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Article

Phenotypic and Molecular Traits of Staphylococcus coagulans Associated with Canine Skin Infections in Portugal

by
Sofia Santos Costa
1,*,
Valéria Oliveira
1,
Maria Serrano
1,
Constança Pomba
2,3 and
Isabel Couto
1,*
1
Global Health and Tropical Medicine (GHTM), Instituto de Higiene e Medicina Tropical (IHMT), Universidade Nova de Lisboa (UNL), Rua da Junqueira 100, 1349-008 Lisboa, Portugal
2
Centre of Interdisciplinary Research in Animal Health (CIISA), Faculty of Veterinary Medicine, University of Lisbon, Avenida da Universidade Técnica, 1300-477 Lisboa, Portugal
3
GeneVet, Laboratório de Diagnóstico Molecular Veterinário, Rua Quinta da Nora Loja 3B, 2790-140 Carnaxide, Portugal
*
Authors to whom correspondence should be addressed.
Antibiotics 2021, 10(5), 518; https://doi.org/10.3390/antibiotics10050518
Submission received: 31 March 2021 / Revised: 20 April 2021 / Accepted: 24 April 2021 / Published: 2 May 2021
(This article belongs to the Special Issue Staphylococcus spp. in Animals: Resistance to Antimicrobials, Virulence and Genetic Lineages)
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Abstract

:
Staphylococcus coagulans is among the three most frequent pathogens of canine pyoderma. Yet, studies on this species are scarce. Twenty-seven S. coagulans and one S. schleiferi, corresponding to all pyoderma-related isolations from these two species at two veterinary laboratories in Lisbon, Portugal, between 1999 and 2018 (Lab 1) or 2018 (Lab 2), were analyzed. Isolates were identified by the analysis of the nuc gene and urease production. Antibiotic susceptibility towards 27 antibiotics was evaluated by disk diffusion. Fourteen antibiotic resistance genes were screened by PCR. Isolates were typed by SmaI-PFGE. Two S. coagulans isolates (2/27, 7.4%) were methicillin-resistant (MRSC, mecA+) and four (4/27, 14.8%) displayed a multidrug-resistant (MDR) phenotype. We observed resistance to penicillin (17/27, 63.0%), fluoroquinolones (11/27, 40.7%), erythromycin and clindamycin (3/27, 11.1%), fusidic acid (3/27, 11.1%) and tetracycline (1/27, 3.7%). The blaZ and erm(B) genes were carried by 16 and 1 isolates resistant to penicillin and erythromycin/clindamycin, respectively. Only three S. coagulans carried plasmids. The single S. schleiferi isolate presented an MDR phenotype. SmaI-PFGE revealed a limited genetic diversity of S. coagulans, with a predominant lineage present from 2001 to 2018. This study describes the first MRSC causing canine infection in Portugal and reveals a high burden of antimicrobial resistance, with the emergence of MDR phenotypes within the main lineages.

1. Introduction

Pyoderma is a common skin infection in dogs and the main cause for antimicrobial use in small animal veterinary medicine [1]. Coagulase-positive staphylococci are the main pathogenic agents of canine pyoderma; Staphylococcus pseudintermedius accounts for up to 90% of pyoderma-related staphylococcal infections, followed by Staphylococcus coagulans (previously known as Staphylococcus schleiferi subsp. coagulans) and Staphylococcus aureus [1,2,3]. Coagulase-negative staphylococci, like Staphylococcus epidermidis, are rare agents of canine pyoderma, frequently in association with S. pseudintermedius [1].
The species S. schleiferi was first described in 1988 by Freney and colleagues in human clinical isolates [4], and later reported as a member of the human axilla microflora [5,6]. In 1990, Igimi and colleagues identified several isolates of S. schleiferi from dogs with otitis externa that presented distinct characteristics from the S. schleiferi isolated from humans, leading to the proposal of a new subspecies denominated S. schleiferi subsp. coagulans [7]. S. schleiferi subsp. coagulans differed from S. schleiferi subsp. schleiferi, among other traits, by the production of the enzymes coagulase and urease [7]. In 2020, a phylogenomic analysis of the Staphylococcus genus led to the re-classification of S. schleiferi subsp. coagulans as the new species S. coagulans and of S. schleiferi subsp. schleiferi as S. schleiferi [8].
S. coagulans is part of the dog skin microflora; it has been isolated from the skin [9] and ear canal of healthy dogs [10], although its presence may be registered in low numbers [11]. This species has also been isolated from the skin of healthy cats [12] and, more recently, from mouth samples of healthy seals [13]. S. coagulans is an opportunistic pathogen. The first case of skin infection caused by S. coagulans was reported by Bes and colleagues in 2002 [14]. Since then, this species has been associated with skin, ear or urinary infections in dogs, many of which are recurrent [10,15,16,17,18,19]. Albeit rare, there have been reports of human opportunistic infections caused by S. coagulans [20,21,22,23,24], some of which are potentially linked to cases of dog-to-human transmission of S. coagulans strains [22,23,24].
Antimicrobial resistance is a frequent trait of staphylococci and increasing rates of antimicrobial resistance have been documented in major animal staphylococcal pathogens, such as S. pseudintermedius and S. aureus [25]. For S. coagulans, there are a limited number of reports on the rate of antimicrobial resistance worldwide. The first methicillin-resistant S. coagulans (MRSC) isolates were identified in the US in 2003 [15]. These MRSC isolates, resistant to all beta-lactam antibiotics except fifth-generation cephalosporins, were linked to recurrent cases of canine pyoderma [15]. Since then, several US-based studies have indicated frequency rates of MRSC from 0% [26] up to 75%, mainly associated with cases of recurrent skin or ear infections in dogs, many of which subjected to previous antibiotic therapy [15,27,28,29,30,31,32,33]. In fact, previous treatment with penicillin or a cephalosporin has been reported as a risk factor for the emergence of MRSC [34]. Studies conducted from other geographic regions have also shown a variability in frequency rates of MRSC isolates linked to skin, ear or urinary infections, from 0% in Slovenia [35], the UK [16], Scotland [36], Italy [37] Portugal [38], Australia [39] and Japan [10] to rates of 12.5–20% in Brazil [17,40], 24% in Korea [41], ca. 30% in Japan [18,42] and 70% in Thailand [43]. However, the MRSC frequency rates determined for some of these studies may not be precise, due to the low number of isolates studied, lack of differentiation between S. schleiferi subspecies and, most importantly, absence of clinical breakpoints for the detection of methicillin resistance in these species, which were only recommended by CLSI from 2018 onwards [44]. Resistance to other antibiotic classes has also been reported, associated or not to methicillin-resistance, and usually includes resistance to fluoroquinolones [37,45], penicillin, erythromycin, clindamycin, gentamicin, chloramphenicol, tetracycline and fusidic acid [10,18,19,29,30,32,34,39,43]. Despite the low prevalence of S. coagulans, and consequently, of the absolute numbers of strains analyzed, an increasing trend of antimicrobial resistance has been reported for this species [33,46], which may affect the management of infections caused by S. coagulans.
In a previous study conducted in Portugal, S. coagulans and S. schleiferi were associated with over 11% of skin, ear and urinary infections in pets during a 16-year period (1999–2014) in a veterinary research laboratory receiving samples from a veterinary teaching hospital and private practices in Lisbon area [38]. Although no MRSC isolates were detected in that earlier study, an increasing trend of antimicrobial resistance burden was observed for S. coagulans during the 16-year timeframe [38]. In the present work, we expand that previous study, focusing on all the S. coagulans and S. schleiferi associated with skin infections, isolated from 1999 to 2018, as well as all S. coagulans and S. schleiferi related to skin infections and collected during 2018 at a second private veterinary diagnostic laboratory. The aims of our study were to analyze the antimicrobial resistance burden of these pathogens and their association with genotypic determinants of resistance, plasmid content and molecular lineages; the latter two traits have not been studied yet in Portugal and have been rarely documented worldwide.

2. Results

2.1. Identification of S. coagulans and S. schleiferi Isolates

The identification of S. coagulans and S. schleiferi isolates among an initial collection of 89 pyoderma-related Staphylococcus isolates was performed or confirmed by the species-specific nuc-PCR strategy proposed by Sasaki and colleagues [47], followed by detection of urease activity [44]. Of the 89 isolates screened, 28 were identified as S. coagulans or S. schleiferi by the nuc-PCR. Of these, 27 were urease-positive and thus identified as S. coagulans, whereas one isolate was urease-negative and identified as S. schleiferi. All isolates were collected from dogs and linked to pyoderma; two S. coagulans isolates were collected from the same dog, corresponding to skin swabs sampled one year apart. In sum, the study collection comprised 27 S. coagulans isolates; 21 collected over 19 years in a veterinary research lab (Lab 1), 7 collected during 2018 at a veterinary diagnostic lab (Lab 2) and a single S. schleiferi isolate collected at Lab 1 in 2016.

2.2. Antimicrobial Resistance Profiles and Association with Resistance Determinants

The antibiotic susceptibility profiles of all S. coagulans isolates are discriminated in Table 1 and Figure 1. Inhibition zone diameters for all antibiotics studied are shown in Tables S1–S3 of the Supplementary Materials.
Antibiotic susceptibility testing showed that of the 27 isolates in study, 16 (16/27, 59.3%) were resistant to one or two antibiotics of distinct classes and 4 (4/27, 14.8%) displayed a multidrug resistance phenotype, showing resistance to, at least, three different classes of antibiotics. Only seven (7/27, 25.9%) were susceptible to all antibiotics tested. Two S. coagulans isolates (2/27, 7.4%) were resistant to oxacillin and carried the mecA gene, being classified as MRSC, and thus, resistant to all beta-lactams, except for fifth-generation cephalosporins. The mecA gene was not detected in the remaining isolates.
The most common resistance pattern for S. coagulans was monoresistance to penicillin, observed in six isolates (6/27, 22.2%), followed by resistance to penicillin and fluoroquinolones (5/27, 18.5%). The MDR isolates were characterized by resistance to penicillin, fluoroquinolones and fusidic acid (1 out of 4 isolates), or penicillin, erythromycin and clindamycin (2 out of 4 isolates), and additional resistance to fluoroquinolones and tetracycline (1 out of 4 isolates). The two MRSC isolates also showed resistance to fluoroquinolones.
Resistance to penicillin was the most frequently observed phenotype, detected in 17 S. coagulans (17/27, 63.0%). Of these, one isolate presented a zone inhibition diameter (ZD) of 31 mm but showed a sharp inhibition border, being considered a beta-lactamase producer and penicillin-resistant. Another isolate showed an ZD of 33 mm and a fuzzy border but carried the mecA, and thus, was also considered resistant to penicillin [48]. The blaZ gene encoding the beta-lactamase BlaZ was present in 16 of the 17 penicillin-resistant isolates.
Resistance to fluoroquinolones was observed in 11 out of the 27 S. coagulans isolates (11/27, 40.7%). These 11 isolates were resistant (n = 9) or intermediate (n = 2) to enrofloxacin; 10 (37.0%) were resistant (n = 6) or intermediate (n = 4) to ciprofloxacin; and 6 (22.2%) were resistant (n = 4) or intermediate (n = 2) to moxifloxacin. Sequencing the quinolone-resistance determining region (QRDR) of the grlA and gyrA genes of the 11 isolates presenting fluoroquinolone resistance revealed six distinct patterns of mutations in GrlA and GyrA (Figure 1). The pair GrlA: S80I/GyrA:S80F, observed in four isolates, was the only associated with a resistance phenotype to the three fluoroquinolones tested. On the other hand, the single GrlA mutation S80R was present in one isolate with intermediate phenotype only towards enrofloxacin. The remaining mutation patterns GrlA:S80I/GyrA:E88A, GrlA:S80R/GyrA:S80F, GlA:S80R/GyrA:E88G and GrlA:S80G/GyrA:S80Y were all linked to resistance or intermediate to either ciprofloxacin or enrofloxacin.
Resistance to erythromycin was detected in three S. coagulans isolates (3/27, 11.1%), two of which were intermediate. These three isolates showed also constitutive resistance to clindamycin (3/27, 11.1%). From the seven macrolide-lincosamide resistance genes screened, only erm(B) was detected in the single isolate classified as resistant to both erythromycin and clindamycin. No resistance gene was detected for the remaining two isolates resistant to clindamycin and intermediate to erythromycin.
Resistance to fusidic acid was detected in two S. coagulans isolates (2/27, 7.4%) and to tetracycline in a single isolate (1/27, 3.7%), but none of these isolates harbored any of the resistance determinants screened, fusB/fusC or tetK/tetM/tetL, respectively.
The single S. schleiferi isolate of this collection presented an MDR phenotype, with resistance to penicillin, fluoroquinolones and fusidic acid, and harbored the blaZ gene and the QRDR mutations GrlA:S80R and GyrA:S80F. Neither of the fusidic acid resistance genes screened, fusB/fusC, were detected in this isolate.
None of the S. coagulans or S. schleiferi isolates were resistant to chloramphenicol, quinupristin-dalfopristin, trimethoprim-sulfamethoxazole, linezolid, rifampicin, minocycline, tigecycline nor to the aminoglycosides gentamicin, tobramycin, kanamycin or amikacin.

2.3. Distributions of Zone Inhibition Diameters for Antibiotics with No Breakpoints Established

One of the aims of this study was to evaluate the overall burden of antimicrobial resistance in S. coagulans to a wide set of antibiotics for multiple classes, independently of their recommended use for canine skin infections [1,2]. This evaluation is impaired by the limited number of breakpoints recommended for S. coagulans/S. schleiferi by Clinical Laboratory and Standards Institute (CLSI) or European Committee on Antimicrobial Susceptibility Testing (EUCAST). For most antibiotics, the recommendation is to use breakpoints established for Staphylococcus spp. isolated from humans [48] and/or established for S. aureus [50]. To overcome this limitation, we estimated the ZD-based cut-off value (COWT) of S. coagulans for antibiotics with no breakpoints available. This parameter corresponds to the smallest ZD value of the wild-type population (the population without phenotypically expressed resistance mechanisms) [51]. It also allows the detection of putative non-wild type populations (with phenotypically expressed resistance mechanisms) in a given bacterial collection. Thus, the distributions of zone inhibition diameters were analyzed to evaluate the possible presence of resistance determinants in S. coagulans for the antibiotics mupirocin, florfenicol, neomycin, bacitracin, novobiocin and apramycin (Figure 2). This analysis only took into consideration the 27 isolates identified as S. coagulans.
The Normalized Resistance Interpretation (NRI) method was used to estimate the distribution of the putative wild-type (WT) population and calculate the COWT value for this population. All zone diameter distributions were unimodal. The normalized distributions of the WT populations were validated as they all included over 15 observations and each associated standard deviation (SD) was below the acceptable SD upper limit of 3.38 mm (Table 2). The application of the estimated COWT values showed the absence of NWT populations of S. coagulans towards all the six antibiotics tested, indicating the absence of isolates with resistance mechanisms to these antibiotics in our collection.

2.4. Plasmid Profiling and Association with Antibiotic Resistance

Plasmid DNA was isolated for all isolates. From the 27 S. coagulans studied, only 3 (3/27, 11.1%) carried plasmids. Two isolates showed a single plasmid of ≥23 kb, whereas the remaining S. coagulans presented a single plasmid of ≤3 kb. Of the two isolates harboring a large plasmid, one showed resistance to penicillin and carried the blaZ gene, while the other was only resistant to fusidic acid with no associated resistance determinant detected. The isolate harboring the small plasmid showed resistance to penicillin and the blaZ gene as well as an intermediate phenotype towards enrofloxacin.

2.5. Molecular Typing and Association with Antimicrobial Resistance Phenotypes

All isolates, but one, were subjected to molecular typing by SmaI-PFGE (Figure 1). The collection comprised nine pulsed-field gel electrophoresis (PFGE) types, classified A to I, and thirteen subtypes. The PFGE type A was the most common, represented by over half of the S. coagulans isolates (14/27, 51.8%) and comprising eight subtypes. PFGE types F and G each included three isolates (3/27, 11.1%) and comprised three and two subtypes, respectively. The remaining six PFGE types were represented by a single isolate. The single S. schleiferi isolate presented a PFGE pattern indistinguishable from S. coagulans, sharing the PFGE type A1 together with two S. coagulans isolates. The two S. coagulans isolates collected one year apart from the same dog belonged to different subtypes of PFGE type F. A calculation of the Simpson’s Index of Diversity (SID) based on the S. coagulans PFGE types revealed that this collection is not very diverse (SID = 0.70, CI: 0.51–0.89).
The main PFGE type A was present in isolates collected from 2001 to 2018. All isolates with this PFGE pattern showed resistance to at least one antibiotic. Additionally, all four MDR isolates belonged to PFGE type A. The two MRSC isolates belonged to two distinct and unique PFGE types (D and E). We observed an increase in antimicrobial resistance accompanying the year of isolation of the S. coagulans isolates, detectable within the main PFGE types. For example, up to 2014, isolates from PFGE type A (n = 7) presented monoresistance to penicillin (n = 3) with additional resistance to fluoroquinolones (n = 2) or macrolides-lincosamides (n = 2, MDR). However, from 2015 to 2018, the remaining isolates with PFGE type A (n = 7) presented more diverse and additional resistance phenotypes, namely resistance to penicillin-fluoroquinolones-fusidic acid (n = 1, MDR) or resistance to penicillin-fluoroquinolones-macrolides-lincosamides-tetracycline (n = 1, MDR), besides the patterns previously detected (monoresistance to penicillin, n = 2 or resistance to penicillin-fluoroquinolones, n = 3). Within PFGE type F, the emergence of resistance to fluoroquinolones was detectable in the two isolates collected in 2015/2016, whereas for PFGE type G, resistance to fusidic acid was detected in the 2018 isolate.
The increasing antimicrobial resistance was also illustrated by the detection of the two MRSC isolates in 2018, belonging to PFGE types D and E.

3. Discussion

Despite being a relevant agent of canine pyoderma, S. coagulans is still poorly characterized regarding antimicrobial resistance traits and, particularly, its circulating clonal lineages. A previous study in Portugal surveyed the antimicrobial resistance burden of S. coagulans associated with several types of infection during a 16-year period (1999–2014). During that timeframe, no MRSC isolates were detected, but MDR phenotypes were observed [38]. In this work, we expanded the collection to encompass the years 2015 up to 2018; additionally, we included all isolates collected during 2018 at a second veterinary diagnostic laboratory. We also broadened the analysis to plasmid profiling and molecular typing. However, we focused our study on isolates related to skin infections.
This study revealed that a significant proportion of all the non-S. pseudintermedius or non-S. aureus isolates collected from companion animals skin infections during the time period studied was identified as S. coagulans (27/89, 30.3%), while a single isolate (1/89, 1.1%) corresponded to S. schleiferi. The low total number of S. coagulans or S. schleiferi isolates collected during this 19-year period (1999–2018) reflects the lower rate of canine skin infections caused by these pathogens when compared to S. pseudintermedius [3]. Several studies have shown that S. coagulans is commonly the second most isolated staphylococci isolated from skin samples of canine pyoderma, in frequencies varying from 3% [32,52] to up to 10% [18]. The predominance of S. coagulans over S. schleiferi in canine skin samples observed in our study agrees with other studies [31,32], although some works documented similar or higher frequency of S. schleiferi in canine pyoderma [53,54].
We registered a high rate of antimicrobial resistance in the collection studied. In total, 75% of the isolates (21/28, considering S. coagulans and S. schleiferi) were resistant to at least one antibiotic and 17.9% (5/28) were MDR. This study also reports the first MRSC isolates in dogs in Portugal. A comparison of the antimicrobial resistance in the S. coagulans isolated between the 1999–2014 period (13 isolates obtained during the study by Couto and colleagues [38]) with the isolates collected afterward (2015–2018, n = 14) revealed an increase in the antimicrobial-resistant isolates. This was manifested by the decrease in the total number of fully-susceptible isolates (n = 5 in 1999–2014 to n = 2 in 2015–2018) and the increase in total number of isolates resistant to one or two classes of antibiotics (n = 6 in 1999–2014 to n = 10 in 2015–2018). Most importantly, we reported the emergence of two MRSC isolates from distinct lineages (different PFGE types) in the last year surveyed (2018). We also describe the emergence, since 2016, of resistance to fusidic acid, which is widely used in the topical treatment of human and canine skin infection caused by either S. coagulans or S. schleiferi. Worryingly, this increase in antimicrobial resistance in S. coagulans has also been reported in other countries, namely in the US [32,33,55]. The frequency rates of MRSC and MDR detected in our study are higher than the ones previously reported for other European countries [16,35,36,37], although there is a lack of recent surveys for direct comparison purposes.
The two MRSC isolates described in this study were also resistant to fluoroquinolones, as observed in other studies [30]. Nearly half of the S. coagulans studied were resistant to fluoroquinolones, and all carried QRDR mutations in a diverse range of combinations. High levels of resistance to fluoroquinolones have been reported worldwide in S. coagulans collected from dogs, irrespective of methicillin-resistance status, including in the UK [16], Italy [37], Japan [18] and the US [19]. The description of QRDR mutations in S. coagulans is sparce. A study by Intorre and colleagues identified the mutations GrlA: S80R or GyrA: E88G in S. coagulans resistant to old generation fluoroquinolones (enrofloxacin, ciprofloxacin and orbifloxacin) yet susceptible to moxifloxacin, gatifloxacin and trovafloxacin [45]. In the present study, we identified a wider set of QRDR mutations. Among the six different patterns of mutations identified, only the combination GrlA:S80I and GyrA:S80F was linked to resistance to the three fluoroquinolones tested, whereas a single mutation in GrlA (S80R) was associated with an intermediate phenotype towards enrofloxacin.
In the last decades, a decrease has been observed in the susceptibility to penicillin, erythromycin, clindamycin and to a lesser extent gentamicin or other aminoglycosides and tetracycline in S. coagulans, but the resistance determinants associated with these resistance phenotypes is scarcely documented [10,18,19,36,41,42,43]. As observed in other studies, resistance to penicillin was linked to the presence of the blaZ gene, encoding the beta-lactamase BlaZ, except for one MRSC isolate which did not carry this determinant. Contrary to other staphylococci, blaZ carriage was not associated with large multiresistance plasmids. Resistance to macrolides and lincosamides is common in S. coagulans and has been linked to the presence of erm(B) and/or erm(C) genes [41,42,43]. In our collection, only one out of the three isolates resistant to these antibiotics harbored the erm(B). Although negative for the other six resistance genes screened [erm(A), erm(C), msrA, mph(C), vga(A) and vga(C)], the remaining two resistant isolates could carry other determinants, such as additional erm genes like erm(43) or lnu(B), which are not usually linked to plasmids [56]. Resistance to fusidic acid was detected in three S. coagulans and S. schleiferi collected from 2016 onwards, highlighting the recent emergence of resistance to this antibiotic. However, none carried the two resistance determinants screened, fusB/fusC, which are usually associated with plasmids or other mobile genetic elements. Resistance to this antibiotic could be linked to mutations occurring in the fusA gene, which are common in other staphylococcal species [56]. Regarding resistance to tetracycline, none of the tet genes screened was found in the single tetracycline-resistant S. coagulans detected. However, this isolate could carry the tet(O) determinant, as observed in the study by Chanchaithong and colleagues [43].
Despite the increase registered in antimicrobial resistance in S. coagulans in Portugal in the last two decades, resistance phenotypes are still mainly restricted to a few antibiotic classes, namely beta-lactams, fluoroquinolones, macrolide-lincosamides and fusidic acid. Reports from other countries such as Thailand [43] showed a higher diversity of resistance phenotypes and resistance determinants in S. coagulans. The low diversity of resistance genes encountered in our collection could be associated with the low abundance of plasmids.
Our knowledge on the molecular epidemiology of S. coagulans is rather limited to a few studies with a limited number of isolates. These have used SmaI-PFGE to evaluate the clonality of this species, indicating a high clonality within the species and that S. coagulans and S. schleiferi often present indistinguishable PFGE patterns [10,19,29,33,43]. Our data also show that S. coagulans collected in Portugal (Lisbon area) throughout the last two decades present a low genetic diversity (Simpson’s index of diversity, SID = 0.70), with a predominant lineage encompassing over half of the isolates collected through almost the entire time span of the collection. Nevertheless, some heterogeneity was found within this predominant lineage, with isolates varying in resistance phenotypes and resistance determinants.
We also analyzed the ZD distributions and corresponding COWT values for six antibiotics (apramycin, bacitracin, florfenicol, mupirocin, neomycin and novobiocin) with no breakpoints available for S. coagulans. These antibiotics are not used or rarely recommended (mupirocin) for the treatment of skin infections in dogs [1,2]. Nevertheless, the emergence and dissemination of resistance to these antibiotics in several staphylococci of animal origin is worrisome [56]. Thus, the availability of cut-off values that allow the identification of isolates potentially harboring resistance mechanisms to these antibiotics could be a valuable tool in future antimicrobial resistance surveillance studies in S. coagulans.
The results gathered in this study are particularly worrisome when analyzed in conjunction with data on the classes of antibiotics most prescribed in small animal practice. Data from the European Medicines Agency (EMA) and a report by Oliveira and colleagues highlight that beta-lactams, fluoroquinolones, macrolides and tetracyclines represent the majority of antibiotics prescribed for treatment of skin infections in small animals [57,58]. Although fusidic acid is not listed in these two studies, it is recommended for the topical management of canine pyoderma [1,2] and, worryingly, is frequently used (for human or animal use) without requiring medical prescription. Our data suggest that the high burden of antimicrobial resistance in S. coagulans may reflect the usage of antibiotics recommended for the treatment of canine pyoderma.

4. Materials and Methods

4.1. Bacterial Isolates

The initial collection studied (total n = 89) included all isolates previously identified as S. schleiferi or Staphylococcus spp. (non-S. pseudintermedius and non-S. aureus) causing skin infections in pets collected over 19 years (1999–2018) at a veterinary research laboratory providing diagnostic services for a veterinary teaching hospital and private veterinary clinics in the Lisbon area (Lab 1, n = 40) and at a private veterinary diagnostic clinic during 2018 (Lab 2, n = 49) (Table 3). This collection included thirteen isolates collected from 1999 to 2014 at Lab 1 and previously identified as S. schleiferi that were partially characterized in a previous study [38]. The type strains S. coagulans DSM 6628T and S. schleiferi DSM 4807T were acquired from DSMZ GmbH (Germany) and included in the study as controls. All isolates were grown in tryptone soya broth or agar (TSB/TSA, Thermo Scientific™ Oxoid™, Basingstoke, UK) at 37 °C, at 180 rpm (for broth cultures). Bacterial stocks were kept at −80 °C in TSB supplemented with 10% (v/v) glycerol.

4.2. Total DNA and Plasmid DNA Isolation

Total DNA was isolated by the boiling method [59] and used as a template for all PCR protocols. Plasmid DNA was isolated with NZYMiniprep Kit (NZYTech, Lisbon, Portugal), according to the manufacturer’s recommendations and with the addition of an incubation step with lysostaphin at 35 mg/L for 60 min at 37 °C following resuspension of the bacterial pellet with buffer A1. All plasmid preparations were analyzed in 1% agarose gel electrophoresis in TAE 1X buffer at 80 V for 90 min using the molecular ladder lambda/HindIII (Thermo Scientific™).

4.3. Identification of the Isolates

The identification of the isolates as S. coagulans or S. schleiferi was confirmed by a species-specific nuc PCR approach described by Sasaki et al. [47], after decreasing the annealing temperature from 56 °C to 50 °C, to obtain a good specific amplification for the two type strains used as positive controls. Total DNA from the type or reference strains S. pseudintermedius DSM 21284T (DSMZ GmbH), S. aureus ATCC® 259323™ and S. epidermidis ATCC® 12228™ (LGC Standards, S.L.U, Barcelona, Spain) were included as negative controls. The differentiation between S. coagulans and S. schleiferi was carried out, for each isolate, by detection of urease activity after growth in Christensen urea agar at 35 °C for up to 48 h [44]. Conversion of the medium color from yellow to pink indicates the presence of urease activity. The urease-negative strains S. schleiferi DSM 4807T and Escherichia coli ATCC® 2922™, and the urease-positive strains S. coagulans DSM 6628T and Klebsiella pneumoniae ATCC® BAA 1706™ were included as controls.

4.4. Antibiotic Susceptibility Testing

Antibiotic susceptibility was determined by agar disk diffusion on Mueller-Hinton agar plates (Thermo Scientific™ Oxoid™) according to CLSI recommendations for bacteria isolated from animals [48] or EUCAST recommendations [50]. We studied a wide panel of antibiotics, not only used in veterinary practice, but also human medicine, to evaluate the overall burden of antimicrobial resistance in S. coagulans. Antibiotic disks were acquired from Thermo Scientific™ Oxoid™ or MAST Group (pradofloxacin) (Liverpool, UK). Susceptibility profiles were interpreted according to CLSI VET01S-ED5 recommendations for enrofloxacin (5 μg), clindamycin (2 μg) and tetracycline (30 μg) [48] or according to CLSI M100-S30 (bacteria isolated from humans) for penicillin (10 U), oxacillin (1 μg), ciprofloxacin (5 μg), moxifloxacin (5 μg), gentamicin (10 μg), erythromycin (15 μg), minocycline (30 μg), trimethoprim/sulfamethoxazole (1.25/23.75 μg), chloramphenicol (30 μg), linezolid (30 μg), rifampicin (5 μg) [49]; or according to EUCAST for tobramycin (10 μg), kanamycin (30 μg), amikacin (30 μg), quinupristin-dalfopristin (15 μg), fusidic acid (10 μg) and tigecycline (15 μg) [50]. Other antibiotics were tested for which no breakpoints are established, namely pradofloxacin (5 μg), neomycin (30 μg), apramycin (15 μg), florfenicol (30 μg), novobiocin (30 μg), mupirocin (200 μg) and bacitracin (10 U). Isolates categorized as intermediate using the CLSI breakpoints were considered resistant, according to these recommendations. The D-zone test was performed for detection of inducible clindamycin resistance [49]. The reference strains S. aureus ATCC®25923™ and S. aureus ATCC®29213™ and the type strains S. coagulans DSM 6628T and S. schleiferi DSM 4807T were used as quality controls. Multidrug resistance (MDR) was considered as not-susceptibility to, at least, one agent of, at least, three classes of antimicrobials [60].

4.5. Calculation of Cut-Off (COWT) Values

The ZD-based COWT values were estimated using the Normalized Resistance Interpretation (NRI) method [51,61]. This method uses the distributions of inhibition zone diameters to make a least-square regression analysis to determine the putative wild-type (WT) population, the mean inhibition zone diameter and the associated standard deviation (SD) for each species-antimicrobial agent combination. The COWT corresponds to the smallest inhibition zone diameter presented by the putative WT population and is calculated at 2.5X the SD above the mean value and rounded up to the lowest absolute value [51,61]. Thus, the COWT allows the distinction between putative WT populations (devoid of phenotypically-detectable acquired resistance mechanisms) and non-wild-type populations (NWT, with phenotypically-detectable acquired resistance mechanisms) [62]. The COWT estimated by the NRI method will include 99.4% of the WT population [61]. The NRI method was used with permission from the patent holder, Bioscand AB, TÄBY, Sweden (European patent No 1383913, US Patent No. 7,465,559). The automatic and manual excel programs were made available through courtesy by P. Smith, W. Finnegan and G. Kronvall at http://www.bioscand.se/nri/ (accessed on 2 December 2020).

4.6. Screening of Resistance Determinants

Carriage of the beta-lactam resistance genes blaZ and mecA was screened by PCR for all isolates, whereas the genes erm(A), erm(B), erm(C), msrA, mph(C), vga(A) and vga(C) for resistance to macrolides and/or lincosamides, genes tet(K), tet(L), tet(M) for resistance to tetracyclines and genes fusB and fusC for resistance to fusidic acid were only screened by PCR for isolates a resistant or intermediate phenotype. The presence of mutations associated with fluroquinolone resistance was screened by sequencing of the quinolone-resistance determining region (QRDR) of the genes grlA and gyrA. Amplification products were purified using the kit NZYGelpure (NZYTech, Lisboa, Portugal) and sequenced. Sequences were analyzed using the programs SnapGene Viewer (GSL Biotech; available at snapgene.com), translated to polypeptide sequnces, aligned in MEGA v. 7.0.26 and compared against the GrlA and GyrA sequences of the type strain S. coagulans DSM6628T (GenBank assembly accession no. GCA_002901995.1). All primers used for the detection of resistance genes or mutations are listed in Supplementary Table S4, while the strains used as controls for PCR assays are discriminated in Supplementary Table S5.

4.7. Molecular Typing by SmaI-PFGE

All isolates in study were subjected to SmaI-PFGE typing. Briefly, agarose disks containing genomic DNA were prepared and restricted with SmaI, as previously described for S. aureus [63]. Restriction fragments were then resolved by PFGE in a contour-clamped homogeneous electric field (CHEF) apparatus (CHEF-DRIII, Bio-Rad, Hercules, CA, USA), using the following running parameters: 14 °C, 200 V (6 V/cm), 120°, 5 s of initial switch, 40 s of final switch and 21 h of running time [19]. In each run, control agarose disks were included containing the genomic DNA of the reference strain S. aureus NCTC8325 (used for gel normalization) and the PFG DNA Ladder (New England Biolabs). Macrorestriction profiles were analyzed with BioNumerics software version 7.6 (Applied Maths, Kortrijk, Belgium) using the unweighted pair group method using arithmetic averages and the Dice similarities coefficient. Band position tolerance and optimization were set at 1% and 0.5%, respectively. Isolates with a similarity coefficient ≥ 81% were considered as belonging to the same PFGE type, whereas isolates with a similarity coefficient ≥ 97% were considered as belonging to the same PFGE sub-type [64]. The genetic diversity of the collection was calculated, based on PFGE types, by Simpson’s index of diversity with a confidence interval of 95% [65].

5. Conclusions

This study on S. coagulans associated with canine pyoderma highlights a high burden of antimicrobial resistance in S. coagulans in Portugal during the last two decades, including the emergence of MRSC. This work also reveals a low genetic diversity and a low content of plasmids in the circulating S. coagulans. Yet, new lineages with relevant resistance phenotypes were identified. This scenario may have a high impact on the future management of canine pyoderma caused by S. coagulans.

Supplementary Materials

The following are available online at https://www.mdpi.com/article/10.3390/antibiotics10050518/s1, Table S1: Distribution of inhibition zone diameters of 21 antibiotics for the 27 S. coagulans studied; Table S2: Distribution of inhibition zone diameters of six antibiotics with no breakpoint or epidemiological cut-off value for the 27 S. coagulans studied; Table S3: Inhibition zone diameters of 27 antibiotics for the single S. schleiferi isolate studied; Table S4: Primers used in this study; Table S5: Control strains used in the screening of antibiotic resistance genes.

Author Contributions

Conceptualization, S.S.C. and I.C.; Funding acquisition, S.S.C. and I.C.; Investigation, V.O., M.S. and S.S.C.; Methodology, S.S.C. and I.C.; Project administration I.C.; Resources, C.P. and I.C.; Supervision, S.S.C. and I.C.; Validation, S.S.C. and I.C.; Visualization, S.S.C.; Writing—original draft, S.S.C.; Writing—review and editing, S.S.C., V.O., M.S., C.P. and I.C. All authors have read and agreed to the published version of the manuscript.

Funding

This work was supported by Project BIOSAFE funded by FEDER through the Programa Operacional Factores de Competitividade—COMPETE, by the Fundação para a Ciência e a Tecnologia (FCT, Portugal)—Grant LISBOA-01-0145-FEDER-030713, PTDC/CAL-EST/30713/2017 and by FCT through funds to GHTM (UID/04413/2020) and the CIISA Project (UID/CVT/00276/2020).

Data Availability Statement

All relevant data have been provided in the paper. Raw data can also be provided by the authors upon reasonable request.

Conflicts of Interest

The authors declare no conflict of interest.

References

  1. Hillier, A.; Lloyd, D.H.; Weese, J.S.; Blondeau, J.M.; Boothe, D.; Breitschwerdt, E.; Guardabassi, L.; Papich, M.G.; Rankin, S.; Turnidge, J.D.; et al. Guidelines for the diagnosis and antimicrobial therapy of canine superficial bacterial folliculitis (Antimicrobial Guidelines Working Group of the International Society for Companion Animal Infectious Diseases). Vet. Dermatol. 2014, 25, 163-e43. [Google Scholar] [CrossRef] [PubMed]
  2. Morris, D.O.; Loeffler, A.; Davis, M.F.; Guardabassi, L.; Weese, J.S. Recommendations for approaches to meticillin-resistant staphylococcal infections of small animals: Diagnosis, therapeutic considerations and preventative measures: Clinical Consensus Guidelines of the World Association for Veterinary Dermatology. Vet. Dermatol. 2017, 28, 304-e69. [Google Scholar] [CrossRef]
  3. Loeffler, A.; Lloyd, D.H. What has changed in canine pyoderma? A narrative review. Vet. J. 2018, 235, 73–82. [Google Scholar] [CrossRef] [Green Version]
  4. Freney, J.; Brun, Y.; Bes, M.; Meugnier, H.; Grimont, F.; Grimont, P.; Nervi, C.; Fleurette, J. Staphylococcus lugdunensis sp. nov. and Staphylococcus schleiferi sp. nov., two species from human clinical specimens. Int. J. Syst. Bacteriol. 1988, 38, 168–172. [Google Scholar] [CrossRef]
  5. Célard, M.; Vandenesch, F.; Darbas, H.; Grando, J.; Jean-Pierre, H.; Kirkorian, G.; Etienne, J. Pacemaker infection caused by Staphylococcus schleiferi, a member of the human preaxillary flora: Four case reports. Clin. Infect. Dis. 1997, 24, 1014–1015. [Google Scholar] [CrossRef]
  6. Da Costa, A.; Lelièvre, H.; Pha, D.; Kirkorian, G.; Célard, M.; Chevalier, P.; Vandenesch, F.; Etienne, J.; Touboul, P. Role of the preaxillary flora in pacemaker infections. Circulation 1998, 97, 1791–1795. [Google Scholar] [CrossRef] [Green Version]
  7. Igimi, S.; Takahashi, E.; