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Inhibition and Interactions of Campylobacter jejuni from Broiler Chicken Houses with Organic Acids

Campylobacter jejuni is a bacterium that causes major diarrheal disease worldwide and is also one of the top five foodborne pathogens encountered in the United States. Poultry is a major source of C. jejuni, and a high-risk factor for contracting campylobacteriosis. Organic acids are used in the United States during food animal processing for removal of bacterial contamination from animal carcasses. Six organic acids were evaluated in inhibition studies of 96 C. jejuni strains obtained from shoe covers used in broiler chicken houses at different poultry farms in several states by determining the susceptibilities of the C. jejuni strains, along with the pH values at the molar minimum inhibitory concentrations (MICMs). The undissociated and dissociated organic acid concentrations were calculated at the MICMs with the Henderson-Hasselbalch equation. The results for the 96 C. jejuni strains were treated similarly for each different organic acid. Campylobacter jejuni inhibition did correlate with the dissociated organic acids, but did not correlate with pH or with the undissociated organic acids. When the concentrations of dissociated organic acids decreased, the C. jejuni strains were not disinfected. A carcass wash using organic acids should have the concentration of dissociated acid species carefully controlled. It is suggested to maintain a dissociated acid concentration for propionic, l-lactic, formic, citric, butyric, and acetic acids at 24, 40, 36, 21, 23, and 25 mM, respectively, and at these dissociated organic acid levels an acid wash would be expected to remove or inhibit 97% or more of the C. jejuni bacteria studied here. However, studies must be undertaken to confirm that the suggested concentrations of dissociated organic acids are adequate to remove C. jejuni bacteria in the field vs. the laboratory. Due to propionate, l-lactate, formate, butyrate, and acetate being utilized by C. jejuni, these organic acids may not be appropriate for use as a carcass wash to remove C. jejuni surface contamination. Of all tested organic acids, dissociated citric acid was the most efficient at inhibiting C. jejuni.


Introduction
Campylobacter jejuni is a bacterial organism that causes gastroenteritis worldwide [1][2][3][4][5][6]. Campylobacter jejuni are Gram-negative bacteria that are non-spore-forming [7] and are known to be a major cause of diarrheal disease in humans [8]. Campylobacter species are within the top five of the 31 major foodborne pathogens in the United States, and the Centers for Disease Control and Prevention (CDC) has estimated that each year, Campylobacter species cause 845,024 illnesses, 8,463 hospitalizations, and 76 deaths in the U.S. [9,10]. The two main Campylobacter species usually associated with human foodborne illnesses worldwide are C. jejuni and C. coli [2,[11][12][13]. These two bacteria have high DNA homology [14], with related or identical antigens [15]. The most bacterial foodborne illnesses in the United States in 2016 were a result of Campylobacter and Salmonella, as described by the CDC [16]. However, most human Campylobacter infections are caused by C. jejuni [2,4,8,17]. Poultry have been found to be a major source of C. jejuni exposure, and consuming poultry food products is recognized as a high-risk factor for contracting campylobacteriosis [18][19][20][21][22][23]. Campylobacter infections may be fatal among young children, the elderly, and immunosuppressed patients (HIV patients) [6,24]. In particular, the incidence of Campylobacter infections in children <2 years of age in Israel has increased over the last few years to become the highest among industrialized countries [23]. A C. jejuni infective dose of only about 500-800 bacteria are required for infection [25,26].
New strategies to control animal-derived foodborne pathogens from the farm-to-fork must be developed to prevent illness due to these pathogens [27]. An important step used in the United States in the meat processing plant is a surface animal carcass wash containing organic acids (OAs) to remove bacterial contamination. Some short-chain OAs have been used to remove C. jejuni from avian carcasses in poultry processing plants [28][29][30][31], and studies using OAs have been conducted to remove or reduce C. jejuni populations in live birds during grow-out and preslaughter feed withdrawal [31][32][33][34][35][36]. The remaining bacteria found on carcasses in processing plants may later proliferate and be found on the processed meat, and meat marination studies have also been conducted using OAs to remove foodborne pathogens on the resulting processed chicken meat [37].
In previous studies designed to evaluate foodborne pathogen interactions with OAs, molar units for concentration were used for the minimum inhibitory concentrations (MIC M s) of the OAs when comparing pH, and undissociated and dissociated OA data, because it results in an accurate analysis between MIC results of OAs with different molecular weights [48]. Our previous studies evaluated Escherichia coli O157:H7 [48], non-O157 Shiga toxin-producing E. coli (non-O157 STECs) [49], Salmonella enterica serovars [50], vancomycin-resistant Enterococcus faecium (VRE) [51], and C. coli [52] against OAs. These studies against OAs showed no correlation between pH or the undissociated OAs and bacterial MIC M s. However, the dissociated OAs did show a close correlation with the MIC M s, and the disintegration of a bacterial LPS layer has been demonstrated by a dissociated OA [53]. It was observed in previous research that bacteria would be expected to escape disinfection if the concentration of the dissociated OAs decreased below optimum levels [48][49][50][51][52].
Here, we studied the interactions of 96 C. jejuni strains isolated from shoe covers used in broiler chicken houses at different poultry farms in several different states with a number of OAs. Susceptibility studies were conducted with the 96 C. jejuni strains against the OAs, propionic, l-lactic, formic, citric, butyric, and acetic acid, and the pH was determined at the MICs. Calculations of the concentrations of undissociated and dissociated OAs at the MIC M s were undertaken. The pH and concentrations of the undissociated and dissociated OA species are compared at the MIC M s for all C. jejuni strains and show a good association between the dissociated OA species and bacterial inhibition.

