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Efficacy data of halogenated phenazine and quinoline agents and an NH125 analogue to veterinary mycoplasmas

Abstract

Background

Mycoplasmas primarily cause respiratory or urogenital tract infections impacting avian, bovine, canine, caprine, murine, and reptilian hosts. In animal husbandry, mycoplasmas cause reduced feed-conversion, decreased egg production, arthritis, hypogalactia or agalactia, increased condemnations, culling, and mortality in some cases. Antibiotics reduce transmission and mitigate clinical signs; however, concerning levels of antibiotic resistance in Mycoplasma gallisepticum and M. capricolum isolates exist. To address these issues, we evaluated the minimum inhibitory concentrations (MICs) of halogenated phenazine and quinoline compounds, an N-arylated NH125 analogue, and triclosan against six representative veterinary mycoplasmas via microbroth or agar dilution methods. Thereafter, we evaluated the minimum bactericidal concentration (MBC) of efficacious drugs.

Results

We identified several compounds with MICs ≤25 μM against M. pulmonis (n = 5), M. capricolum (n = 4), M. gallisepticum (n = 3), M. alligatoris (n = 3), M. agassizii (n = 2), and M. canis (n = 1). An N-arylated NH125 analogue, compound 21, served as the most efficacious, having a MIC ≤25 μM against all mycoplasmas tested, followed by two quinolines, nitroxoline (compound 12) and compound 20, which were effective against four and three mycoplasma type strains, respectively. Nitroxoline exhibited bactericidal activity among all susceptible mycoplasmas, and compound 21 exhibited bactericidal activity when the MBC was able to be determined.

Conclusions

These findings highlight a number of promising agents from novel drug classes with potential applications to treat veterinary mycoplasma infections and present the opportunity to evaluate preliminary pharmacokinetic indices using M. pulmonis in rodents as an animal model of human infection.

Background

The Mollicutes, a class of wall-less, fastidious bacteria, cause infections primarily in the respiratory and urogenital tracts in humans, and similarly infect a wide array of animal species including avian, bovine, canine, caprine, murine, and reptilian hosts. Disease negatively impacts aspects of animal husbandry by decreasing feed conversion, egg and milk production, and increasing condemnations and culling [1, 2]. In wildlife, mycoplasmas cause upper respiratory tract (URT) disease in threatened species, including desert and gopher tortoises in the U.S., as well as fulminant disease in the American alligator [3, 4]. Lastly, mycoplasma infection in laboratory animals can skew results and alter immune responses [5]. Use of antibiotics in animals alleviates clinical signs and decreases shedding and hence transmission. However, heavy use of antimicrobials has resulted in increased and sometimes substantial levels of antibiotic resistance in Mycoplasma gallisepticum and M. capricolum isolates [6,7,8]. As mycoplasmas lack a cell wall, this further restricts available treatment to those that interfere with either protein synthesis or DNA replication [9]. Further, as mutations that cause resistance against one drug in a class can extend resistance to others within the same class, novel antibiotics are desperately needed to ensure animal and hence, human health [10].

M. gallisepticum serves as the most pathogenic and economically impactful mycoplasma to infect poultry [1]. In chickens, it causes a classic triad of pneumonia, tracheitis, and airsacculitis, also termed ‘chronic respiratory disease [9].’ In turkeys, M. gallisepticum causes a characteristic ‘infectious sinusitis,’ resulting in severe mucopurulent sinusitis and infraorbital swelling, and airsacculitis that leads to more severe outcomes such as respiratory distress [1]. Illness associated with M. gallisepticum infection negatively impacts commercial flocks by causing reduced feed consumption, weight loss, reductions in egg production, mortality, and carcass downgrading or condemnation upon processing [1]. Although primary prevention methods are employed, outbreaks occur and treatment with broad spectrum antibiotics reduces mortality, pathology, clinical signs, egg production losses, and transmission [1].

However, studies have identified concerning and rising minimum inhibitory concentrations (MICs) in M. gallisepticum isolates. For example, a 2008 Israeli study detected increases in M. gallisepticum MICs to enrofloxacin among isolates from turkeys, and an Israeli study in 2011 found resistance to enrofloxacin, tylosin, and tilmicosin in 72% of M. gallisepticum isolates from 2006 and onward [8]. Further, a study in Jordan found rising MICs over time to all macrolide (n = 3), quinolone (n = 2), and tetracycline (n = 3) compounds tested [6]. M. gallisepticum isolates collected from myriad of countries between 1986 and 2010 found varying levels of enrofloxacin resistance in isolates from England (33%, n = 1), the Netherlands (37.5%, n = 3), Israel (46%, n = 23), Germany (53.3%, n = 8), and Austria (75%, n = 3) [11]. This study also highlighted increasing trends in resistance, as 61% of isolates from 2004 and onward displayed enrofloxacin resistance, compared to only 5.8% of isolates collected pre-2004 [11]. To supplement our summary, Table 1 highlights antibiotic resistance prevalence and MIC50/90 values extracted from recent studies across diverse, geographical settings. A recent review by Gautier-Bouchardon provides a more comprehensive summary of antibiotic resistance trends among M. gallisepticum field isolates [8].

Table 1 Antibiotic resistance prevalence and MIC50/90 values of M. gallisepticum field isolates to select antibiotics

Mycoplasma capricolum sub. capricolum (Mcc), detected primarily in regions that support small ruminant dairy production in Europe, the Mediterranean, North Africa, and sporadically in the U.S., serves as one of the three principal agents that causes contagious agalactia (CA) [16]. Mcc, more prevalent in goats than sheep, can cause severe serous or fibrinopurulent arthritis, mastitis, hypogalactia or agalactia, and abortion in adults and death in kids [16]. In countries that depend on goat and sheep products as large dietary sources or exports, economic losses from agalactia, abortions, reduced growth, culling or death due to Mcc can have substantial impacts [2]. To avoid economic losses, the industry relies on vaccines and antibiotics. A trivalent, killed vaccine incorporating a Mcc antigen exists; however, there is little data available regarding its efficacy [17]. Unlike M. gallisepticum, less data on antibiotic resistance in Mcc exists. A recent study evaluating antibiotic resistance in 32 Mcc field isolates from the Canary Islands, mainland Spain, and Italy found notable levels of resistance to erythromycin (100%), norfloxacin (77.4%), spectinomycin (64.5%), clindamycin (48.4%), and tylosin (19.4%) [7]. In contrast, a study performed in Jordan from 2002 to 2003 found no resistance and strikingly lower MIC50/90 values to erythromycin, tylosin, and enrofloxacin [18]. Table 2 highlights additional findings from these two studies.

