabilization effect was obtained at the highest apo-OT concentration employed which corresponds to the concentration (13 g/L) found in EW. In contrast, apo-OT was not able to permeabilize the inner membrane to any notable degree.

To explore the role of the iron-chelating activity of OT, the impact of OT saturation by iron on the permeabilization of the outer and inner membranes of S. Enteritidis was investigated at 30°C (Figure 5). For this purpose, OT (at 13 g/L, the concentration found in EW) was 0 to 110% iron-saturated using iron citrate, in SM. The results indicate that the ability of OT to disrupt the outer membrane is independent of its degree of iron-saturation (Vmax of 7.35 ± 0.63 and 7.25 ± 0.86 at 0 and 110% iron saturation of OT, respectively; Figure 5A). These results suggest that the metal-chelating activity and iron status of OT do not influence the ability of OT to permeabilize the outer membrane of S. Enteritidis. For the inner membrane, 110% iron-saturated OT induced a slightly, but not significantly, higher level of inner-membrane permeabilization than apo-OT (Figure 5B). These results suggest that apo-OT and iron-saturated OT have no notable impact on inner membrane permeabilization.

Although apo-OT was found not to induce permeabilization of the inner membrane, it remained possible that it could induce a depolarization effect. Therefore, the impact of apo-OT on the depolarization of the S. Enteritidis inner membrane was investigated using the DiSC₃(5) fluorescent probe (Epand et al., 2010). Initially, depolarization of the inner membrane was measured after 10 min incubation at 30°C in response to melittin, as positive control (Figure 6A). The fluorescence reached an intensity of 344 ± 76 relative fluorescent units (RFU) and was significantly 3.6-fold greater than that obtained in response to 5 mM HEPES (pH 7.2), used as negative control (95 ± 8 RFU; data not shown). After 10 min exposure to EW, the RFU reached a similar level as with melittin (372 ± 117 RFU), indicating the ability of EW to induce inner-membrane depolarization. However, when SM was applied in the absence of any EW proteins or peptides, the level of fluorescence achieved was low (100 ± 20 RFU, similar to the 5 mM HEPES negative control at 95 ± 8 RFU; data not shown) which indicates that EW proteins/peptides are responsible for the major depolarization effect caused by EW (Figure 6A).

Salmonella Enteritidis was also exposed to apo-OT in SM, at concentrations ranging from 1.3 to 13 g/L (Figure 6A). No notable depolarization effect was detected for apo-OT at 1.3 g/L (99 ± 25 RFU) with respect to that obtained with SM (100 ± 20 RFU). However, a depolarization effect was observed at higher apo-OT concentrations, which an increased effect obtained as the apo-OT concentration was raised (Figure 6A). Indeed, at the concentration found in EW (i.e., 13 g/L), apo-OT caused an 83% increase in the degree of membrane depolarization (from 100 to 183 ± 37 RFU). It should be noted that the raised depolarization effect caused by apo-OT provision (with respect to SM) only became significant when apo-OT was provided at its concentration found in EW (13 g/L). This effect of 13 g/L apo-OT was significantly lower than observed for EW (372 RFU ± 117). Thus, these findings indicate that OT is at least partly responsible for the depolarization of the inner membrane observed in response to EW, but also suggest that OT is not the only EW component involved in the EW-induced depolarization of the S. Enteritidis inner membrane.

To confirm these results and to explore any impact of the metal-chelation activity of apo-OT on the depolarization effect, the depolarization of the inner membrane of S. Enteritidis was examined in response to 0 to 110% iron-saturated OT (13 g/L) (Figure 6B). The results show that as the degree of OT iron-saturation increased, there was a corresponding reduction in the level of OT-induced depolarization of the S. Enteritidis inner membrane (maximum reduction of 1.5-fold; Figure 6B). However, it should be noted that only OT at 110% iron-saturation (112 ± 8 RFU) gave a depolarization effect that was significantly lower than that observed for unsaturated OT (168 ± 12 RFU).

To confirm the impact of OT on the S. Enteritidis envelope, the cell surface was examined by SEM. The cells were significantly shorter in SM (1.39 +/− 0.30 μm) and in SM + OT (1.24 +/− 0.35 μm) in comparison with their length in TSB (1.56 +/−0.32 μm). S. Enteritidis cells propagated in TSB display a relatively smooth and intact surface (Figures 7A,B). Those propagated in SM possessed a more corrugated surface although this effect was minor and the surface appeared intact (Figures 7C,D). After incubation in SM with apo-OT (13 g/L), the cells seemed more compact, displayed a granular surface and some showed shape deformation and/or pitting (Figures 7E,F). However, no evidence of cell lysis or cell debris was observed. These results thus indicate that apo-OT (at 13 g/L) induces a major morphological change, without lysis, on the S. Enteritidis cell surface under EW conditions.