Campylobacter jejuni
Campylobacter jejuni strains (n = 96) were isolated from broiler chicken houses at different poultry farms in several different states. Two shoe covers (97041-234, VWR, Missouri City, TX, USA) were placed into an autoclavable plastic container with 100 mL of 2× skim milk (232100, Difco™, Becton, Dickinson and Company, Sparks, MD, USA) and autoclaved for 15 min at 121 • C. Four pairs of shoe covers were used for each chicken house. The shoe covers were placed over boots and used as swabs to collect bacteria from the litter on the chicken house floor. The shoe covers were worn while walking 1 2 the length of the house on one side, and then they were removed and replaced with two fresh shoe covers. When reaching the end of the house, this process was repeated for the walk back to the front of the house. The four pairs of exposed shoe covers were packed in an ice chest and shipped to the laboratory. After arrival at the laboratory, 90 mL of buffered peptone water (212367, BBL™, Becton, Dickinson and Company, Sparks, MD, USA) was added to each pair of shoe covers and shaken. Samples were subjected to direct plating (one plate directly from each sample) and one from a 1:10 peptone water dilution (for a total of two plates) for enumeration on Campy-cefex agar (C-C) plates [54], and were incubated at 42 • C in a microaerobic environment (5% O 2 , 10% CO 2, 85% N 2 ) for 48 h. Additionally, 5 mL of each peptone water sample was added to 5 mL of 2× Bolton enrichment broth [54] and incubated at 42 • C overnight. The samples were then plated onto C-C plates and incubated at 42 • C in the microaerobic environment for 48 h. Five colonies from each positive C-C plate were isolated and placed on trypticase soy agar w/5% sheep blood BD BBL™ Stacker™ (TSA) plates (#221261, Becton, Dickinson and Company, Sparks, MD, USA) in an anaerobic chamber (5% H 2 , 5% CO 2 , 90% N 2 ), and then transferred to Brucella Broth (211088, BBL™, Becton, Dickinson and Company, Sparks, MD, USA) containing 20% glycerol (GX0185-5, EM Science, Gibbstown, NJ, USA) and placed at −80 • C for storage. Samples were also sent to the National Antimicrobial Resistance Monitoring System (NARMS) for Sensititre™ antimicrobial susceptibility testing.