Table 2 Antibiotic resistance prevalence and MIC50/90 values of M. capricolum subsp. capricolum

M. canis, designated as an opportunistic pathogen, primarily causes urogenital tract disease but has been associated with granulomatous or necrotizing meningoencephalitis in canines [9, 19, 20]. Likely through canine-cattle interactions, M. canis has been identified in cattle from Canada and northern Europe, and was detected in 13 pneumatic calf outbreaks in Britain during the mid- to late-1990s [17]. M. canis served as the sole agent detected in five outbreaks, wherein three outbreaks reported calf mortality [17, 21]. Recently, M. canis was isolated from wound tissues of a German woman after a dog bite [22]. No studies have investigated antibiotic resistance in M. canis isolated from either dogs or cattle.

Mycoplasmas that infect reptilians include, but are not limited to M. alligatoris, a virulent pathogen of alligators and caimans, and M. agassizii, a pathogen that causes URT disease in tortoises. M. alligatoris was initially discovered as the causative agent of an outbreak among captive alligators that caused interstitial pneumonia, fibrinous pericarditis, arthritis, and 80% herd mortality [4]. Seroprevalence studies across Florida detected 60% seropositivity among 20 sites tested, and 5.4% seropositivity overall among 32 samples [23]. In-vitro studies found M. alligatoris isolates had low MICs (< 1 mg/L) to doxycycline, enrofloxacin, tilmicosin, and tylosin, but higher MICs against erythromycin (32–128 mg/L), chloramphenicol (8–16 mg/L), and clindamycin (1–8 mg/L) [24].

In the 1980s, an URT infection coupled with other factors coincided with substantial declines in the desert tortoise (Gopherus agassizii) population in the Mojave Desert in California, with similar disease occurring in wild and captive gopher tortoises (G. polyphemus) in Florida [25]. Isolation, sequencing, and experimental infection studies led to identification of M. agassizii as a unique mycoplasma species that causes dyspnea, nasal discharge, rhinitis, and conjunctivitis in desert and gopher tortoises [3, 26]. Although enrofloxacin has been used to treat infected tortoises, it does not completely eliminate the organism [3].

M. pulmonis, which causes pathology in both the respiratory and urogenital tracts, as well as otitis media, conjunctivitis, and arthritis, infects both captive and wild rodents [9, 27]. M. pulmonis infection in laboratory rats and mice, in concert with its effects on the immune system, can confound research studies, especially as subclinical infections can escape detection [5]. M. pulmonis genital and respiratory mycoplasmosis prevalence in laboratory rats has been reported in up to 40% and in nearly 100% of conventionally-maintained animals, respectively [27]. Antibiotics are employed during rederivation to prevent vertical transmission following embryo transfer [5, 28]. Urogenital and respiratory infection models in rodents have been established for M. pulmonis; therefore novel antibiotics found effective against M. pulmonis could undergo pharmacokinetic and pharmacodynamic (PK/PD) analysis using these infection models to determine preliminary parameters [27, 29].

Herein, we evaluated the MICs and minimum bactericidal concentrations (MBCs) of a collection of seven halogenated phenazine and quinoline compounds, an N-arylated NH125 analogue, nitroxoline, and triclosan against six veterinary Mycoplasma spp. type strains (Fig. 1). The library of halogenated phenazine and quinoline compounds and the NH125 analogue were created by using a previously efficacious compound as a base structure and modifying different chemical groups at targeted sites to produce a library of more potent phenazine, quinoline, and NH125 analogues [30,31,32]. Nitroxoline, a compound approved for treating urinary tract infections outside of the U.S., was added to the testing as it has a similar structure to the compounds in the library. Triclosan was included as an agent known to be effective against several microorganisms [33, 34]. In a previous study, we tested this library of novel agents against clinical isolates of Ureaplasma spp. and M. hominis, as well as against human mycoplasma type strains [35]. We found a number of compounds with efficacious MICs against several human mycoplasmas that have displayed elevated resistance patterns in recent years [35]. With antibiotic resistance increasing in both human and animal mycoplasmas and limited therapeutic options available for mycoplasma treatment, new classes of antibiotics are needed in both human and veterinary medicine. Further, as well-established murine models of mycoplasma respiratory and urogenital tract infections exist, compounds effective against M. pulmonis could serve as a stepping stone for establishing important PK/PD parameters for furthering these compounds along the translational spectrum.

Fig. 1
figure1

Compounds synthesized by the Huigens Lab. Halogenated phenazine and quinoline compounds, and an N-arylated NH125 analogue have gray, orange, and green boxes around compound numbers, designating each class, respectively. Compounds with an orange and blue dotted box surrounding their structure represent those that had the most frequent MICs ≤25 μM against the veterinary mycoplasmas and demonstrated bactericidal activity against four mycoplasmas. A blue, dotted box represents the third most efficacious compound

Results

MIC results (Table 3)

Overall, an N-arylated NH125 analogue (compound 21), nitroxoline (compound 12), and a quinoline (compound 20), proved most effective against the veterinary mycoplasmas. Compound 21 had MICs ≤25 μM (11.6 mg/L) to all type strains (n = 6), and had a median MIC of 15.7 μM (7.3 mg/L) (95% CI: 12.5–25 μM) against these organisms. Nitroxoline had MICs ≤25 μM (4.8 mg/L) against four type strains: M. alligatoris, M. capricolum, M. gallisepticum, and M. pulmonis, with a median MIC of 12.5 μM (2.4 mg/L) (95% CI: 6.25–25 μM) against these four organisms. Compound 20 had MICs ≤25 μM (7.9 mg/L) against three type strains, M. alligatoris, M. capricolum, and M. gallisepticum, but had a slightly higher median MIC of 18.8 μM (5.93 mg/L) (95% CI: 12.5–25 μM) against these organisms. Compound 10, a quinoline, and compounds 11 and 14, halogenated quinolines, were solely effective against M. pulmonis and each had a MIC of 12.5 μM. Compound 15, a halogenated quinoline and compound 19, a halogenated phenazine, had MICs of 25 μM against M. agassizii and M. capricolum, respectively. Compound 4 served as the only test compound that did not have a MIC ≤25 μM against any of the type strains.

