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Article

Mechanisms of Antimicrobial Action of Cinnamon and Oregano Oils, Cinnamaldehyde, Carvacrol, 2,5-Dihydroxybenzaldehyde, and 2-Hydroxy-5-Methoxybenzaldehyde against Mycobacterium avium subsp. paratuberculosis (Map)

by
Stella W. Nowotarska
1,
Krzysztof Nowotarski
1,
Irene R. Grant
1,
Christopher T. Elliott
1,
Mendel Friedman
2,* and
Chen Situ
1,*
1
Institute for Global Food Security, School of Biological Sciences, Queen’s University Belfast, David Keir Building, Stranmillis Road, Belfast BT9 5AG, UK
2
Western Regional Research Center, Agricultural Research Service, U.S. Department of Agriculture, Albany, CA 94710, USA
*
Authors to whom correspondence should be addressed.
Foods 2017, 6(9), 72; https://doi.org/10.3390/foods6090072
Submission received: 26 July 2017 / Revised: 8 August 2017 / Accepted: 21 August 2017 / Published: 24 August 2017
(This article belongs to the Special Issue Application of Essential Oils in Food Systems)
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Abstract

:
The antimicrobial modes of action of six naturally occurring compounds, cinnamon oil, cinnamaldehyde, oregano oil, carvacrol, 2,5-dihydroxybenzaldehyde, and 2-hydroxy-5-methoxybenzaldehyde, previously found to inhibit the growth of Mycobacterium avium subsp. paratuberculosis (Map) reported to infect food animals and humans and to be present in milk, cheese, and meat, were investigated. The incubation of Map cultures in the presence of all six compounds caused phosphate ions to leak into the extracellular environment in a time- and concentration-dependent manner. Cinnamon oil and cinnamaldehyde decreased the intracellular adenosine triphosphate (ATP) concentration of Map cells, whereas oregano oil and carvacrol caused an initial decrease of intracellular ATP concentration that was restored gradually after incubation at 37 °C for 2 h. Neither 2,5-dihydroxybenzaldehyde nor 2-hydroxy-5-methoxybenzaldehyde had a significant effect on intracellular ATP concentration. None of the compounds tested were found to cause leakage of ATP to the extracellular environment. Monolayer studies involving a Langmuir trough apparatus revealed that all anti-Map compounds, especially the essential oil compounds, altered the molecular packing characteristics of phospholipid molecules of model membranes, causing fluidization. The results of the physicochemical model microbial membrane studies suggest that the destruction of the pathogenic bacteria might be associated with the disruption of the bacterial cell membrane.

1. Introduction

Many naturally-occurring compounds, such as plant extracts, secondary metabolites, and phytochemicals, have been extensively evaluated for antimicrobial activity [1,2,3,4,5,6,7,8,9]. Many of them have been shown to be active against both Gram-positive and Gram-negative bacteria, including Bacillus cereus [10,11], Listeria monocytogenes [12,13], Pseudomonas aeruginosa, Salmonella typhimurium and Staphylococcus aureus [14,15], Escherichia coli [16,17], and Campylobacter jejuni [18,19,20]. Some natural compounds, e.g., cinnamon oil and oregano oil, have exhibited activity against pathogenic bacteria that have developed resistance to conventional antibiotics [21,22].
Map is a bacterial pathogen of animal health and potential public health significance [23]. As the causative agent of Johne’s disease (paratuberculosis) in domesticated ruminants, such as cattle, sheep, goats, and rabbits [24,25,26,27,28], as well as hens [29], starlings [30], and wildlife [31], it can cause chronic diarrhea, progressive weight loss, decreased milk production, and infertility in these food animals, as well as significant economic losses to farmers [32,33,34,35].
Currently there is no drug approved for the treatment of Johne’s disease. Click [36] reported that infection with the probiotic bacterium Dietzia, alone or in combination with dexamethasone, inhibited the growth of the mycobacterium in cattle. Godden, et al. [37] and Verhegghe, et al. [38] describe the use of heat-treated colostrum for reducing Map in dairy cows. Vaccines in development also have the potential to protect dairy herds against Map [39,40,41,42].
Human epidemiological and medical studies suggest that Map might also contribute to the etiology of human diseases. These include Crohn’s disease of the digestive tract [43,44], type 1 diabetes [45,46,47], and multiple sclerosis [48]. The cited studies suggest the need to further define the possible conflicting role of Map in the cause, mechanism, and prevention of Map-induced adverse effects in humans [49].
Once farm animals are identified as being infected with Map, they are culled prematurely. However, because of the relatively long latent period of Map infections, generally between two and five years, by the time the first clinically-affected animal is identified a significant proportion of the herd could have been infected by the bacterium. Map can be readily transmitted through the fecal-oral route between animals and via contaminated water because it can persist in the farm environment for lengthy periods [50,51,52,53,54]. Transmission of Map to humans may be via contaminated dairy products, meat, or water [55]. Map has been isolated from or detected in dairy products such as cheese, raw and pasteurized milk, and infant milk formula [56,57,58,59]. The bacteria can survive extreme conditions such as low pH, high pasteurization temperatures, or low refrigeration temperatures [60].
In a previous study we investigated the effect of a range of naturally-occurring compounds on Map cells. Six compounds (cinnamon oil, trans-cinnamaldehyde, oregano oil, carvacrol, 2,5-dihydroxybenzaldehyde, and 2-hydroxy-5-methoxybenzaldehyde) inhibited the growth of Map [61]. Following appearance of our study, Crandall et al. [62] reported that citrus oils inhibited the growth of Mycobacterium tuberculosis species in vitro. These authors suggested that the observed anti-mycobacterium properties of the Valencia orange oil warrant further study designed to elucidate the specific mechanisms of action. In a related study, we explored the use of monolayers of bacterial phospholipids as artificial model membranes to study the interaction these compounds with the artificial cell membranes [63].
To further define the antimicrobial mechanisms, in the present study, the potential anti-mycobacterium mechanisms of these compounds have been investigated with Map bacteria. Naturally-occurring compounds, such as potato and tomato glycoalkaloids and plant essential oils and their constituents are generally known to target the cell membrane of microorganisms and animal tissues owing to their hydrophobic nature, which enables them to partition into the hydrophobic part of the phospholipid bilayer and accumulate at the cell membrane [64,65]. However, the molecular interactions between the naturally-occurring compounds and bacterial cells still require further determination [15]. It has been suggested that naturally-occurring antimicrobial compounds might have several modes of action to achieve metabolic inhibition and growth inhibition of microbes, subsequently leading to cell death [66].
Methods for studying antibacterial mechanisms include: measuring the change of cell homeostasis, e.g., using fluorescent probes to measure the change of intracellular pH, the relative change of membrane potential and ATP synthesis [10]; measuring oxygen consumption [16]; proteomic studies to investigate protein expression or repression under stressful, but non-lethal, antimicrobial treatments [67]; observing changes in cell morphology after antimicrobial treatment using transmission [68] and scanning electron microscopy [69]; and measuring cell membrane stability, e.g., whole cell autolysis which could indicate whether the antimicrobials cause the disintegration of cells [70]. In the present study, we determined extracellular phosphate ion concentration, intracellular and extracellular ATP concentrations, and monitored changes in absorbance of supernatants from broth cultures exposed to the six active naturally-occurring compounds. In addition, monolayer model membrane studies using a Langmuir trough apparatus were performed. Monolayer model membrane studies are a biophysical approach to study the interaction of antimicrobials with lipid monolayers that mimic the outer surface of biological membranes. These techniques have recently been employed for mode of action studies [71,72,73].
Biological membranes have an extremely complex chemical composition including different types of phospholipids [74] which serve as a matrix for other essential components, e.g., proteins, including enzymes and biopolymers for cellular function [75,76,77,78]. Due to the complexity of biological membranes, different varieties of model membrane systems, e.g., liposome, planar lipid bilayer, and monolayer have been studied [79]. In this study, a monolayer model membrane was used as a single component system to analyze the influence of antimicrobial substances on lipid behavior in the membrane. We believe this to be the first reported study to determine the cellular response of Map to six naturally-occurring compounds previously demonstrated to inhibit growth of this bacterium. Possible modes of action of the plant antimicrobials against Map are discussed.