Susceptibility Testing of C. jejuni Strains with Organic Acids
The C. jejuni OA MICs were obtained by using broth microdilution testing for fastidious bacteria, as described by the Clinical and Laboratory Standards Institute (CLSI) [55] and the TREK Diagnostic Systems published method for determining susceptibility using Campylobacter sensititre plates [56]. The susceptibility studies carried out here required Campylobacter incubation at 42 • C for 48 h because some strains did not sufficiently grow in 24 h, as was also observed in an earlier Campylobacter coli study [52]. Briefly, 50 µL of cation-adjusted Mueller-Hinton broth w/TES w/Lysed horse blood (Remel, Lenexa, KS, USA) was added to wells 2-12 of a 96-well U-bottom Greiner bio-one microplate (#650161, VWR International, LLC, Bridgeport, NJ, USA), and 50 µL of each standard OA solution was added to wells 1 and 2, and the solution in well 2 was further diluted 1:2 across the microplate through column 11, and the wells in column 12 were the positive controls [52]. Campylobacter jejuni colonies were then selected from TSA plates, and diluted into tubes containing 5 mL cation-adjusted Mueller-Hinton broth w/TES (Remel, Lenexa, KS, USA) to be equivalent to a 0.5 McFarland standard using a TREK Diagnostic Systems Nephelometer (East Grinsted, UK). Because the wells in the organic acid susceptibility plates contain a final volume of 100 µL, 200 µL of the 0.5 McFarland suspension was then added to tubes that contained 11 mL Mueller-Hinton broth w/TES w/Lysed horse blood, resulting in 1 × 10 6 CFU/mL of each bacterial isolate, as previously described [52]. The horse blood bacterial solution (50 µL/well) was added to each well of the 96-well plates. A perforated plastic adhesive cover sheet (YG522EA, Remel) was placed over the bacteria-loaded microplates, and the covered plates were placed in the BD GasPak™ EZ incubation containers (Becton, Dickinson and Company, Sparks, MD, USA). Sachets (BD #260680) were enclosed in the EZ containers according to the manufacturer's instructions, along with a 100 mL beaker half full of water to provide a moisturized atmosphere, and the containers were closed. This system provided a microaerobic atmosphere, where they were incubated for 48 h at 42 • C. The microplate well containing the smallest OA concentration that had no visible bacterial growth was considered the minimum inhibitory concentration (MIC) [57], as observed on a SensiTouch imaging system (TREK Diagnostic Systems Ltd., East Grinsted, UK). Campylobacter jejuni ATCC 33560 was run along with each test as the control organism. The results obtained here for ATCC 33560 were compared with results obtained from testing these same OAs against the control organism Escherichia coli ATCC 25922 in aerobic conditions, as ATCC 25922 was used as the control organism during all previous aerobic OA susceptibility testing studies [48][49][50][51][58][59][60][61].
2.3. Determination of pH in Wells of the 96-Well Microplates at the C. jejuni MICs pH analysis was performed as previously described [52]. Briefly, the pH was determined of the solutions in the MIC wells for all OAs in triplicate, and the means and standard deviations were calculated. The solutions at the same MIC from 16-wells (100 µL/well) for each OA were added together (for a total of 1600 µL) in a 5 mL sterile microtube (Argos Technologies, Inc., Vernon Hills, IL, USA). An Orion benchtop pH meter with a ROSS Ultra glass combination pH electrode was used to determine the pH (Thermo Fisher Scientific, Chelmsford, MA, USA).

The Calculated Ratio of Undissociated/Dissociated OAs
It is well-known that when the pH and pK a are known, the ratio of the undissociated/dissociated weak organic acid concentration can be calculated using the Henderson-Hasselbalch equation [62]: where pK a is equal to the −log 10 of the organic acid dissociation constant (K a ), [A -] is the molar concentration of the conjugate base (dissociated organic acid), and [HA] is the molar concentration of the undissociated organic acid [62]. Rearrangement of the Henderson-Hasselbalch equation can provide the ratio of the undissociated/dissociated weak organic acid [40]: The ratio of the undissociated/dissociated acid can then be calculated using the published pK a of each OA and the results of the measured pH at the MICs. The pK a for propionic, l-lactic, formic, citric, butyric, and acetic acid is 4.87, 3.86, 3.75, 3.14, 4.82, and 4.75, respectively. The pH was experimentally determined, the molar concentrations of the OAs are known at the bacterial MICs, and the molar concentrations of the undissociated and dissociated OA species at each MIC can then be calculated from the ratio obtained from the Henderson-Hasselbalch equation [48][49][50][51][52].