Table 3 MIC results of test agents against veterinary mycoplasma type strains

The organisms most susceptible to the test compounds were M. pulmonis, M. capricolum, and M. gallisepticum, wherein five (55%), four (44%) and three (33%) compounds had MICs ≤25 μM against each, respectively. Among the compounds that registered MICs ≤25 μM against M. pulmonis and M. gallisepticum, the median MIC for those compounds was 12.5 μM against each; for the four found effective against M. capricolum, the median MIC of those compounds was 18.8 μM. Although M. canis and M. agassizii had fewer compounds that displayed MICs ≤25 μM against them, compound 21 had a low, median MIC of 12.5 μM (5.8 mg/L) against M. canis and a median MIC of 18.8 μM (8.7 mg/L) against M. agassizii. Triclosan was most effective against reptilian mycoplasmas (M. alligatoris, MIC: 120 μM and M. agassizii, MIC: 60 μM) and an avian mycoplasma (M. gallisepticum, MIC: 120 μM). Triclosan had MICs > 120 μM against the mammalian mycoplasma type strains. The raw MIC data are available in Supplemental File 1.

MBC results (Table 4)

In terms of the MBC assays, many of the compounds had MICs on the higher end of the doses tested. Therefore, in some cases, the MBC was undetermined as one requires information on growth at 4X the MIC to determine if the drug demonstrates bacteriostatic activity. However, as some drugs had MBCs at the MIC or 2X the MIC level, we were able to ascertain bactericidal activity in those cases. This was the case for nitroxoline and compound 21. Nitroxoline exhibited bactericidal activity against four type strains including M. alligatoris, M. capricolum, M. gallisepticum, and M. pulmonis. Among those type strains, nitroxoline had the lowest MBCs against M. pulmonis (mean MBC: 17.5 μM; 3.3 mg/L) and M. gallisepticum (MBCs: 12.5, 25 μM; 2.4, 4.8 mg/L). Compound 21 demonstrated bactericidal activity against all mycoplasmas that underwent MBC testing (M. agassizii, M. canis, M. gallisepticum, and M. pulmonis) in all but two cases (M. alligatoris, M. capricolum), wherein the activity was undeterminable. For the remaining test compounds (10, 11, 14, 15, 19, 20), their MBC was undeterminable. Overall, nitroxoline and compound 21 exhibited bactericidal activity against the majority of type strains. The raw MBC data are available in Supplemental File 1.

Table 4 MBC data for test agents against veterinary mycoplasma type strains

Discussion

Veterinary mycoplasmas inflict substantial fiscal burdens in the poultry, dairy, and beef industries and are often refractory to treatment [1, 2, 6, 36]. Rising antibiotic resistance, mutations that confer resistance to multiple drugs within a single class, mycoplasmas, inherent resistance to major drug classes, and animals with persistent carrier status necessitate the identification of new drug classes [6, 7, 9, 10, 16, 37]. To address these issues, we tested a combination of halogenated phenazines and quinolines, an NH125 analogue, and triclosan against six veterinary mycoplasmas to facilitate identification of new treatment modalities.

We evaluated MICs using methods derived from a standardized, Clinical Laboratory Standards Institute (CLSI) protocol for evaluating resistance among human mycoplasmas [38]. As antibiotic resistance continues to emerge and new drugs need evaluation, a standardized method should be adopted for the purposes of ensuring validity and comparability across studies. Validated, established guidelines can also reduce time spent determining quality control limits and optimizing procedures which will enhance knowledge dissemination and facilitate drug evaluation against mycoplasmas that infect animals.

Overall, we identified compounds in the quinoline and phenazine families and an N-arylated NH125 analogue that exhibited MICs ≤25 μM against a diverse group of veterinary mycoplasmas. A previous study found evidence to support that NH125 analogues, such as compound 21, have a mechanism of action that involves rapid bacterial membrane destruction [39]. As mycoplasmas lack a cell wall, leaving its bacterial membrane vulnerable, we posited that NH125 analogues would demonstrate efficacy and bactericidal activity against mycoplasmas. We found evidence for the former hypothesis, as compound 21 had MICs ≤25 μM against all six mycoplasma type strains in this study. Our results reflect a similar trend in compound 21 efficacy against mycoplasmas, as a recent study found that compound 21 displayed low MICs against M. pneumoniae, M. genitalium (MICs: 3.13 μM), and 72 Ureaplasma spp. clinical isolates (MIC90: 12.5 μM) [35]. In this study, we found some support for the latter hypothesis, as compound 21 demonstrated bactericidal activity in all scenarios wherein one could determine the MBC, which included bactericidal activity against M. agassizii, M. canis, M. gallisepticum, and M. pulmonis type strains.

Nitroxoline (compound 12) and compound 20 served as the second and third most effective compounds against the veterinary mycoplasmas, having a MIC ≤25 μM against four and three type strains, respectively. In particular, both had low MICs against M. capricolum and M. gallisepticum—two mycoplasmas that have had significant and rising levels of antibiotic resistance in recent years, respectively. Further, nitroxoline demonstrated bactericidal activity in all veterinary mycoplasmas tested. This serves as a property which could reduce mycoplasma carrier status among herds or flocks following infection and treatment, when stress could decrease immune clearance of the pathogen.