2. Materials and Methods

2.1. Plant Materials

The naturally-occurring compounds 2,5-dihydroxybenzaldehyde, 2-hydroxy-5-methoxybenzaldehyde, carvacrol, and trans-cinnamaldehyde were obtained from Sigma-Aldrich (Poole, Dorset, UK); the purity levels of these compounds ranged from 98 to 99% according to the manufacturer’s specifications. Cinnamon oil (purity > 95%), containing 85% trans-cinnamaldehyde, was obtained from Yerba Buena Co. (Berkeley, CA, USA). Oregano oil (purity > 95%), containing 85% carvacrol, was obtained from Lhasa Karnak Herb Co. (Berkeley, CA, USA). The purity levels of 2,4,6-trihydroxybenzaldehyde, geraniol, and vanillic acid (Sigma-Aldrich, Dorset, UK); ranged from 97% to 98% according to the manufacturer’s data. Stock solutions, 50 mg/mL for solid compounds and 50 µL/mL for oil compounds, were prepared by suspension in absolute ethanol. As a high percentage of ethanol is bactericidal, the maximum concentration of ethanol that a strain could tolerate (showing no observable inhibition of growth) was determined in a previous study of the bactericidal assay [61]. The final concentration of ethanol present in all studies using Map culture was standardized at 0.4% (v/v).

2.2. Bacterial Strains and Growth Conditions

Mycobacterium avium subsp. paratuberculosis NCTC 8578 (a bovine isolate) was originally obtained from the National Collection of Type Cultures, Colindale, London. The strain was maintained in Cryobank vials (Mast Group Ltd., Merseyside, UK) at −70 °C. When a broth culture was required, two cryobeads were inoculated into 10 mL of Middlebrook 7H9 broth (Difco Laboratories, Detroit, MI, USA), supplemented with 0.05% (w/v) Tween 80 (Sigma-Aldrich, Dorset, UK), 10% (v/v) oleic albumin dextrose catalase (OADC) supplement (Difco), and 2 µg/mL of mycobactine J (Synbiotics Europe SAS, Lyon, France), pH 6.6 ± 0.2, and incubated at 37 °C with shaking at 100 rpm for 28 to 35 days until the optical density at 600 nm (OD600) was between 0.7 and 1.0. Fifty milliliters of early stationary phase Map culture (OD600 = 0.7–1.0, ~5 × 107 cfu/mL) was centrifuged at 2500× g for 30 min to pellet the cells. Cell pellets were washed three times in 50 mL of sterile reverse osmosis water (Milli Q water system; Millipore, Molsheim, France) at room temperature. Map cells were resuspended differently depending on the analysis to be performed, as indicated below.

2.3. Determination of Extracellular Phosphate Concentration

The phosphate assay was carried out as described by Lambert, et al. [15] with minor modifications. Briefly, the washed Map cell pellets were resuspended to the original volume in sterile HPLC water (Sigma-Aldrich, Dorset, UK). Aliquots (2 mL) of the cell suspension were transferred into sterile Eppendorf tubes to which the test compounds were added. Four of the anti-Map compounds (cinnamaldehyde, carvacrol, 2,5-dihydroxybenzaldehyde, and 2-hydroxy-5-methoxynenzaldehyde) and a non-active compound vanillic acid, were tested at three-fold dilutions ranging from eight to 1000 µg/mL. Ethanol (0.4%, v/v) was used as negative control. The samples were incubated at 37 °C for 24 h with aliquots taken at 0, 1, 2, 4, 8, and 24 h time points. Aliquots were transferred into Eppendorf tubes and centrifuged at 16,873× g for 15 min. Supernatants were carefully transferred into fresh Eppendorf tubes. All samples were stored at −20 °C until used. For the phosphate test, aliquots of each sample (50 µL) were pipetted into a flat-bottom 96-well microtitre plate (Sarstedt Ltd., Leicester, UK) and Biomol Green™ phosphate assay reagent (100 µL) (Enzo Life Sciences UK Ltd., Exeter, UK) was dispensed into each well. The plate was sealed and incubated at room temperature for 20 min to allow for color development. The OD620 was then measured using a microplate reader (Tecan UK Ltd., Reading, UK). Phosphate standard solution (Enzo Life Sciences UK Ltd., Exeter, UK) was prepared to establish a calibration curve range from 0 to 40 µM to allow the phosphate concentration to be determined. The experiment was repeated twice on different dates.

2.4. Determination of Intra- and Extra-Cellular ATP Concentration

The intracellular and extracellular concentrations of ATP were investigated using the procedures described by Gill and Holley [12] with minor modifications. Briefly, the washed Map pellet was resuspended in 7H9 broth base (45 mL) without OADC or mycobactine J and incubated at 37 °C to starve (deplete the intracellular ATP) for six weeks. Aliquots of the cell suspension (3.6 mL) were transferred into small bottles, and supplemented with 0.5% d-glucose. Duplicate bottles were supplemented with natural compound stock (17.76 µL) to achieve the previously-determined minimum inhibitory concentration (MIC) of each compound (MIC: cinnamaldehyde, 24 mg/L; cinnamon oil, 24 mg/L, carvacrol, 74 mg/L, oregano oil, 74 mg/L; 2,5-dihydroxybenzaldehyde, 74 mg/L; and 2-hydroxy-5-methoxybenzaldehyde, 74 mg/L). Two other bottles were supplemented with the non-active compound 2,4,6-trihydroxybenzaldehyde (17.76 µL) stock to achieve a final concentration of 74 mg/L. Another two bottles were supplemented with absolute ethanol (17.76 µL) to a final concentration 0.4% v/v to serve as negative controls. At 0, 1, 2, 4, 8, and 24 h, samples were taken and subjected to the following procedure. A sample (500 µL) from each bottle was transferred to an Eppendorf tube; the cells were pelleted by centrifugation at 2500× g for 15 min, and the supernatant (250 µL) was carefully transferred to an Eppendorf tube containing 200 mM Tris (250 µL) + 4 mM EDTA + 0.05% dodecyl trimethyl ammonium bromide (DTAB) for stabilization and determination of extracellular ATP concentration. The remaining half of the supernatant was carefully discarded. The cell pellet was then resuspended in an ‘extractant’ (500 µL; 100 mM Tris + 2 mM EDTA + 0.025% DTAB). To facilitate ATP extraction, the cell suspensions mixtures were heated in a boiling bath for 20 min. After heat treatment, samples were placed in an ice bath to facilitate rapid cooling. Triplicate aliquots (50 µL) of each sample were pipetted into a white 96-well plate (Greiner Bio-One Ltd., Gloucestershire, UK). ATP standard (Sigma-Aldrich, Dorset, UK) at a concentration of 1, 2, 4, 8, 16, 32, and 64 nM prepared in the extractant was used to generate a calibration curve. The ATP assay mix reagent (50 μL) (Sigma-Aldrich, Dorset, UK) was dispensed into each sample and standard well. The bioluminescence was then read immediately using a microplate reader (Mithras LB 940, Berthold Technologies UK Ltd., Herts, UK). This experiment was repeated twice.

2.5. Absorbance Scans of Culture Supernatant after Antimicrobial Treatment

The washed Map cell pellets were resuspended in the original volume of sterile reverse osmosis water. Aliquots (4 mL) were transferred to small sterile bottles and supplemented with test compounds. Three of the anti-Map compounds (carvacrol, 2,5-dihydroxybenzaldehyde and 2-hydroxy-5-methoxynenzaldehyde) and the non-active vanillic acid were tested at 74 µg/mL, and cinnamaldehyde was tested at 24 mg/L. Since all of the natural compounds were suspended in absolute ethanol as a stock solution prior to addition to the Map cultures, ethanol (0.4% (v/v) was used as a negative control. The bottles were incubated at 37 °C for 48 h. At 0, 1, 2, 4, 8, 24, and 48 h, sample aliquots were pipetted into Eppendorf tubes and centrifuged at 16,873× g for 15 min. Supernatants were carefully transferred into fresh Eppendorf tubes. For the scan experiment, samples (200 µL) were pipetted into separate wells of a flat-bottom 96-well UV plate (Costar, Corning Ltd., Sunderland, UK). The samples were scanned from 230 nm to 370 nm with a wavelength step size of 5 nm, using a microplate reader (Tecan UK Ltd., Reading, UK). Since most of the natural compounds absorb UV light and might show more than one peak when scanned for a series of wavelengths, a corresponding blank (composed of water and natural compound only, without culture) was prepared for each natural compound and processed under the same conditions as the Map-containing sample to allow a comparison of supernatant samples. This experiment was repeated twice.

2.6. Monolayer Studies

A Langmuir trough (Precision Plus) (µTrough XL; Kibron, Helsinki, Finland) equipped with a computer-controlled microbalance (Kibron) and MicroSpot (Kibron) was used to measure surface pressure-area (π-A), using the control software (FilmWare 3.61; Kibron). The total surface area of the trough was 227.15 cm2, and the volume of the subphase was approximately 0.1 L. Phospholipids 1,2-di-(9Z-octadecenoyl)-sn-glycero-3-phosphoethanolamine (DOPE) and 1,2-di-(9Z-octadecenoyl)-sn-glycero-3-phospho-(1′-rac-glycerol) sodium salt (DOPG) were purchased from Avanti Polar Lipids (Alabaster, Alabama, USA). Stock solutions of the phospholipids (5 mg/mL) were prepared in chloroform (Sigma-Aldrich, Dorset, UK) and stored at −20 °C. The naturally-occurring antimicrobial compounds were prepared as stock solutions in reverse osmosis water for powder compounds (100 mg/mL) and chloroform for oil compounds (500 mg/mL). Reverse osmosis water was freshly obtained and used in all experiments. The stocks of powder compounds were freshly prepared before each experiment and used on the same day. The stocks of oil compounds were stored at −20 °C until required. The compounds were tested at concentrations closed to the MIC determined in previous antibacterial assays [61] was 74 mg/L for powder compounds. For the essential oil compounds, the above stock solution (1 µL) was deposited onto the surface of the subphase. The concentration could not be determined as the oil compounds were surface active and no shaking or stirring was employed to facilitate mixing. The phospholipids prepared in chloroform were deposited onto the water surface (pure water with or without natural compounds in the subphase) interface using a 5-µL Hamilton micro-syringe (Supelco, Bellefonte, PA, USA). The selection of subphases was based on the results of the previous antimicrobial assays by Wong, et al. [61]. After spreading the phospholipids, the monolayer was allowed to equilibrate for 10 min (to ensure evaporation of the solvent). Film compression was initiated by moving the two barriers symmetrically, with a speed of 21.157 Å2/chain/min to allow for the reorientation and relaxation of the lipids during compression. Surface pressure (π) was measured with an accuracy of ±0.1 mN/m using a metal wire probe (Kibron) linked to a high precision microbalance connected to a computer. All isotherms were recorded at 23 °C. The subphase temperature was controlled thermostatically to within 0.1 °C by a circulating water system (Grant Instruments (Cambridge) Ltd., Cambridgeshire, UK).

2.7. Analysis of Isotherms

The interaction between lipid molecules deposited on subphase containing different antimicrobials and their molecular organization were analyzed by calculating the compression modulus CS−1, which is a reciprocal of isothermal compressibility (CS) as previously described [80]. The CS value of the investigated films at the given surface pressure (π) was obtained from π-A data as follows: CS = (−1/Aπ) (dA/dπ)T, where Aπ is the area per molecule at the indicated surface pressure π. The CS values were calculated using Origin® 8 program (OriginLab Corporation, Northampton, MA, USA). Accordingly, the higher the value of the compressibility modulus CS−1; the lower the interfacial fluidity will be [81].

2.8. Data Analysis

Graphs were plotted using the mean of the replicates of each experiment. Ordinary ANOVA was performed on data, when appropriate, by using GraphPad InStat (GraphPad Software, Inc., La Jolla, CA, USA).

3. Results

3.1. Extracellular Phosphate Assay

The effect of cinnamaldehyde on phosphate leakage of Map cells is shown in Figure 1. The results showed an increase in extracellular phosphate level in the presence of cinnamaldehyde that was concentration- and time- dependent, suggesting increased membrane permeability. Figure 2 shows the effects of four anti-Map compounds and two negative controls, non-active compound vanillic acid and ethanol, on phosphate leakage of the Map culture. Similar to cinnamaldehyde, the results indicated that membrane permeability increased in the presence of all naturally-occurring compounds, including the non-active compound, and the observed increase was time-dependent.

3.2. Intracellular and Extracellular ATP Assays

Cinnamon oil and its active ingredient cinnamaldehyde significantly decreased intracellular ATP (p < 0.05). Oregano oil and its active constituent carvacrol resulted in an initial rapid decrease of intracellular ATP concentration, before it rose again (data not shown). The final intracellular ATP concentrations of Map cells exposed to these two compounds were still low (p < 0.05) compared to the two negative controls. No significant change in intracellular ATP was observed with the other tested compounds.
Low levels of ATP were found in the extracellular environment in all the samples tested including anti-Map compounds and negative controls (data not shown). The extracellular ATP concentration was very low (0.5 nM) and remained unchanged throughout the incubation period.

3.3. Absorbance Scans of Culture Supernatant after Antimicrobial Treatment

The absorbance scan (from 230 to 370 nm) of cinnamaldehyde (24 µg/mL) in sterile reverse osmosis water incubated at 37 °C is shown in Figure 3a. A peak was observed and the highest absorbance was measured at 290 nm (A290). The A290 reading represents the abundance of cinnamaldehyde in the sample, which decreased from about 2.75 to 2.25 during the two-day incubation period. When a similar scan was performed on the supernatant of the culture incubated with 24 mg/L cinnamaldehyde (the MIC that inhibits the growth of Map in broth medium), the A290 reading also decreased over the two-day incubation period (Figure 3b). A new peak, which had the highest absorbance at about 250 nm, appeared after one day of incubation.
An absorbance scan (230 to 370 nm) of carvacrol (74 mg/L) in sterile reverse osmosis water or the supernatant of Map cultures incubated at 37 °C is illustrated in Figure 4a,b. Maximum absorbance was observed at about 270 nm (A270) (Figure 4a). When a similar scan was performed on the supernatant of the Map culture incubated with 74 mg/L carvacrol (the MIC that inhibits the growth of Map in broth medium) (Figure 4b), the A270 reading decreased as the time of incubation increased.

3.4. Monolayer Studies

The compression isotherms and compression modulus for the DOPE monolayer deposited on subphases containing natural antimicrobial compounds are shown in Figure 5a,b. In subphase containing pure water only, the lift-off value was approximately 105 Å2 per molecule and increased gradually into the liquid-condensed (LC) phase up to around 62 Å2 per molecule, at which point the monolayer collapsed (collapse pressure was about 38 mN/m) (Figure 5a). Analysis of the compression modulus for the DOPE monolayer in the presence of different naturally occurring antimicrobial compounds is shown in Figure 5b.
The compression isotherms and compression modulus for the DOPG monolayer deposited on subphases containing selected naturally-occurring antimicrobial compounds are shown in Figure 6a,b. In the subphase containing pure water only, the lift-off value was approximately 120 Å2 per molecule and increased gradually into the liquid-condensed (LC) phase up to around 68 Å2 per molecule, at which point the monolayer collapsed (collapse pressure was about 42 mN/m) (Figure 6a).
Analysis of the compression modulus for the DOPG monolayer in the presence of different antimicrobial compounds is shown in Figure 6b.

4. Discussion

Mechanisms of Antimicrobial Effects against Map

The measurement of intracellular constituents in the extracellular environment, e.g., soluble proteins [69], nucleic acids [82], ATP [83], and phosphate and potassium ions [15] are good indicators of membrane leakage and can reflect the severity of membrane damage. These cellular constituents are important for cellular functions. Presumably, leakage of these constituents might cause further disturbances in cellular metabolism and viability.
As shown in Figure 1 and Figure 2, the degrees of phosphate leakage varied between different compounds in the present study. Cinnamaldehyde caused the highest level of phosphate leakage (Figure 2) in a dose- and time-dependent manner (Figure 1). By contrast, 2,5-dihydroxybenzaldehyde induced the lowest level of leakage. Lambert, et al. [15] reported that oregano essential oil caused leakage of phosphate ion in both the Gram-positive bacterium S. aureus and the Gram-negative bacterium P. aeruginosa. However, because supplementary controls were not included, it is unclear whether the leakage observed from the two organisms was caused only by the oregano essential oil.
The effects of six anti-Map compounds at their MIC values on the intracellular and extracellular ATP concentration of Map cells that had been starved for six weeks were also investigated. Significant effects (p < 0.05) of cinnamon oil and cinnamaldehyde were observed. The transient effect (an initial rapid decrease) of oregano oil and its active ingredient carvacrol (data not shown), suggests that oregano oil and carvacrol might exert their antimicrobial effect by means of initially stressing Map. The data show that Map was able to partially overcome such a challenge and to decrease the effect to some degree. Thus ATP synthesis might have resumed or ATP hydrolysis might have slowed down as a result of a self-defense mechanism. In the present study, we found that carvacrol did not deplete the intracellular ATP pool of Map. This finding contrasts with observation that carvacrol rapidly depleted the ATP pool in the Gram-positive foodborne pathogen Bacillus cereus [10].
A possible explanation for the different effects might be due to the differences in the cell membrane compositions. The Map membrane is characterized by a thicker, waxy, and hydrophobic cell wall, which is very rich in mycolic acid, making it more resistant to chemical damage and environmental stress. Low levels of extracellular ATP found in our study may be due to a weak ATP efflux as a result of Map being stressed when exposed to the antimicrobial compounds. This also implies that the compounds did not increase the membrane permeability for ATP.
The absorbance scan of cinnamaldehyde (24 μg/mL) in water or Map culture showed a decrease of the peak at 290 nm over the two-day incubation period (Figure 3a,b). When comparing the culture supernatant at time 0 min with the corresponding blank, the A290 reading is approximately 0.5 absorbance units lower in the supernatant. The explanation for this finding might be due to the adsorption of cinnamaldehyde to the cell surface or uptake of cinnamaldehyde into the cells. Furthermore, a new peak, which had the highest absorbance at about 250 nm, appeared after one day. The new peak could either be a product transformed by Map by cinnamaldehyde during the incubation, or an intracellular constituent that had leaked from the cells. Since the peak showed the highest absorbance within the UV region (250 nm), it is possibly an indication of nucleic acid or leakage of other constituents from the cells. The appearance of such a new peak was unique to cinnamaldehyde; culture supernatants from cells exposed to all of the other compounds did not show additional peaks. Attempts were made to identify this peak, using QToF LC/MS and NMR spectroscopy, but without success.
An absorbance scan (230 to 370 nm) of carvacrol in sterile reverse osmosis water (Figure 4a) or supernatant cultures (Figure 4b) shows that the highest absorbance was observed at 270 nm (A270). The A270 value decreased from about 0.58 to 0.53 during the two-day incubation period (Figure 4a), similar to the absorbance scan of cinnamaldehyde in water. However, the decrease in A270 was much smaller than that with cinnamaldehyde. When a similar scan was performed on the supernatant of the Map culture incubated with carvacrol (74 mg/L; the MIC that inhibits the growth in broth medium) (Figure 4b), the A270 reading decreased as the time of incubation increased, i.e., from about 0.55 to 0.44. The decreased quantity of carvacrol suggested the uptake of carvacrol by the Map organism. However, in contrast to the cinnamaldehyde experiment, the decrease in absorbance reading in culture supernatant treated with carvacrol was much smaller and no additional peaks were observed.
Lipid monolayers were formed at the air-liquid interface to mimic the outer surface of the bacterial membrane by using DOPE and DOPG. PE and PG phospholipids were selected for this study because they are the predominant zwitterionic and anionic phospholipids found in the membranes of both Gram-positive and Gram-negative bacteria [75,78]. The changes in compressibility modulus in both the DOPE and DOPG monolayers reflect the physical state of the lipid monolayer compressed on the surface of different subphases. The factor that determines compressibility of the isotherm is its slope. This can be calculated as a derivative of area per molecule versus surface pressure, which reflects the rate of change of the area per molecule against surface pressure. The higher the value of the compressibility modulus, the higher the rigidity of the model membrane and, vice versa, a low value of compressibility modulus indicates high fluidity of the model membrane [84].
Isotherms of DOPE deposited on the subphase with naturally-occurring antimicrobial compounds showed the lift-off value increased and varied from approximately 110 to 200 Å2 per molecule (Figure 5a). The increase in the lift-off value indicated these antimicrobial compounds could have been incorporated into the lipid monolayers in the gas state resulting in the observed reduced packing effectiveness of DOPE molecules. In the presence of three oil compounds, cinnamaldehyde, carvacrol, and geraniol, the slopes of the isotherms were the flattest. For the DOPE monolayer compressed on the subphase containing pure water only, the maximal value of CS−1 was observed at approximately 122 mN/m, whereas the value for 2,4,6-trihydroxybenzaldehyde was approximately 138 mN/m, suggesting a rigidifying effect of this compound on the DOPE monolayer (Figure 5b). For the other compounds, the maximal values of the compression modulus varied from 50 to 110 mN/m. Such a decrease in the maximal value of the compression modulus indicated a fluidizing effect possibly in the DOPE monolayer. Carvacrol showed the highest fluidizing effect, whereas 2,5-dihydroxybenzaldehyde exhibited the lowest effect.
Isotherms of DOPG deposited on the subphase with natural antimicrobial compounds showed the lift-off value varied from approximately 117 to 195 Å2 per molecule (Figure 6a). In the presence of two of the oil compounds, carvacrol and geraniol, the slopes of the isotherms were the flattest. 2,4,6-Trihydroxybenzaldehyde and 2,5-dihydroxybenzaldehyde caused a non-significant decrease in the lift-off value (p > 0.05). For the DOPG monolayer compressed on a subphase containing pure water only, the maximal value of CS−1 was observed at approximately 118 mN/m, whereas the value for 2,4,6-trihydroxybenzaldehyde was approximately 137 mN/m, indicating a rigidifying effect (Figure 6b). For the other compounds, the maximal values of the compression modulus varied from 42 to 117 mN/m. Geraniol showed the highest fluidizing effect, whereas 2,5-dihydroxybenzaldehyde showed the lowest effect.
It has been reported that antimicrobial compounds interact more easily with the gas or liquid phase of the monolayer than with the liquid-condensed phase [85]. The shape and size of lipid rafts/aggregates seem to be determined by competition between the line tension at the raft boundary and the electrostatic repulsion between molecular polar heads [86]. The present biophysical experiment indicated that antimicrobial compounds interacted differently with the lipid rafts in both lipids, depending on the electrical charge at the polar head as indicated by the higher lift-off values. The difference might be due to the electrostatic interaction between charged head groups and antimicrobials inserted between hydrophobic tails.
In the present study, only 2,4,6-trihydroxybenzaldehyde caused a slight rigidifying effect on both DOPE and DOPG. All other compounds exhibited either a small or large fluidizing effect. The essential oil compounds carvacrol and geraniol showed a greater fluidizing effect in all the monolayers tested than did the solid compound 2,5-dihydroxybenzaldehyde. Sikkema, et al. [87] suggested that the toxicity of a compound is highly related to its ability to disturb the hydrophobic interactions between the lipids and proteins in the cell membrane. The toxicity is, thus, highly related to the decline in membrane integrity. The present results on the relationship between antimicrobial and membrane effects are consistent with this suggestion.
It has been suggested that hydrophobic oil compounds interact with the bacterial cell membrane, changing the membrane structure, stability, and permeability of certain intracellular constituents. Results of this study clearly indicated that natural antimicrobial compounds could modify the lipid monolayer structure, leading to the leakage of phosphate and other essential cell components and a change in the membrane potential and the cell environments, ultimately causing the death of cells. A related study showed that exposure of Bacillus subtilis ATCC 6633 cells to Trachyspermum ammi essential oil caused an instant loss of cytoplasm membrane integrity causing it to become increasingly permeable to protons and ions that might be responsible for the antibacterial activity [88]. Studies with green tea catechins have showed that hydrogen bonding of phenolic hydroxyl groups of catechins to cell membranes might be correlated with antimicrobial and anti-cancer-cell effects of catechins [89,90,91].

5. Conclusions

To conclude, the cellular responses of the potentially zoonotic pathogen Map in the presence of naturally-occurring compounds were studied. The natural compounds tested caused the leakage of phosphate ions from Map cells in relation to the time of exposure to and concentration of the test compounds; however, the extent of phosphate leakage was not consistent with the relative antimicrobial activities of the compounds. Exposure of Map cells to cinnamon oil or its constituent cinnamaldehyde caused a decline in intracellular ATP concentration; however, none of the naturally-occurring compounds caused a leakage of ATP to the extracellular environment. Exposure to cinnamaldehyde may have resulted in a leakage of intracellular constituents, possibly protein or nucleic acids, or the transformation to a new product by Map. The monolayer model membrane studies showed that natural antimicrobial compounds could modify the lipid monolayer structure by incorporation into the monolayer, formation of aggregates/rafts of antimicrobials and lipids, and reduction in the packing effectiveness of the lipid molecules, resulting in an increase in membrane fluidity. The monolayer studies, therefore, confirmed that the antimicrobial compounds, especially oil compounds, are targeting the cell membrane. The described studies offer insights into the interaction between antimicrobials and membrane lipids and identifying characteristics or actions of the most potent compounds.

Acknowledgments

This work was supported by a Research Studentship from Queen’s University Belfast, UK. We thank Carol Levin for facilitating preparation of the manuscript.