Statistics
The central tendency of the organic acid MICs and MIC M s for the 96 C. jejuni strains isolated from chicken houses was defined by showing the 90th percentile, range, mode, and median of the data. The mean and standard deviation of triplicate pH samples at each MIC for each OA were calculated. Table 1 presents the MICs and MIC M s data determined for the 96 C. jejuni strains against all the OAs evaluated. l-Lactic and formic acid MIC M s demonstrated the greatest levels of OAs needed to inhibit all the C. jejuni strains tested (90.94 and 89.0 mM), respectively. The OA molar concentration required for inhibition of C. jejuni by these two acids was followed by the molar concentrations of acetic, propionic, and butyric acid of 68.21, 55.29, and 46.49 mM, respectively. The lowest molar concentration required to inhibit the C. jejuni strains was for citric acid (21.32 mM). The C. jejuni citric acid MIC M concentrations were by far the lowest levels observed of all the OAs tested. The central tendency of the MIC data is shown in Table 2. The central tendency is a typical value found for a probability distribution. The highest median values are for l-lactic acid, formic acid, and butyric acid of 22.74, 22.25, and 23.24 mM, respectively, while the highest range values are for l-lactic acid, formic acid, acetic acid, and propionic acid of 90.94, 89.00, 68.21, and 55.29 mM, respectively, and the 90th percentile follows the highest range values for l-lactic, formic, and acetic acid of 45.47, 44.50, and 34.10 mM, respectively, except for butyric and propionic acid of 23.25 and 13.82 mM, respectively.

Experimentally Determined pH at the C. jejuni MICs for the 96 Strains Evaluated with the OAs
The 96 C. jejuni strains were grouped together as one group for each OA; therefore, the six OAs resulted in six OA groups, each containing 96 strains. The experimentally determined pH values of the 96-well plates at the C. jejuni MIC M s are shown in a graphical presentation in Figure 1. Triplicate samples were evaluated at each pH data point, and the number of strains at each MIC M is depicted next to each data point. The pH necessary to inhibit 100% of the strains with butyric acid was 5.14, and that for 99% of the strains with propionic, citric, and acetic acid was 5.74, 5.58, and 5.18, respectively. However, the MIC M pH for 99% of the bacterial strains evaluated with formic acid and 97% of the strains against l-lactic acid was 4.4 and 4.39, respectively. The pH value needed for inhibition of 97-100% of C. jejuni against the six OAs falls into two different pH groupings, which has, on average, 1.01 pH unit difference. The pH at 100% inhibition of the C. jejuni strains against formic acid and l-lactic acid is 3.71 and 3.74, respectively. Using these values, the pH difference for the two groupings with 100% of the strains being inhibited by formic acid and l-lactic acid is, on average, 1.69 pH units.  Figure 3 shows the pH vs. undissociated OA concentrations at the MICMs of the six OAs against the 96 C. jejuni strains. The number of C. jejuni strains at the MICM is displayed adjacent to each data point.
Most of the C. jejuni strains were inhibited by undissociated OAs at concentrations approaching zero. The difference in the points where both citric acid and L-lactic acid inhibit 100% of the strains is approximately 51 mM undissociated OA and a Δ pH = 0.74 unit. At the points where 97% of the strains were inhibited by undissociated butyric acid and all 96 strains were inhibited by undissociated citric acid, the undissociated OA concentrations approach zero and the Δ pH = 1.97 unit. At the points where 99% of the strains were inhibited by undissociated acetic acid and propionic acid, there is approximately a 5 mM difference in undissociated OA concentrations and the Δ pH = 0.56 unit.

Calculated Dissociated OA Concentrations at the C. jejuni MICMs
The dissociated OA concentrations of propionic, L-lactic, formic, citric, butyric, and acetic acids calculated using the Henderson-Hasselbalch equation at the MICMs of the 96 C. jejuni strains are shown in Figure 4. The dissociated OA concentrations required to produce MICMs for all 96 C. jejuni strains by citric acid and 99% of the strains by propionic acid and acetic acid and 97% of the strains by butyric acid are shown by the narrow, darker-shaded band in

283
Food processing plants often base pathogen decontamination strategies on pH [63,64]. Organic acids 284 are regularly used to remove foodborne bacteria from poultry carcasses in the United States [28][29][30].