The collection of halogenated phenazine and quinoline compounds tested in this study originated by probing pyocyanin, a compound produced within the natural setting through bacterial competition. Pyocyanin, a phenazine compound produced by Pseudomonas aeruginosa and the presumed compound credited with outcompeting Staphylococcus aureus in the context of cystic fibrosis lung infections, served as the base structure used to initiate this exploration [40]. Halogenated phenazine analogue libraries were created by substituting and testing the impact of different chemical moieties at key positions along the pyocyanin cyclic structure. Through scaffold hopping, similar quinoline structures were synthesized that possessed key structural features such as a 1-hydroxy atom positioned adjacently on the second aromatic ring. Later experiments revealed that such positioning created a five-membered chelate, responsible for starving bacterial biofilms by binding with divalent metal cations [41]. Nitroxoline’s mechanism of action also involves divalent, metal ion chelation [42]. Previous studies indicated reduced nitroxoline efficacy in the presence of Mg2+ and Mn2+ coupled with spectrophotometric absorbance shifts indicating formation of drug-ion complexes for which stability of Mn2+ and Mg2+ superseded that of Ca2+ [42].

In our study, we identified that M. pulmonis appeared more susceptible to the halogenated quinoline compounds compared to other veterinary mycoplasmas. Few studies have examined the impact of iron chelation in mycoplasmas. However, one study found that incubating the chelating agent, 2,2′ -dipyridyl for 12 h with M. pulmonis at 1 mg/mL versus 0.1 mg/mL decreased the CFU by over 97%, compared to a 50% CFU reduction seen in M. gallisepticum [43]. Only after 30 h, treatment with 2,2′ -dipyridyl resulted in a 95% decrease in M. gallisepticum CFU [43]. Thus, based on that data, it appears that M. pulmonis might have less resilience in dealing with iron sequestration, which could explain why more halogenated quinolines had an impact on M. pulmonis compared to M. gallisepticum.

For M. pulmonis, compounds 10, 11, 12 and 14 also had efficacious MICs compared to sister quinolines 15 and 20. In previous studies evaluating halogenated quinoline libraries against MRSA and MRSE, compounds 15 and 20 demonstrated 1.5 and 4-fold higher MICs to MRSA, and compound 20 had a 6-fold higher MIC to MRSE compared to compound 14 [30, 31]. Thus, it appears this might be reflective of potency seen against other gram-positive organisms, albeit compound 20 had more frequent, efficacious MICs overall against the veterinary mycoplasmas.

It makes sense that compounds 10, 11, 12, and 14 had efficacious MICs against M. pulmonis as a cluster, since they have very similar structural motifs. For M. pulmonis, it appears that the quinolines proved effective (had MICs at 12.5 μM) when a nitrite was present at the 5-position, regardless of additional methyl or halogenated groups. However, substituting the nitrite with a bromine coupled with addition of a bromine at the 7-position proved effective only when a methyl group was stationed at the 2-position. Interestingly, previous studies evaluating halogenated quinoline against MRSE also identified the 2-position as a key component of the quinoline scaffold for enhanced activity [44]. However, it appears that compound 15, bearing a chlorinated phenol group attached via a nitrogen group, did not show effectiveness. The reason for this is unknown. Further, nitroxoline had more efficacious MICs compared to similar analogues; thus, additional methyl or halogenated groups on the scaffold did not seem to enhance antimicrobial against veterinary mycoplasmas in general.

Compounds that had efficacious MICs against M. pulmonis (10, 12, 14, and 21) also had previously efficacious MICs against human mycoplasmas [35]. As M. pulmonis infection models have been established in rats for both urogenital and respiratory tract disease [27, 29], one could use these established models to evaluate important PK/PD parameters to determine a compound’s preliminary, therapeutic index. This would contribute to important pre-clinical information to advance knowledge of these compounds to prepare them for clinical studies.

In terms of preliminary safety testing, in-vitro work showed that compounds 14 and 20 produced scant hemolysis at doses of 200 μM (≤ 1%), but compound 15 caused hemolysis in 18.8% of red blood cells at 200 μM [30, 31]. Thus far, the majority of halogenated phenazine compounds have showed no cytotoxicity against HeLa cells at concentrations of 100 μM [41]. However, the N-arylated NH125 analogue demonstrated potent hemolysis activity against human red blood cells [32]. Therefore, NH125 analogues may have applications as disinfectants or antiseptics.

As the halogenated phenazine and quinoline compounds contain a hydroxyl group, they are potential substrates for biotransformation via glucuronidation and sulfonation, the same pathways used by triclosan. The glucuronide and sulfate metabolites would likely be inactive and terminate their biological activity. Preliminary studies have shown that although both glucuronide and sulfate metabolites can be formed in human liver microsomes, these compounds are relatively poor substrates that are slowly metabolized [45].

We added further information on the efficacy of triclosan against veterinary mycoplasmas. Herein, we found that triclosan had a MIC of 60 μM (17.4 mg/L) against M. alligatoris and MICs of 120 μM (34.7 mg/L) against M. gallisepticum and M. agassizii. One previous study evaluated triclosan’s efficacy against two distinct M. gallisepticum type strains (PG31 and BG44T) and reported similar MICs (32 mg/L; 110 μM) to what we found in the M. gallisepticum S6 type strain [46].

Although our work and that of others have shown triclosan to be an effective antibacterial, it is a somewhat controversial chemical. The FDA banned the use of triclosan in soaps and body washes sold to the general public in the U.S. effective September 2017 and banned its use in medical settings effective December 2018. This was because concerns were raised about triclosan’s environmental persistence, the toxicity of triclosan’s breakdown products, and the endocrine-disrupting activities of triclosan itself [47, 48]. However, the FDA permitted triclosan’s continued use in plaque-reducing toothpaste, and it is not banned world-wide.