Author Contributions

C.S., I.R.G., C.T.E., and M.F. conceived and designed the experiments; S.W.N. and K.N. performed the experiments; and all authors participated in drafting and revising the manuscript.

Conflicts of Interest

The authors declare no conflict of interest.

References

  1. Friedman, M.; Henika, P.R.; Levin, C.E. Bactericidal activities of health-promoting, food-derived powders against the foodborne pathogens Escherichia coli, Listeria monocytogenes, Salmonella enterica, and Staphylococcus aureus. J. Food Sci. 2013, 78, M270–M275. [Google Scholar] [CrossRef] [PubMed]
  2. Friedman, M.; Henika, P.R.; Mandrell, R.E. Bactericidal activities of plant essential oils and some of their isolated constituents against Campylobacter jejuni, Escherichia coli, Listeria monocytogenes, and Salmonella enterica. J. Food Prot. 2002, 65, 1545–1560. [Google Scholar] [CrossRef] [PubMed]
  3. Friedman, M. Antimicrobial activities of plant essential oils and their components against antibiotic-susceptible and antibiotic-resistant foodborne pathogens. In Essential Oils and Nanotechnology for Treatment of Microbial Diseases; Rai, M., Zachino, S., Derita, M.D., Eds.; CRC Press: Boca Raton, FL, USA, 2017; pp. 14–38. [Google Scholar]
  4. Friedman, M. Antibiotic-resistant bacteria: Prevalence in food and inactivation by food-compatible compounds and plant extracts. J. Agric. Food Chem. 2015, 63, 3805–3822. [Google Scholar] [CrossRef] [PubMed]
  5. Friedman, M. Chemistry and multi-beneficial bioactivities of carvacrol (4-isopropyl-2-methylphenol), a component of essential oils produced by aromatic plants and spices. J. Agric. Food Chem. 2014, 62, 7652–7670. [Google Scholar] [CrossRef] [PubMed]
  6. Todd, J.; Friedman, M.; Patel, J.; Jaroni, D.; Ravishankar, S. The antimicrobial effects of cinnamon leaf oil against multi-drug resistant Salmonella Newport on organic leafy greens. Int. J. Food Microbiol. 2013, 166, 193–199. [Google Scholar] [CrossRef] [PubMed]
  7. Moore-Neibel, K.; Gerber, C.; Patel, J.; Friedman, M.; Jaroni, D.; Ravishankar, S. Antimicrobial activity of oregano oil against antibiotic-resistant Salmonella enterica on organic leafy greens at varying exposure times and storage temperatures. Food Microbiol. 2013, 34, 123–129. [Google Scholar] [CrossRef] [PubMed]
  8. Juneja, V.K.; Gonzales-Barron, U.; Butler, F.; Yadav, A.S.; Friedman, M. Predictive thermal inactivation model for the combined effect of temperature, cinnamaldehyde and carvacrol on starvation-stressed multiple Salmonella serotypes in ground chicken. Int. J. Food Microbiol. 2013, 165, 184–199. [Google Scholar] [CrossRef] [PubMed]
  9. Juneja, V.K.; Yadav, A.S.; Hwang, C.-A.; Sheen, S.; Mukhopadhyay, S.; Friedman, M. Kinetics of thermal destruction of Salmonella in ground chicken containing trans-cinnamaldehyde and carvacrol. J. Food Prot. 2012, 75, 289–296. [Google Scholar] [CrossRef] [PubMed]
  10. Ultee, A.; Kets, E.P.; Smid, E.J. Mechanisms of action of carvacrol on the food-borne pathogen Bacillus cereus. Appl. Environ. Microbiol. 1999, 65, 4606–4610. [Google Scholar] [PubMed]
  11. Friedman, M.; Henika, P.R.; Levin, C.E.; Mandrell, R.E.; Kozukue, N. Antimicrobial activities of tea catechins and theaflavins and tea extracts against Bacillus cereus. J. Food Prot. 2006, 69, 354–361. [Google Scholar] [CrossRef] [PubMed]
  12. Gill, A.O.; Holley, R.A. Mechanisms of bactericidal action of cinnamaldehyde against Listeria monocytogenes and of eugenol against L. monocytogenes and Lactobacillus sakei. Appl. Environ. Microbiol. 2004, 70, 5750–5755. [Google Scholar] [CrossRef] [PubMed]
  13. Ravishankar, S.; Jaroni, D.; Zhu, L.; Olsen, C.W.; McHugh, T.H.; Friedman, M. Inactivation of Listeria monocytogenes on ham and bologna using pectin-based apple, carrot, and hibiscus edible films containing carvacrol and cinnamaldehyde. J. Food Sci. 2012, 77, M377–M382. [Google Scholar] [CrossRef] [PubMed]
  14. Je, J.-Y.; Kim, S.-K. Chitosan derivatives killed bacteria by disrupting the outer and inner membrane. J. Agric. Food Chem. 2006, 54, 6629–6633. [Google Scholar] [CrossRef] [PubMed]
  15. Lambert, R.J.W.; Skandamis, P.N.; Coote, P.J.; Nychas, G.-J.E. A study of the minimum inhibitory concentration and mode of action of oregano essential oil, thymol and carvacrol. J. Appl. Microbiol. 2001, 91, 453–462. [Google Scholar] [CrossRef] [PubMed]
  16. Fitzgerald, D.J.; Stratford, M.; Gasson, M.J.; Ueckert, J.; Bos, A.; Narbad, A. Mode of antimicrobial of vanillin against Escherichia coli, Lactobacillus plantarum and Listeria innocua. J. Appl. Microbiol. 2004, 97, 104–113. [Google Scholar] [CrossRef] [PubMed]
  17. Friedman, M.; Zhu, L.; Feinstein, Y.; Ravishankar, S. Carvacrol facilitates heat-induced inactivation of Escherichia coli O157:H7 and inhibits formation of heterocyclic amines in grilled ground beef patties. J. Agric. Food Chem. 2009, 57, 1848–1853. [Google Scholar] [CrossRef] [PubMed]
  18. Friedman, M.; Henika, P.R.; Mandrell, R.E. Antibacterial activities of phenolic benzaldehydes and benzoic acids against Campylobacter jejuni, Escherichia coli, Listeria monocytogenes, and Salmonella enterica. J. Food Prot. 2003, 66, 1811–1821. [Google Scholar] [CrossRef] [PubMed]
  19. Ravishankar, S.; Zhu, L.; Law, B.; Joens, L.; Friedman, M. Plant-derived compounds inactivate antibiotic-resistant Campylobacter jejuni strains. J. Food Prot. 2008, 71, 1145–1149. [Google Scholar] [CrossRef] [PubMed]
  20. Mild, R.M.; Joens, L.A.; Friedman, M.; Olsen, C.W.; McHugh, T.H.; Law, B.; Ravishankar, S. Antimicrobial edible apple films inactivate antibiotic resistant and susceptible Campylobacter jejuni strains on chicken breast. J. Food Sci. 2011, 76, M163–M168. [Google Scholar] [CrossRef] [PubMed]
  21. Friedman, M.; Buick, R.; Elliott, C.T. Antibacterial activities of naturally occurring compounds against antibiotic-resistant Bacillus cereus vegetative cells and spores, Escherichia coli, and Staphylococcus aureus. J. Food Prot. 2004, 67, 1774–1778. [Google Scholar] [CrossRef] [PubMed]
  22. Ravishankar, S.; Zhu, L.; Olsen, C.W.; McHugh, T.H.; Friedman, M. Edible apple film wraps containing plant antimicrobials inactivate foodborne pathogens on meat and poultry products. J. Food Sci. 2009, 74, M440–M445. [Google Scholar] [CrossRef] [PubMed]
  23. Naser, S.A.; Ghobrial, G.; Romero, C.; Valentine, J.F. Culture of Mycobacterium avium subspecies paratuberculosis from the blood of patients with Crohn’s disease. Lancet 2004, 364, 1039–1044. [Google Scholar] [CrossRef]
  24. Lombard, J.E.; Gardner, I.A.; Jafarzadeh, S.R.; Fossler, C.P.; Harris, B.; Capsel, R.T.; Wagner, B.A.; Johnson, W.O. Herd-level prevalence of Mycobacterium avium subsp. paratuberculosis infection in United States dairy herds in 2007. Prev. Vet. Med. 2013, 108, 234–238. [Google Scholar] [CrossRef] [PubMed]
  25. Sweeney, R.W.; Collins, M.T.; Koets, A.P.; McGuirk, S.M.; Roussel, A.J. Paratuberculosis (Johne’s disease) in cattle and other susceptible species. J. Vet. Intern. Med. 2012, 26, 1239–1250. [Google Scholar] [CrossRef] [PubMed]
  26. Pithua, P.; Kollias, N.S. Estimated prevalence of caprine paratuberculosis in boer goat herds in Missouri, USA. Vet. Med. Int. 2012, 2012. [Google Scholar] [CrossRef] [PubMed]
  27. Windsor, P.A. Paratuberculosis in sheep and goats. Vet. Microbiol. 2015, 181, 161–169. [Google Scholar] [CrossRef] [PubMed]
  28. Arrazuria, R.; Juste, R.A.; Elguezabal, N. Mycobacterial infections in rabbits: From the wild to the laboratory. Transbound. Emerg. Dis. 2017, 64, 1045–1058. [Google Scholar] [CrossRef] [PubMed]
  29. Shitaye, J.E.; Matlova, L.; Horvathova, A.; Moravkova, M.; Dvorska-Bartosova, L.; Treml, F.; Lamka, J.; Pavlik, I. Mycobacterium avium subsp. avium distribution studied in a naturally infected hen flock and in the environment by culture, serotyping and IS901 RFLP methods. Vet. Microbiol. 2008, 127, 155–164. [Google Scholar] [CrossRef]
  30. Gaukler, S.M.; Linz, G.M.; Sherwood, J.S.; Dyer, N.W.; Bleier, W.J.; Wannemuehler, Y.M.; Nolan, L.K.; Logue, C.M. Escherichia coli, Salmonella, and Mycobacterium avium subsp. paratuberculosis in Wild European starlings at a Kansas cattle feedlot. Avian Dis. 2009, 53, 544–551. [Google Scholar] [CrossRef]
  31. Carta, T.; Álvarez, J.; Pérez de la Lastra, J.M.; Gortázar, C. Wildlife and paratuberculosis: A review. Res. Vet. Sci. 2013, 94, 191–197. [Google Scholar] [CrossRef] [PubMed]
  32. Ott, S.L.; Wells, S.J.; Wagner, B.A. Herd-level economic losses associated with Johne’s disease on US dairy operations. Prev. Vet. Med. 1999, 40, 179–192. [Google Scholar] [CrossRef]
  33. Garcia, A.B.; Shalloo, L. Invited review: The economic impact and control of paratuberculosis in cattle. J. Dairy Sci. 2015, 98, 5019–5039. [Google Scholar] [CrossRef] [PubMed]