285
However, many foodborne pathogens have acid stress mechanisms that can help them adapt to varying 286 pH environments [38,[65][66][67][68]. Campylobacter jejuni has the gene make-up required to induce an acid-287 tolerance response [68]. In addition, there is an increase of acid tolerance in C. jejuni caused by 288 coincubation with protozoa [69], and the genes involved in iron control and uptake are also induced 289 [67,68]. We evaluated the interactions of six different OAs-propionic, L-lactic, formic, citric, butyric, and

Discussion
Food processing plants often base pathogen decontamination strategies on pH [63,64]. Organic acids are regularly used to remove foodborne bacteria from poultry carcasses in the United States [28][29][30]. However, many foodborne pathogens have acid stress mechanisms that can help them adapt to varying pH environments [38,[65][66][67][68]. Campylobacter jejuni has the gene make-up required to induce an acid-tolerance response [68]. In addition, there is an increase of acid tolerance in C. jejuni caused by coincubation with protozoa [69], and the genes involved in iron control and uptake are also induced [67,68]. We evaluated the interactions of six different OAs-propionic, l-lactic, formic, citric, butyric, and acetic-against 96 C. jejuni potential foodborne pathogen strains, while evaluating the effects that pH and the undissociated and dissociated OA species have on the bacteria at their OA MIC M s.
The central tendency of the MIC data show that median MIC M values for butyric, l-lactic, and formic acid necessary for inhibition of the same strains have the highest values and the median acetic acid MIC M necessary for inhibition of the C. jejuni strains has an intermediate value, while the median MIC M values for inhibition by propionic and citric acid have the lowest values. However, l-lactic acid, followed by formic acid and acetic acid, have the highest ranges of MIC M values, and l-lactic acid and formic acid have the highest 90th percentile values, while citric acid has the lowest overall inhibition concentration (10.66 mM). The citric acid 90th percentile value is the same value as was observed for citric acid in a previous study of C. coli [52]. It has previously been shown that citrate cannot be utilized by whole cells of Vibrio fetus (Campylobacter fetus) as an alternative energy source [70], nor by C. jejuni from swine [71]. Our data also suggests that citric acid is not utilized by C. jejuni, thereby making citric acid a good candidate to be used for disinfection of this bacterium.

Differences in pH Between Solutions of Different OAs at the MIC M
Interestingly, it took a pH of 4.39 and 4.4 to inhibit 97% and 99% of the strains by l-lactic acid and formic acid, respectively, while it took a pH of 6.45, 5.74, 5.58, and 5.18 to inhibit 97%, 99%, 99%, and 99% of the strains by butyric, propionic, citric, and acetic acid, respectively. This is an average of 1.34 pH unit difference between the pH necessary to inhibit 97-99% of the same 96 C. jejuni strains by these two groups of acids. We have reported pH differences at the MIC M s of other Gram-negative strains against OAs, and only one other bacterium had a greater pH difference between inhibition of all strains, C. coli with a 1.76 pH unit difference [52]. The inhibition of 98% of 175 Pseudomonas aeruginosa strains by different OAs had a 0.98 pH unit difference [72]. The inhibition of 98% of 344 E. coli O157:H7 strains had a 0.56 pH unit difference between three different OAs [48], the inhibition of 138 non-O157 STEC strains had a 0.99 pH unit difference between four different OAs [49], and inhibition of 95% of 145 Salmonella strains by four different OAs resulted in an observed 1.1 pH unit difference [50]. These data demonstrate that inhibition of C. jejuni or the other Gram-negative bacteria previously studied are primarily not dependent on pH, as others have suggested [40], but bacterial inhibition by OAs must be dependent on some other aspect of the OAs [52,73]. One might expect that the MIC M s for the same bacteria against different OAs would be at the same pH value if pH were the primary cause of inhibition [52], but we did not observe that during experimentation.