One issue that plagues husbandry includes subclinical persistence of mycoplasmas following treatment, which can lead to relapse or inadvertent introduction to naïve flocks or herds during transhumance [16, 37]. Further, relapse of Mcc has been reported to range between 10 and 30% in herds [16]. Some postulate that biofilms may give rise to carrier status and cause relapse [49]. Thus, antibiofilm activity of antimicrobials against mycoplasmas could serve as an effective property. Several of the compounds found to have lower MICs against these veterinary mycoplasmas (12, 14, 15, 20, and 21) also reported effective eradication activities against MRSA and MRSE biofilms in prior studies [30, 32, 50]. Studies have identified that M. gallisepticum, M. pulmonis and, to a lesser extent, Mcc form biofilms [49, 51, 52]. Thus, future directions include studying the biofilm eradicating properties of these compounds in mycoplasmas, which may have implications for animal and human health.

Conclusion

Overall, we found a number of compounds belonging to three novel antimicrobial classes that had activity against a group of diverse mycoplasmas that infect food and fiber, companion, reptilian as well as laboratory animals. In determining bactericidal or bacteriostatic activity, we found that nitroxoline possessed bactericidal activity against all veterinary mycoplasmas tested, while an NH125 analogue had bactericidal activity against M. agassizii, M. canis, M. gallisepticum, and M. pulmonis. This property may serve as a useful characteristic to limit mycoplasma carrier status, which contributes to ongoing mycoplasma transmission and subsequent health and agricultural losses. Further, as the majority of compounds showed activity against M. pulmonis, which serves as an existing animal model to study both respiratory and urogenital mycoplasmas in humans, this could serve as a starting point to calculate essential, pre-clinical compound data.

Methods

Mycoplasma type strains

For this study, we evaluated the test compounds against the following six veterinary mycoplasma type strains: M. agassizii ATCC 700616, M. alligatoris ATCC 700619, M. canis PG14 (ATCC 19525), Mycoplasma capricolum sub. capricolum ATCC 27343, M. gallisepticum S6 (ATCC 15302), and M. pulmonis × 1048. For stock culture growth and MIC/MBC testing of M. agassizii, M. alligatoris, and M. canis type strains, we used our standard, laboratory prepared SP4 medium and agar supplemented with glucose with a pH range between 7.6–7.8. For M. capricolum, M. gallisepticum, and M. pulmonis culture and MIC/MBC testing, we used our standardized, laboratory prepared Frey’s medium and agar, supplemented with glucose at a pH between 7.6–7.8.

Antimicrobial compounds

For quality control purposes, we used enrofloxacin and tylosin tartrate sourced from Sigma Aldrich (St. Louis, MO, USA). Stock solutions of quality control agents were dissolved and diluted according to CLSI standards, and drug purity was accounted for during the dilution process [53]. We stored stock solutions in 1 mL aliquots at − 20 °C for up to 3 months. MICs obtained from quality control drugs that were within a four-fold dilution range were considered acceptable for quality control purposes. The test compounds and triclosan were provided at either 10 mM or 1 mM concentrations in DMSO and were stored at room temperature, protected from light. Drugs were diluted in broth on the day of testing and tested within 6 months of receipt.

MIC determination

We followed a previously validated, microbroth or agar dilution method to evaluate MICs as previously described [35, 38]. For the microbroth dilution assay, we used sterile, 96-well plates wherein each row contained an antimicrobial agent in doubling dilutions from 25 μM to 3.13 μM for each type strain, in duplicate, unless otherwise noted in Table 3. Duplicate growth control, drug control, solvent control, and medium controls were set up for each drug and organism tested. A 1:10 dilution of DMSO served as the solvent control. Plates were inoculated with 175 μL of organism between 104 and 105 CFU/mL, unless otherwise indicated, which was pre-incubated in broth for either 1 hour for M. alligatoris or for 2 hours for all other mycoplasmas tested. Plates were sealed with sterile acetate sealers in ambient air and incubated at 37 °C for all mycoplasma type strains except for M. alligatoris and M. agassizii, which were incubated at 30 °C. When the growth control displayed a distinct color change, the MIC was read and interpreted as the lowest concentration of drug that inhibited any color change. We confirmed the organism CFU and CCU on the date of testing and reported results when an organism’s CFU fell outside of this range in two cases. MIC readings were confirmed with a second, independent test. In some cases, multiple MICs were obtained from the initial MIC testing and from conducting the MBC assays. Under these circumstances, the median MIC and the corresponding 95% confidence interval was reported for each drug/organism combination.

As compound 12 (nitroxoline), altered broth color due to its yellow hue at concentrations of 12.5 μM and higher, drug control wells at drug concentrations ≥12.5 μM were placed adjacent to the drug and organism wells, so as to represent the baseline color for that drug concentration in broth. The MIC was interpreted as the lowest drug concentration with no visible color change compared to the corresponding control well.

In the event that a compound and organism combination did not show a distinct color change in broth, which occurred when testing compound 20 and triclosan against M. canis, we confirmed the MIC using a validated agar dilution method to evaluate drug MIC. Briefly, the method consisted of incorporating 600 μL of antibiotic within 5.4 mL of molten agar by adding the appropriate volume of stock antibiotic to yield concentrations spanning from 25 to 3.13 μM for each drug. We created a solvent and growth control plate by mixing 5.4 mL of molten agar with 600 μL of a 1:10 DMSO solution and with 600 μL of filter-sterilized, double-distilled water, respectively. Following a two-hour pre-incubation period, we added three separate 10 μL drops of organism at 103, 104 and 105 CFU/mL concentrations onto each agar plate. Using the organism dilution between 104 and 105 CFU/mL, the MIC for each drug was read as the lowest antibiotic concentration that inhibited colony formation when the growth control plate exhibited colonies.