  34. McAloon, C.G.; Whyte, P.; More, S.J.; Green, M.J.; O’Grady, L.; Garcia, A.; Doherty, M.L. The effect of paratuberculosis on milk yield—A systematic review and meta-analysis. J. Dairy Sci. 2016, 99, 1449–1460. [Google Scholar] [CrossRef] [PubMed]
  35. Kirkeby, C.; Graesboll, K.; Nielsen, S.S.; Toft, N.; Halasa, T. Epidemiological and economic consequences of purchasing livestock infected with Mycobacterium avium subsp. paratuberculosis. BMC Vet. Res. 2017, 13, 202. [Google Scholar] [CrossRef] [PubMed]
  36. Click, R.E. Successful treatment of asymptomatic or clinically terminal bovine Mycobacterium avium subspecies paratuberculosis infection (Johne’s disease) with the bacterium Dietzia used as a probiotic alone or in combination with dexamethasone: Adaption to chronic human diarrheal diseases. Virulence 2011, 2, 131–143. [Google Scholar] [CrossRef] [PubMed]
  37. Godden, S.M.; Wells, S.; Donahue, M.; Stabel, J.; Oakes, J.M.; Sreevatsan, S.; Fetrow, J. Effect of feeding heat-treated colostrum on risk for infection with Mycobacterium avium ssp. paratuberculosis, milk production, and longevity in Holstein dairy cows. J. Dairy Sci. 2015, 98, 5630–5641. [Google Scholar] [CrossRef] [PubMed]
  38. Verhegghe, M.; Rasschaert, G.; Herman, L.; Goossens, K.; Vandaele, L.; De Bleecker, K.; Vlaemynck, G.; Heyndrickx, M.; De Block, J. Reduction of Mycobacterium avium ssp. paratuberculosis in colostrum: Development and validation of 2 methods, one based on curdling and one based on centrifugation. J. Dairy Sci. 2017, 100, 3497–3512. [Google Scholar] [CrossRef] [PubMed]
  39. Cho, J.; Tauer, L.W.; Schukken, Y.H.; Gómez, M.I.; Smith, R.L.; Lu, Z.; Grohn, Y.T. Economic analysis of Mycobacterium avium subspecies paratuberculosis vaccines in dairy herds. J. Dairy Sci. 2012, 95, 1855–1872. [Google Scholar] [CrossRef] [PubMed]
  40. Lu, Z.; Schukken, Y.H.; Smith, R.L.; Mitchell, R.M.; Gröhn, Y.T. Impact of imperfect Mycobacterium avium subsp. paratuberculosis vaccines in dairy herds: A mathematical modeling approach. Prev. Vet. Med. 2013, 108, 148–158. [Google Scholar] [CrossRef] [PubMed]
  41. Shippy, D.C.; Lemke, J.J.; Berry, A.; Nelson, K.; Hines, M.E.; Talaat, A.M. Superior protection from live-attenuated vaccines directed against Johne’s Disease. Clin. Vaccine Immunol. 2017, 24, e00478-16. [Google Scholar] [CrossRef] [PubMed]
  42. Chaubey, K.K.; Gupta, R.D.; Gupta, S.; Singh, S.V.; Bhatia, A.K.; Jayaraman, S.; Kumar, N.; Goel, A.; Rathore, A.S.; Sahzad; et al. Trends and advances in the diagnosis and control of paratuberculosis in domestic livestock. Vet. Q. 2016, 36, 203–227. [Google Scholar] [CrossRef] [PubMed]
  43. McNees, A.L.; Markesich, D.; Zayyani, N.R.; Graham, D.Y. Mycobacterium paratuberculosis as a cause of Crohn’s disease. Expert Rev. Gastroenterol. Hepatol. 2015, 9, 1523–1534. [Google Scholar] [CrossRef] [PubMed]
  44. Waddell, L.A.; Rajic, A.; Stark, K.D.; Mc, E.S. The zoonotic potential of Mycobacterium avium ssp. paratuberculosis: A systematic review and meta-analyses of the evidence. Epidemiol. Infect. 2015, 143, 3135–3157. [Google Scholar] [CrossRef] [PubMed]
  45. Naser, S.A.; Thanigachalam, S.; Dow, C.T.; Collins, M.T. Exploring the role of Mycobacterium avium subspecies paratuberculosis in the pathogenesis of type 1 diabetes mellitus: A pilot study. Gut Pathog. 2013, 5, 14. [Google Scholar] [CrossRef] [PubMed]
  46. Hesam Shariati, S.; Alaei, A.; Keshavarz, R.; Mosavari, N.; Rabbani, A.; Niegowska, M.; Sechi, L.A.; Feizabadi, M.M. Detection of Mycobacterium avium subsp. paratuberculosis in Iranian patients with type 1 diabetes mellitus by PCR and ELISA. J. Infect. Dev. Ctries. 2016, 10, 857–862. [Google Scholar] [CrossRef] [PubMed]
  47. Songini, M.; Mannu, C.; Targhetta, C.; Bruno, G. Type 1 diabetes in Sardinia: Facts and hypotheses in the context of worldwide epidemiological data. Acta Diabetol. 2017, 54, 9–17. [Google Scholar] [CrossRef] [PubMed]
  48. Cossu, D.; Yokoyama, K.; Hattori, N. Conflicting role of Mycobacterium species in multiple sclerosis. Front. Neurol. 2017, 8, 216. [Google Scholar] [CrossRef] [PubMed]
  49. Singh, A.V.; Chauhan, D.S.; Singh, S.V.; Kumar, V.; Singh, A.; Yadav, A.; Yadav, V.S. Current status of Mycobacterium avium subspecies paratuberculosis infection in animals & humans in India: What needs to be done? Indian J. Med. Res. 2016, 144, 661–671. [Google Scholar] [CrossRef] [PubMed]
  50. Corbett, C.S.; De Buck, J.; Orsel, K.; Barkema, H.W. Fecal shedding and tissue infections demonstrate transmission of Mycobacterium avium subsp. paratuberculosis in group-housed dairy calves. Vet. Res. 2017, 48, 27. [Google Scholar] [CrossRef] [PubMed]
  51. Sechi, L.A.; Paccagnini, D.; Salza, S.; Pacifico, A.; Ahmed, N.; Zanetti, S. Mycobacterium avium subspecies paratuberculosis bacteremia in type 1 diabetes mellitus: An infectious trigger? Clin. Infect. Dis. 2008, 46, 148–149. [Google Scholar] [CrossRef] [PubMed]
  52. Cossu, A.; Rosu, V.; Paccagnini, D.; Cossu, D.; Pacifico, A.; Sechi, L.A. MAP3738c and MptD are specific tags of Mycobacterium avium subsp. paratuberculosis infection in type I diabetes mellitus. Clin. Immunol. 2011, 141, 49–57. [Google Scholar] [CrossRef] [PubMed]
  53. Bach, H.; Rosenfeld, G.; Bressler, B. Treatment of Crohn’s disease patients with infliximab is detrimental for the survival of Mycobacterium avium ssp. paratuberculosis within macrophages and shows a remarkable decrease in the immunogenicity of mycobacterial proteins. J. Crohn’s Colitis 2012, 6, 628–629. [Google Scholar] [CrossRef]
  54. Elguezabal, N.; Chamorro, S.; Molina, E.; Garrido, J.M.; Izeta, A.; Rodrigo, L.; Juste, R.A. Lactase persistence, NOD2 status and Mycobacterium avium subsp. paratuberculosis infection associations to Inflammatory Bowel Disease. Gut Pathog. 2012, 4. [Google Scholar] [CrossRef]
  55. Gill, C.O.; Saucier, L.; Meadus, W.J. Mycobacterium avium subsp. paratuberculosis in dairy products, meat, and drinking water. J. Food Prot. 2011, 74, 480–499. [Google Scholar] [CrossRef] [PubMed]
  56. Eltholth, M.M.; Marsh, V.R.; Van Winden, S.; Guitian, F.J. Contamination of food products with Mycobacterium avium paratuberculosis: A systematic review. J. Appl. Microbiol. 2009, 107, 1061–1071. [Google Scholar] [CrossRef] [PubMed]
  57. Carvalho, I.A.; Pietralonga, P.A.G.; Schwarz, D.G.G.; Faria, A.C.S.; Moreira, M.A.S. Short communication: Recovery of viable Mycobacterium avium subspecies paratuberculosis from retail pasteurized whole milk in Brazil. J. Dairy Sci. 2012, 95, 6946–6948. [Google Scholar] [CrossRef] [PubMed]
  58. Giacometti, F.; Serraino, A.; Finazzi, G.; Daminelli, P.; Losio, M.N.; Arrigoni, N.; Piva, S.; Florio, D.; Riu, R.; Zanoni, R.G. Sale of raw milk in Northern Italy: Food safety implications and comparison of different analytical methodologies for detection of foodborne pathogens. Foodborne Pathog. Dis. 2012, 9, 293–297. [Google Scholar] [CrossRef] [PubMed]
  59. Mundo, S.L.; Gilardoni, L.R.; Hoffman, F.J.; Lopez, O.J. Rapid and sensitive method to identify Mycobacterium avium subsp. paratuberculosis in cow milk using DNA-methylase Genotyping. Appl. Environ. Microbiol. 2012, 79, 1612–1618. [Google Scholar] [CrossRef] [PubMed]
  60. Klanicova, B.; Slana, I.; Roubal, P.; Pavlik, I.; Kralik, P. Mycobacterium avium subsp. paratuberculosis survival during fermentation of soured milk products detected by culture and quantitative real time PCR methods. Int. J. Food Microbiol. 2012, 157, 150–155. [Google Scholar] [CrossRef] [PubMed]
  61. Wong, S.Y.Y.; Grant, I.R.; Friedman, M.; Elliott, C.T.; Situ, C. Antibacterial activities of naturally occurring compounds against Mycobacterium avium subsp. paratuberculosis. Appl. Environ. Microbiol. 2008, 74, 5986–5990. [Google Scholar] [CrossRef] [PubMed]
  62. Crandall, P.G.; Ricke, S.C.; O’Bryan, C.A.; Parrish, N.M. In vitro effects of citrus oils against Mycobacterium tuberculosis and non-tuberculous Mycobacteria of clinical importance. J. Environ. Sci. Health B 2012, 47, 736–741. [Google Scholar] [CrossRef] [PubMed]
  63. Nowotarska, S.W.; Nowotarski, K.I.; Friedman, M.; Situ, C. Effect of structure on the interactions between five natural antimicrobial compounds and phospholipids of bacterial cell membrane on model monolayers. Molecules 2014, 19, 7497–7515. [Google Scholar] [CrossRef] [PubMed]
  64. Blankemeyer, J.T.; White, J.B.; Stringer, B.K.; Friedman, M. Effect of α-tomatine and tomatidine on membrane potential of frog embryos and active transport of ions in frog skin. Food Chem. Toxicol. 1997, 35, 639–646. [Google Scholar] [CrossRef]
  65. Friedman, M.; Burns, C.F.; Butchko, C.A.; Blankemeyer, J.T. Folic acid protects against potato glycoalkaloid α-chaconine-induced disruption of frog embryo cell membranes and developmental toxicity. J. Agric. Food Chem. 1997, 45, 3991–3994. [Google Scholar] [CrossRef]