Relationships of MIC M Concentrations and pH to the Undissociated OA Concentrations
The inhibition of 100% of all 96 C. jejuni strains by the six undissociated OAs, propionic, l-lactic, formic, citric, butyric, and acetic acid required concentrations of 0.932 mM citric acid to 51.71 mM l-lactic acid, which is a difference in the level of undissociated acid of 50.78 mM across all six OA species for inhibition of the same 96 strains. The MICs of most of the strains are observed at very dilute undissociated OA concentrations that approach 0.5 to 5 µM. No correlation was observed as to the concentration of undissociated OAs required to produce the MIC M s for the 96 C. jejuni strains. These results agree with our earlier studies on other Gram-negative foodborne pathogens. Inhibition of 100% of P. aeruginosa (175 strains) by undissociated citric (2.53 mM) or undissociated acetic acid (21.65 mM) resulted in a difference of ∆ = 19.12 mM OAs [72]. Inhibition of 98.3% of E. coli O157:H7 (344 strains) by undissociated citric (2.86 mM) or undissociated acetic acid (50.63 mM) was a difference of ∆ = 47.77 mM OAs for disinfection of these strains [48]. Inhibition of 100% of non-O157 STEC (138 strains) by undissociated citric (2.2 mM) and undissociated acetic acid (49.11 mM) resulted in a difference of ∆ = 46.91 mM OAs for disinfection of these strains [49]. Inhibition of 100% of Salmonella (145 strains) by undissociated citric (2.29 mM) and undissociated acetic acid (19.0 mM) resulted in a difference of ∆ = 16.71 mM OAs for disinfection of these strains [50], and inhibition of C. coli (111 strains) by undissociated citric (0.024 mM) or undissociated acetic acid (39.93 mM) resulted in a difference of ∆ = 39.91 mM [52]. In all five cases, the undissociated OA concentrations did not correlate with the MIC M s of the different bacteria. The levels of undissociated acids necessary to inhibit non-O157 STECs, E. coli O157:H7, C. coli, and in this study for C. jejuni were the highest, but most likely this increase was caused because of the glutamate and arginine-dependent acid-resistance systems [66] used to protect E. coli strains from extreme acid stress or the maintenance of iron homeostasis to protect against oxidative stress and acid resistance in Campylobacter spp. [74] and specifically C. jejuni [67,68], or bacteria utilization of OAs as an energy source.
The concentrations of undissociated OAs required to inhibit the 96 strains can be viewed from another perspective. Looking at the pH of the system at the points where the 96 strains are inhibited by the undissociated OA clearly shows that close to all 96 strains are inhibited by undissociated citric acid as the undissociated OA concentration approaches zero, and in fact, most of the strains are inhibited by all six organic acids as the undissociated OA concentrations approach zero. These results are not realistic, suggesting that the undissociated OAs play a small part, if any, in inhibiting C. jejuni.