MBC determination

We evaluated the MBCs of compounds that had MICs ≤25 μM by adapting a previously published method [54]. The MBC assay called for transferring 30 μL aliquots directly from the MIC microtiter plate at 1, 2 and 4 times the MIC drug concentration into culture tubes with 2.97 mL of fresh broth immediately following MIC interpretation. For positive and negative controls, we transferred 30 μL from the growth control and 30 μL from the medium control into separate tubes with 2.97 mL of fresh broth. Following inoculation, all tubes were incubated at 37 °C (or at 30 °C for reptilian mycoplasmas) in ambient air for 14 and 10 days for M. agassizii and M. gallisepticum, respectively, and for 7 days for all other veterinary mycoplasmas. Compounds were considered bactericidal if the lowest concentration that did not show growth was within one to four times the predetermined MIC level following incubation. We replicated the MBC assay for compounds that registered an MBC value considered bactericidal.

Availability of data and materials

The datasets used and analyzed during the current study are available from the corresponding author on reasonable request. All mycoplasma type strains used in testing are available through the American Type Culture Collection (https://www.atcc.org), with the exception of M. pulmonis × 1048, which can be requested through the Mycoplasma Culture Collection (http://iom-online.org/node/28).

Abbreviations

CA:

Contagious agalactia

CLSI:

Clinical Laboratory Standards Institute

MBC:

Minimum bactericidal concentration

Mcc:

Mycoplasma capricolum sub. capricolum

MIC:

Minimum inhibitory concentration

PD:

Pharmacodynamic

PK:

Pharmacokinetic

URT:

Upper respiratory tract

References

  1. 1.

    Ley DH. Mycoplasma gallisepticum infection. In: Saif YM, editor. Diseases of poultry. Ames, Iowa: Blackwell Publishing; 2008. p. 807–34.

    Google Scholar 

  2. 2.

    Gómez-Martín A, Amores J, Paterna A, De la Fe C. Contagious agalactia due to Mycoplasma spp. in small dairy ruminants: epidemiology and prospects for diagnosis and control. Vet J. 2013;198(1):48–56.

    PubMed  Article  PubMed Central  Google Scholar 

  3. 3.

    Origgi FC, Jacobson ER. Diseases of the respiratory tract of chelonians. Vet Clin North America. 2000;3(2):537–49.

    CAS  Google Scholar 

  4. 4.

    Clippinger TL, Bennett RA, Johnson CM, Vliet KA, Deem SL, Oros J, et al. Morbidity and mortality associated with a new mycoplasma species from captive American alligators (Alligator mississippiensis). J Zoo Wildl Med. 2000;31(3):303–14.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  5. 5.

    Otto GM, Franklin CL, Clifford CB, Fox JG, Anderson LC, Pritchett-Corning KR, et al. Chapter 4 - biology and diseases of rats. In: Laboratory animal medicine. 3rd ed. Boston: Academic Press; 2015. p. 151–207.

    Google Scholar 

  6. 6.

    Gharaibeh S, Al-Rashdan M. Change in antimicrobial susceptibility of Mycoplasma gallisepticum field isolates. Vet Microbiol. 2011;150(3–4):379–83.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  7. 7.

    Tatay-Dualde J, Prats-van der Ham M, de la Fe C, Paterna A, Sanchez A, Corrales JC, et al. Antimicrobial susceptibility and multilocus sequence typing of Mycoplasma capricolum subsp. capricolum. PLoS One. 2017;12(3):e0174700.

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  8. 8.

    Gautier-Bouchardon AV. Antimicrobial resistance in Mycoplasma spp. Microbiol Spectr. 2018;6(4). https://doi.org/10.1128/microbiolspec.ARBA-0030-2018.

  9. 9.

    Brown DR. Phylum XVI. Tenericutes Murray 1984a, 356VP (effective publication: Murray 1984b, 33.). In: Krieg NR, Staley JT, Brown DR, Hedlund BP, Paster BJ, Ward NL, et al., editors. Bergey’s manual® of systematic bacteriology: volume four the Bacteroidetes, Spirochaetes, Tenericutes (Mollicutes), Acidobacteria, Fibrobacteres, Fusobacteria, Dictyoglomi, Gemmatimonadetes, Lentisphaerae, Verrucomicrobia, Chlamydiae, and Planctomycetes. New York, NY: Springer New York; 2010. p. 567–723.

  10. 10.

    Fair RJ, Tor Y. Antibiotics and bacterial resistance in the 21st century. Perspect Med Chem. 2014;6:25–64.

    Google Scholar 

  11. 11.

    Lysnyansky I, Gerchman I, Levisohn S, Mikula I, Feberwee A, Ferguson NM, et al. Discrepancy between minimal inhibitory concentration to enrofloxacin and mutations present in the quinolone-resistance determining regions of Mycoplasma gallisepticum field strains. Vet Microbiol. 2012;160(1–2):222–6.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  12. 12.

    Gerchman I, Levisohn S, Mikula I, Manso-Silván L, Lysnyansky I. Characterization of in vivo-acquired resistance to macrolides of Mycoplasma gallisepticum strains isolated from poultry. Vet Res. 2011;42:90.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  13. 13.

    Ammar AM, Abd El-Aziz NK, Gharib AA, Ahmed HK, Lameay AE. Mutations of domain V in 23S ribosomal RNA of macrolide-resistant Mycoplasma gallisepticum isolates in Egypt. J Infect Dev Ctries. 2016;10(8):807–13.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  14. 14.

    Beylefeld A, Wambulawaye P, Bwala DG, Gouws JJ, Lukhele OM, Wandrag DBR, et al. Evidence for multidrug resistance in nonpathogenic Mycoplasma species isolated from South African poultry. Appl Environ Microbiol. 2018;84(21).

  15. 15.

    Hannan PC. Guidelines and recommendations for antimicrobial minimum inhibitory concentration (MIC) testing against veterinary mycoplasma species. International research Programme on comparative Mycoplasmology. Vet Res. 2000;31(4):373–95.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  16. 16.

    Bergonier D, Berthelot X, Poumarat F. Contagious agalactia of small ruminants: current knowledge concerning epidemiology, diagnosis and control. Rev Sci Tech. 1997;16(3):848–73.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  17. 17.