  66. Burt, S. Essential oils: Their antibacterial properties and potential applications in foods—A review. Int. J. Food Microbiol. 2004, 94, 223–253. [Google Scholar] [CrossRef] [PubMed]
  67. Cho, Y.S.; Schiller, N.L.; Kahng, H.Y.; Oh, K.H. Cellular responses and proteomic analysis of Escherichia coli exposed to green tea polyphenols. Curr. Microbiol. 2007, 55, 501–506. [Google Scholar] [CrossRef] [PubMed]
  68. Raafat, D.; Von Bargen, K.; Haas, A.; Sahl, H.-G. Insights into the mode of action of chitosan as an antibacterial compound. Appl. Environ. Microbiol. 2008, 74, 3764–3773. [Google Scholar] [CrossRef] [PubMed]
  69. Kwon, J.A.; Yu, C.B.; Park, H.D. Bacteriocidal effects and inhibition of cell separation of cinnamic aldehyde on Bacillus cereus. Lett. Appl. Microbiol. 2003, 37, 61–65. [Google Scholar] [CrossRef] [PubMed]
  70. Gustafson, J.E.; Liew, Y.C.; Chew, S.; Markham, J.; Bell, H.C.; Wyllie, S.G.; Warmington, J.R. Effects of tea tree oil on Escherichia coli. Lett. Appl. Microbiol. 1998, 26, 194–198. [Google Scholar] [CrossRef] [PubMed]
  71. Rakotomanga, M.; Saint-Pierre-Chazalet, M.; Loiseau, P.M. Alteration of fatty acid and sterol metabolism in miltefosine-resistant Leishmania donovani promastigotes and consequences for drug-membrane interactions. Antimicrob. Agents Chemother. 2005, 49, 2677–2686. [Google Scholar] [CrossRef] [PubMed]
  72. Gidalevitz, D.; Ishitsuka, Y.; Muresan, A.S.; Konovalov, O.; Waring, A.J.; Lehrer, R.I.; Lee, K.Y. Interaction of antimicrobial peptide protegrin with biomembranes. Proc. Natl. Acad. Sci. USA 2003, 100, 6302–6307. [Google Scholar] [CrossRef] [PubMed]
  73. Giordani, C.; Molinari, A.; Toccacieli, L.; Calcabrini, A.; Stringaro, A.; Chistolini, P.; Arancia, G.; Diociaiuti, M. Interaction of tea tree oil with model and cellular membranes. J. Med. Chem. 2006, 49, 4581–4588. [Google Scholar] [CrossRef] [PubMed]
  74. Simons, K.; Vaz, W.L. Model systems, lipid rafts, and cell membranes. Annu. Rev. Biophys. Biomol. Struct. 2004, 33, 269–295. [Google Scholar] [CrossRef] [PubMed]
  75. Epand, R.M.; Epand, R.F. Domains in bacterial membranes and the action of antimicrobial agents. Mol. BioSyst. 2009, 5, 580–587. [Google Scholar] [CrossRef] [PubMed]
  76. Janas, T.; Nowotarski, K.; Gruszecki, W.I.; Janas, T. The effect of hexadecaprenol on molecular organisation and transport properties of model membranes. Acta Biochim. Pol. 2000, 47, 661–673. [Google Scholar] [PubMed]
  77. Lorite, G.S.; Nobre, T.M.; Zaniquelli, M.E.D.; de Paula, E.; Cotta, M.A. Dibucaine effects on structural and elastic properties of lipid bilayers. Biophys. Chem. 2009, 139, 75–83. [Google Scholar] [CrossRef] [PubMed]
  78. Epand, R.M.; Epand, R.F. Lipid domains in bacterial membranes and the action of antimicrobial agents. Biochim. Biophys. Acta 2009, 1788, 289–294. [Google Scholar] [CrossRef] [PubMed]
  79. Yoneyama, F.; Imura, Y.; Ohno, K.; Zendo, T.; Nakayama, J.; Matsuzaki, K.; Sonomoto, K. Peptide-lipid huge toroidal pore, a new antimicrobial mechanism mediated by a lactococcal bacteriocin, lacticin Q. Antimicrob. Agents Chemother. 2009, 53, 3211–3217. [Google Scholar] [CrossRef] [PubMed]
  80. Smaby, J.M.; Kulkarni, V.S.; Momsen, M.; Brown, R.E. The interfacial elastic packing interactions of galactosylceramides, sphingomyelins, and phosphatidylcholines. Biophys. J. 1996, 70, 868–877. [Google Scholar] [CrossRef]
  81. Hac-Wydro, K.; Wydro, P. The influence of fatty acids on model cholesterol/phospholipid membranes. Chem. Phys. Lipids 2007, 150, 66–81. [Google Scholar] [CrossRef] [PubMed]
  82. Chen, C.Z.; Cooper, S.L. Interactions between dendrimer biocides and bacterial membranes. Biomaterials 2002, 23, 3359–3368. [Google Scholar] [CrossRef]
  83. Ultee, A.; Gorris, L.G.M.; Smid, E.J. Bactericidal activity of carvacrol towards the food-borne pathogen Bacillus cereus. J. Appl. Microbiol. 1998, 85, 211–218. [Google Scholar] [CrossRef] [PubMed]
  84. Sabatini, K.; Mattila, J.-P.; Kinnunen, P.K.J. Interfacial behavior of cholesterol, ergosterol, and lanosterol in mixtures with DPPC and DMPC. Biophys. J. 2008, 95, 2340–2355. [Google Scholar] [CrossRef] [PubMed]
  85. Demel, R.A.; Peelen, T.; Siezen, R.J.; De Kruijff, B.; Kuipers, O.P. Nisin Z, mutant nisin Z and lacticin 481 interactions with anionic lipids correlate with antimicrobial activity: A monolayer study. Eur. J. Biochem. 1996, 235, 267–274. [Google Scholar] [CrossRef] [PubMed]
  86. Diociaiuti, M.; Ruspantini, I.; Giordani, C.; Bordi, F.; Chistolini, P. Distribution of GD3 in DPPC monolayers: A thermodynamic and atomic force microscopy combined study. Biophys. J. 2004, 86, 321–328. [Google Scholar] [CrossRef]
  87. Sikkema, J.; De Bont, J.A.M.; Poolman, B. Mechanisms of membrane toxicity of hydrocarbons. Microbiol. Rev. 1995, 59, 201–222. [Google Scholar] [PubMed]
  88. Paul, S.; Dubey, R.C.; Maheswari, D.K.; Kang, S.C. Trachyspermum ammi (L.) fruit essential oil influencing on membrane permeability and surface characteristics in inhibiting food-borne pathogens. Food Control 2011, 22, 725–731. [Google Scholar] [CrossRef]
  89. Sirk, T.W.; Brown, E.F.; Friedman, M.; Sum, A.K. Molecular binding of catechins to biomembranes: Relationship to biological activity. J. Agric. Food Chem. 2009, 57, 6720–6728. [Google Scholar] [CrossRef] [PubMed]
  90. Sirk, T.W.; Brown, E.F.; Sum, A.K.; Friedman, M. Molecular dynamics study on the biophysical interactions of seven green tea catechins with lipid bilayers of cell membranes. J. Agric. Food Chem. 2008, 56, 7750–7758. [Google Scholar] [CrossRef] [PubMed]
  91. Sirk, T.W.; Friedman, M.; Brown, E.F. Molecular binding of black tea theaflavins to biological membranes: Relationship to bioactivities. J. Agric. Food Chem. 2011, 59, 3780–3787. [Google Scholar] [CrossRef] [PubMed]
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Figure 1. Extracellular levels of phosphate ion in aliquots of Map cultures incubated with various concentrations of cinnamaldehyde (MIC 24 mg/L) and non-inhibitory concentration of ethanol (0.4%, v/v) as the negative control.
Figure 1. Extracellular levels of phosphate ion in aliquots of Map cultures incubated with various concentrations of cinnamaldehyde (MIC 24 mg/L) and non-inhibitory concentration of ethanol (0.4%, v/v) as the negative control.
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Figure 2. Extracellular concentration of phosphate ion in cultures of Map incubated with different active compounds, non-inhibitory compound (vanillic acid) at 74 mg/L, and non-inhibitory concentration of ethanol (0.4%, v/v).
Figure 2. Extracellular concentration of phosphate ion in cultures of Map incubated with different active compounds, non-inhibitory compound (vanillic acid) at 74 mg/L, and non-inhibitory concentration of ethanol (0.4%, v/v).
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Figure 3. Absorbance scan (230 to 370 nm) of 24 mg/L cinnamaldehyde prepared in sterile reverse osmosis water and incubated in (a) absence of and (b) presence of Map NCTC 8578 at 37 °C for 48 h.
Figure 3. Absorbance scan (230 to 370 nm) of 24 mg/L cinnamaldehyde prepared in sterile reverse osmosis water and incubated in (a) absence of and (b) presence of Map NCTC 8578 at 37 °C for 48 h.
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Figure 4. Absorbance scan (230 to 370 nm) of 74 mg/L carvacrol prepared in sterile reverse osmosis water and incubated in (a) absence of and (b) presence of Map NCTC 8578 at 37 °C for 48 h.
Figure 4. Absorbance scan (230 to 370 nm) of 74 mg/L carvacrol prepared in sterile reverse osmosis water and incubated in (a) absence of and (b) presence of Map NCTC 8578 at 37 °C for 48 h.
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Figure 5. The surface pressure-area (π-A) (a) and compression modulus (CS−1) values versus surface pressure (π); and (b) isotherms recorded for monolayers formed by DOPE on the subphases containing pure water with and without naturally-occurring antimicrobial compounds.
Figure 5. The surface pressure-area (π-A) (a) and compression modulus (CS−1) values versus surface pressure (π); and (b) isotherms recorded for monolayers formed by DOPE on the subphases containing pure water with and without naturally-occurring antimicrobial compounds.
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Figure 6. The surface pressure-area (π-A) (a) and compression modulus (CS−1) values versus surface pressure (π); and (b) isotherms recorded for the monolayers formed by DOPG on the subphases containing pure water with and without naturally occurring antimicrobial compounds.
Figure 6. The surface pressure-area (π-A) (a) and compression modulus (CS−1) values versus surface pressure (π); and (b) isotherms recorded for the monolayers formed by DOPG on the subphases containing pure water with and without naturally occurring antimicrobial compounds.
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MDPI and ACS Style

Nowotarska, S.W.; Nowotarski, K.; Grant, I.R.; Elliott, C.T.; Friedman, M.; Situ, C. Mechanisms of Antimicrobial Action of Cinnamon and Oregano Oils, Cinnamaldehyde, Carvacrol, 2,5-Dihydroxybenzaldehyde, and 2-Hydroxy-5-Methoxybenzaldehyde against Mycobacterium avium subsp. paratuberculosis (Map). Foods 2017, 6, 72. https://doi.org/10.3390/foods6090072

AMA Style

Nowotarska SW, Nowotarski K, Grant IR, Elliott CT, Friedman M, Situ C. Mechanisms of Antimicrobial Action of Cinnamon and Oregano Oils, Cinnamaldehyde, Carvacrol, 2,5-Dihydroxybenzaldehyde, and 2-Hydroxy-5-Methoxybenzaldehyde against Mycobacterium avium subsp. paratuberculosis (Map). Foods. 2017; 6(9):72. https://doi.org/10.3390/foods6090072

Chicago/Turabian Style

Nowotarska, Stella W., Krzysztof Nowotarski, Irene R. Grant, Christopher T. Elliott, Mendel Friedman, and Chen Situ. 2017. "Mechanisms of Antimicrobial Action of Cinnamon and Oregano Oils, Cinnamaldehyde, Carvacrol, 2,5-Dihydroxybenzaldehyde, and 2-Hydroxy-5-Methoxybenzaldehyde against Mycobacterium avium subsp. paratuberculosis (Map)" Foods 6, no. 9: 72. https://doi.org/10.3390/foods6090072

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