Relationships of MIC M Concentrations and pH to the Dissociated OA Concentrations
The inhibition of 96 C. jejuni strains by dissociated citric acid at 20.39 mM and inhibition of 99% of the strains by propionic and acetic acid at 24.36 and 24.86 mM, respectively, and 97% of the strains by butyric acid at 22.72 mM formed a narrow inhibition band with a ∆ = 4.47 mM. This small concentration range observed for inhibition of most of the strains (97-99%) is very defined, unlike what was observed for the undissociated acids. However, the largeness of the C. jejuni inhibition concentration range against dissociated l-lactic and formic acid is most likely due to the bacterial utilization of these two acids. Formate is metabolized by the multi-subunit formate dehydrogenase (FDH) in C. jejuni [75], which exhibits a chemoattraction to and respiration of formate, compared with other OAs making formic acid a primary energy source [76,77]. Other OAs, like acetic [77,78], butyric [77,78], propionic [78], and l-lactic [78,79] can also be utilized by C. jejuni as energy sources. Campylobacter jejuni utilization of l-lactate proceeds through two NAD-independent l-LDHs-a non-flavin iron-sulfur containing enzyme, and a flavin and iron-sulfur containing enzyme [79]. Therefore, dissociated l-lactic and formic acid may be expected to have a high C. jejuni inhibition concentration, as was seen in our experiments. However, it was determined that C. jejuni strains isolated from humans did not utilize propionic acid [80]. The susceptibility of C. jejuni to OAs has been investigated by several researchers showing inconsistent results [22,31,38,80,81]. Due to C. jejuni utilization of acetic, butyric, and propionic acids, our experimental results show increased concentrations of dissociated OAs widening the band of C. jejuni inhibition, but the high dependence of C. jejuni on formic and l-lactic acid for energy production skews the formic and l-lactic acid curves well beyond those for other OAs. This same dependence on formic acid for energy production was observed in studies with C. coli [52], and major utilization of l-lactic acid was observed in a study of P. aeruginosa strains [72]. However, a relatively small band (∆ = 5.24 mM) of inhibition resulting from 100% of the strains by l-lactic acid and citric acid and 97-99% of the strains by butyric acid, propionic acid, and acetic acid shows a well-correlated group of dissociated OAs that inhibit C. jejuni. Previous studies of P. aeruginosa strains resulted in inhibition of 98% of the 175 strains by dissociated citric acid (10.24 mM) and dissociated acetic acid (9.98 mM), resulting in a difference in dissociated OAs of only ∆ = 0.26 mM [72]. Inhibition of 98.3% of E. coli O157:H7 (344 strains) by dissociated propionic (13.82 mM) and l-lactic acid (19.12 mM) had a difference of ∆ = 5.54 mM [48]. In a study of 138 non-O157 STEC strains, inhibition of 100% of the strains was accomplished by dissociated l-lactic acid (12.93 mM) and citric acid (19.12 mM) having a difference of only ∆ = 6.19 mM [49]. Inhibition of all 145 Salmonella strains by dissociated propionic (13.67 mM) and citric acid (19.03 mM) had a small difference of ∆ = 5.36 mM [50], and inhibition of 111 C. coli strains by dissociated butyric (22.56 mM) and l-lactic acid (21.17 mM) resulted in a very small difference of ∆ = 1.39 mM [52]. However, citric acid was not utilized by C. coli [52,71] and inhibition of 100% of the 111 C. coli strains by dissociated citric acid occurred at 10.64 mM [52]. It should be noted that 95 of 96 C. jejuni strains were inhibited by dissociated citric acid at 10.62 mM in this study.
Alternatively, we can look at the pH vs. the dissociated OA concentrations at the MIC M s. The pH varies widely at the C. jejuni MIC M s against the dissociated OAs, but dissociated citric acid, the only OA not utilized by C. jejuni as an energy source, inhibited 100% of the strains at a concentration of 20.39 mM. This dissociated OA value compares well with dissociated OA values obtained from previous studies of many other pathogens. Inhibition of 100% of Salmonella strains by all dissociated OAs tested required ≤19.03 mM [50]; all VRE strains were inhibited by all dissociated OAs tested at ≤19.53 mM [51]; all P. aeruginosa strains were inhibited by dissociated citric and acetic acid using a level of ≤18.79 mM [72]; all non-O157 STEC strains were inhibited by all dissociated OAs tested at a level of ≤19.12 mM [49]; all C. coli strains were inhibited by dissociated citric acid using a level of ≤10.64 mM [52]; and 98.3% of E. coli O157:H7 strains were inhibited by all OAs tested using a level of ≤19.36 mM [48]. Approximately 20 mM dissociated OA appears to be an optimum level for inhibition of the bacteria tested, unless the OA is utilized by the bacteria. The inhibition of 97-99% of the strains by dissociated propionic, acetic, and butyric acid are also utilized by C. jejuni required levels of ≤24.86 mM [77,78], and have similar OA concentrations at the point of inhibition of the C. jejuni strains (∆ = 2.14 mM). The inhibition of 97-99% of the strains by dissociated l-lactic acid and formic acid are utilized in a major way by C. jejuni required levels of ≤36.36 mM to inhibit the C. jejuni strains. Unlike the undissociated OAs having a broad concentration pattern at the MIC M s of the bacteria, the dissociated OAs have similar concentrations when inhibiting 97-100% of the 96 C. jejuni strains. The work described here is extremely promising, and provides insight into the mechanism of OA inhibition of bacteria, and also correlates well with our previous work on six other pathogenic bacteria. However, the studies described here were conducted in a laboratory setting under controlled conditions and controlled concentrations of bacteria as well as OAs, and further confirmation work in the field must be performed to confirm the results obtained in the laboratory.

Mechanism by Which Organic Acids Control Bacteria Based on Our Studies
The mechanism of OA bacterial inhibition has traditionally been assumed to be mainly dependent on pH [38] or the undissociated form of the OAs [39][40][41][42][43][44]. The activities of OAs change with pH levels, and the type and concentration of OA [47]; and OAs affect bacteria differently depending on whether the bacteria utilize the OA as an energy source [52]. An underlying premise of previous studies is that the OA must be protonated in order to pass through the outer membrane of the bacterial cell. Our present study with C. jejuni clearly shows that dissociated OA levels correlate best with the MIC M s of C. jejuni, suggesting that the earlier premise followed by researchers might be wrong. Even though C. jejuni utilizes many of the OAs studied as energy sources, these dissociated OAs still correlate better with the MIC M s than either pH alone or the undissociated OAs. Almost all 96 C. jejuni strains (97-100%) were inhibited by either dissociated citric, propionic, acetic, or butyric acid in the concentration range of 20.39-24.86 mM. Formic and lactic acid required much higher levels of dissociated OA for inhibition, most likely because these two OAs are well-utilized by C. jejuni as energy sources [76,77,79]. A previous publication states that "intracellular accumulation of anions is a primary contributor to inhibition of bacterial growth" [46], and our previous studies and these C. jejuni data fit well with that statement. Also, our previous work on six other pathogens, E. coli O157:H7 [48], non-O157 STECs [49], P. aeruginosa [72], Salmonella [50], VRE [51], and C. coli [52] correlates well with this current C. jejuni study. The first five bacterial pathogens required a dissociated OA concentration of 12.45-19.76 mM for inhibition of nearly all strains tested, except for lactic acid which is utilized by P. aeruginosa as an energy source [72]. C. coli requires a dissociated OA concentration of from 10.64-22.56 mM for inhibition by the OAs not utilized as an energy source for C. coli [52]. Therefore, we have generated a large data pool that demonstrates bacterial inhibition by OAs is caused by a distinct concentration of the dissociated OA species, and the concentration is similar regardless of what OA is used, except for those OAs that are utilized by the bacteria as energy sources. In accordance with the Henderson-Hasselbalch equation, the pH, pK a , and the concentration of OA acid will specifically produce a concentration of dissociated OA species that inhibits bacteria. For the many pathogenic bacteria that we have studied, the general concentration range of dissociated OA species required to inhibit 97-100% of the bacteria is 20 to 25 mM.

Conclusions
In our study of C. jejuni inhibition by OAs, the inhibition of strains was associated with the concentration of dissociated propionic, citric, butyric, and acetic acid, and these OAs correlated with the MIC M s of 97-100% of the C. jejuni strains tested. Bacterial inhibition was not dependent on pH or on the concentration of the undissociated OAs. Even though C. jejuni cannot utilize the citric acid cycle (CAC) to produce energy, C. jejuni can utilize some of the CAC intermediates and many OAs to produce energy: propionic, l-lactic, formic, butyric, and acetic acid can all be utilized by C. jejuni to produce energy, and l-lactic and formic acid are known to be good energy sources, while C. jejuni exhibits enhanced chemoattraction to formate in comparison to other OAs. This may account for the high concentrations of l-lactic and formic acid required to inhibit C. jejuni in our studies. Based on how well C. jejuni utilizes formate and l-lactate, the use of l-lactic and formic acid would most likely not be appropriate for disinfection or removal of this bacterium. The other OAs utilized by C. jejuni, acetic, butyric, and propionic acid, also would not be expected to be good for removing C. jejuni from carcasses, because these acids would have the tendency to revive the bacteria at reduced levels of dissociated acid. Dissociated citric acid showed good properties in our studies, inhibiting 100% of the C. jejuni strains at a reasonable concentration, and citric acid is not utilized by C. jejuni. A concentration of dissociated citric acid (21 mM) could potentially be used to eliminate C. jejuni surface bacteria from animal carcasses. If the concentration of dissociated citric acid is reduced from the suggested 21 mM, then C. jejuni bacteria may escape disinfection. However, studies must be undertaken to confirm that the suggested concentrations of dissociated organic acids are adequate to remove C. jejuni bacteria in the field vs. the laboratory. If the dissociated OA used in a carcass wash is not controlled at the proper concentration, the wash may not provide the expected level of elimination of surface bacteria. Of the six OAs studied here, citric acid is the most efficient at inhibiting C. jejuni.