    Nicholas R, Ayling R, McAuliffe L. Mycoplasma diseases of ruminants : disease, diagnosis and control. Wallingford, United Kingdom: CABI; 2008.

    Google Scholar 

  18. 18.

    Al-Momani W, Nicholas RA, Janakat S, Abu-Basha E, Ayling RD. The in vitro effect of six antimicrobials against Mycoplasma putrefaciens, Mycoplasma mycoides subsp. mycoides LC and Mycoplasma capricolum subsp. capricolum isolated from sheep and goats in Jordan. Trop Anim Health Prod. 2006;38(1):1–7.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  19. 19.

    Chalker VJ. Canine mycoplasmas. Res Vet Sci. 2005;79(1):1–8.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  20. 20.

    Barber RM, Porter BF, Li Q, May M, Claiborne MK, Allison AB, et al. Broadly reactive polymerase chain reaction for pathogen detection in canine granulomatous meningoencephalomyelitis and necrotizing meningoencephalitis. J Vet Intern Med. 2012;26(4):962–8.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  21. 21.

    Chazel M, Tardy F, Le Grand D, Calavas D, Poumarat F. Mycoplasmoses of ruminants in France: recent data from the national surveillance network. BMC Vet Res. 2010;6:32.

    PubMed  PubMed Central  Article  Google Scholar 

  22. 22.

    Klein S, Klotz M, Eigenbrod T. First isolation of Mycoplasma canis from human tissue samples after a dog bite. New Microbes New Infect. 2018;25:14–5.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  23. 23.

    Brown DR, Zacher LA, Carbonneau DA. Seroprevalence of Mycoplasma alligatoris among free-ranging alligators (Alligator mississippiensis) in Florida—2003. J Zoo Wildl Med. 2005;36(2):340–1.

    PubMed  Article  PubMed Central  Google Scholar 

  24. 24.

    Helmick KE, Brown DR, Jacobson ER, Brown MB. In vitro drug susceptibility pattern of Mycoplasma alligatoris isolated from symptomatic American alligators (Alligator mississippiensis). J Zoo Wildl Med. 2002;33(2):108–11.

    PubMed  Article  PubMed Central  Google Scholar 

  25. 25.

    Jacobson ER, Brown MB, Wendland LD, Brown DR, Klein PA, Christopher MM, et al. Mycoplasmosis and upper respiratory tract disease of tortoises: a review and update. Vet J. 2014;201(3):257–64.

    PubMed  Article  PubMed Central  Google Scholar 

  26. 26.

    Brown MB, Brown DR, Klein PA, McLaughlin GS, Schumacher IM, Jacobson ER, et al. Mycoplasma agassizii sp. nov., isolated from the upper respiratory tract of the desert tortoise (Gopherus agassizii) and the gopher tortoise (Gopherus polyphemus). Int J Syst Evol Microbiol. 2001;51(Pt 2):413–8.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  27. 27.

    Brown MB, Peltier M, Hillier M, Crenshaw B, Reyes L. Genital mycoplasmosis in rats: a model for intrauterine infection. Am J Reprod Immunol. 2001;46(3):232–41.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  28. 28.

    Charles River Research Models and Services: Mycoplasma pulmonis: Technical Sheet. 2009. https://www.criver.com/sites/default/files/resources/MycoplasmapulmonisTechnicalSheet.pdf. Accessed 08 March 2020.

  29. 29.

    Baker DG. Natural pathogens of laboratory mice, rats, and rabbits and their effects on research. Clin Microbiol Rev. 1998;11(2):231–66.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  30. 30.

    Garrison AT, Abouelhassan Y, Yang H, Yousaf HH, Nguyen TJ, Huigens RW III. Microwave-enhanced Friedländer synthesis for the rapid assembly of halogenated quinolines with antibacterial and biofilm eradication activities against drug resistant and tolerant bacteria. Med Chem Commun. 2017;8:720–4.

    CAS  Article  Google Scholar 

  31. 31.

    Basak A, Abouelhassan Y, Huigens RW. Halogenated quinolines discovered through reductive amination with potent eradication activities against MRSA, MRSE and VRE biofilms. Org Biomol Chem. 2015;13(41):10290–4.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  32. 32.

    Abouelhassan Y, Basak A, Yousaf H, Huigens RW 3rd. Identification of N-arylated NH125 analogues as rapid eradicating agents against MRSA persister cells and potent biofilm killers of gram-positive pathogens. Chembiochem. 2017;18(4):352–7.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  33. 33.

    Jones RD, Jampani HB, Newman JL, Lee AS. Triclosan: a review of effectiveness and safety in health care settings. Am J Infect Control. 2000;28(2):184–96.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  34. 34.

    Rodricks JV, Swenberg JA, Borzelleca JF, Maronpot RR, Shipp AM. Triclosan: a critical review of the experimental data and development of margins of safety for consumer products. Crit Rev Toxicol. 2010;40(5):422–84.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  35. 35.

    Valentine-King MA, Cisneros K, James MO, Huigens RW 3rd, Brown MB. Turning the tide against antibiotic resistance by evaluating novel, halogenated phenazine, quinoline, and NH125 compounds against Ureaplasma spp. clinical isolates and Mycoplasma type strains. Antimicrob Agents Chemother. 2019;63(3). https://doi.org/10.1128/AAC.02265-18.

  36. 36.

    Lysnyansky I, Ayling RD. Mycoplasma bovis: mechanisms of resistance and trends in antimicrobial susceptibility. Front Microbiol. 2016;7:595.

    PubMed  PubMed Central  Article  Google Scholar 

  37. 37.

    Ley DH. Mycoplasma gallisepticum infection in poultry. In: Merck Veterinary Manual. Merck Sharp & Dohme Corp. 2016. https://www.merckvetmanual.com/poultry/mycoplasmosis/mycoplasma-gallisepticum-infection-in-poultry#v3342225. Accessed 02 Jan 2019.

  38. 38.

    Waites KB, Duffy LB, Bebear CM, Matlow A, Talkington DF, Kenny GE, et al. Standardized methods and quality control limits for agar and broth microdilution susceptibility testing of Mycoplasma pneumoniae, Mycoplasma hominis, and Ureaplasma urealyticum. J Clin Microbiol. 2012;50(11):3542–7.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  39. 39.

    Basak A, Abouelhassan Y, Zuo R, Yousaf H, Ding Y, Huigens RW. Antimicrobial peptide-inspired NH125 analogues: bacterial and fungal biofilm-eradicating agents and rapid killers of MRSA persisters. Org Biomol Chem. 2017;15(26):5503–12.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  40. 40.

    Huigens RW, Abouelhassan Y, Yang H. Phenazine antibiotic-inspired discovery of bacterial biofilm-eradicating agents. Chembiochem. 2019;20(23):2885–902.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  41. 41.

    Garrison AT, Abouelhassan Y, Norwood VM, Kallifidas D, Bai F, Nguyen MT, et al. Structure-activity relationships of a diverse class of halogenated phenazines that targets persistent, antibiotic-tolerant bacterial biofilms and Mycobacterium tuberculosis. J Med Chem. 2016;59(8):3808–25.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  42. 42.

    Pelletier C, Prognon P, Bourlioux P. Roles of divalent cations and pH in mechanism of action of nitroxoline against Escherichia coli strains. Antimicrob Agents Chemother. 1995;39(3):707–13.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  43. 43.

    Madsen ML, Nettleton D, Thacker EL, Minion FC. Transcriptional profiling of Mycoplasma hyopneumoniae during iron depletion using microarrays. Microbiology. 2006;152(Pt 4):937–44.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  44. 44.

    Basak A, Abouelhassan Y, Kim YS, Norwood VM, Jin S, Huigens RW. Halogenated quinolines bearing polar functionality at the 2-position: identification of new antibacterial agents with enhanced activity against Staphylococcus epidermidis. Eur J Med Chem. 2018;155:705–13.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  45. 45.

    Valentine-King M, Cisneros K, James M, Huigens R, Brown M: A TL1 team approach to evaluating novel antimicrobial compounds against mycoplasmas and their interaction with drug metabolizing enzymes. In: Translational Science 2018. Washington, D. C.; 2018.

  46. 46.

    Li L, Shen W, Zhang K, Tang X, Guo N, Shen F, et al. In-vitro antimycoplasmal activity of triclosan in combination with fluoroquinolones against five Mycoplasma species. Iran J Pharm Res. 2012;11(4):1111–9.

    CAS  PubMed  PubMed Central  Google Scholar 

  47. 47.

    Halden RU, Lindeman AE, Aiello AE, Andrews D, Arnold WA, Fair P, et al. The Florence statement on triclosan and triclocarban. Environ Health Perspect. 2017;125(6):064501.

    PubMed  PubMed Central  Article  Google Scholar 

  48. 48.

    Jackson EN, Rowland-Faux L, James MO, Wood CE. Administration of low dose triclosan to pregnant ewes results in placental uptake and reduced estradiol sulfotransferase activity in fetal liver and placenta. Toxicol Lett. 2018;294:116–21.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  49. 49.

    Chen H, Yu S, Hu M, Han X, Chen D, Qiu X, et al. Identification of biofilm formation by Mycoplasma gallisepticum. Vet Microbiol. 2012;161(1–2):96–103.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  50. 50.

    Abouelhassan Y, Yang Q, Yousaf H, Nguyen MT, Rolfe M, Schultz GS, et al. Nitroxoline: a broad-spectrum biofilm-eradicating agent against pathogenic bacteria. Int J Antimicrob Agents. 2017;49(2):247–51.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  51. 51.

    Simmons WL, Bolland JR, Daubenspeck JM, Dybvig K. A stochastic mechanism for biofilm formation by Mycoplasma pulmonis. J Bacteriol. 2007;189(5):1905–13.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  52. 52.

    McAuliffe L, Ellis RJ, Miles K, Ayling RD, Nicholas RA. Biofilm formation by mycoplasma species and its role in environmental persistence and survival. Microbiology. 2006;152(Pt 4):913–22.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  53. 53.

    CLSI. Performance standards for antimicrobial susceptibility testing; twenty-second informational supplement. CLSI document M100-S22. Wayne, PA: Clinical and Laboratory Standards Institute; 2012.

  54. 54.

    Waites KB, Crabb DM, Bing X, Duffy LB. In vitro susceptibilities to and bactericidal activities of garenoxacin (BMS-284756) and other antimicrobial agents against human mycoplasmas and ureaplasmas. Antimicrob Agents Chemother. 2003;47(1):161–5.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

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Acknowledgements

We kindly thank Dina Michaels and Dan Brown for providing M. canis and M. gallisepticum type strains.

Funding

This work was supported by the National Institute of General Medical Sciences of the National Institutes of Health (R35 GM128621 to RH) and the National Center for Advancing Translational Sciences of the National Institutes of Health under University of Florida Clinical and Translational Science Awards (TL1 TR001428 and UL1 TR00142, to MV and KC). Funding agencies had no role in the study design, data collection or interpretation, or manuscript preparation.

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MV, KC, MJ, RH and MB all contributed to the conception of the research project. MB and MV designed the study. RH synthesized the compounds evaluated in this study. MV carried out the laboratory work, MV and KC interpreted the results, and MV drafted the manuscript. MB, MJ, and RH provided critical revisions of the manuscript. All authors have reviewed and approved it for final submission.

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Correspondence to Mary B. Brown.

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Valentine-King, M.A., Cisneros, K., James, M.O. et al. Efficacy data of halogenated phenazine and quinoline agents and an NH125 analogue to veterinary mycoplasmas. BMC Vet Res 16, 107 (2020). https://doi.org/10.1186/s12917-020-02324-4

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Keywords

  • Veterinary mycoplasmas
  • Drug evaluation
  • Quinoline
  • NH125 analogue
  • Phenazine
  • Nitroxoline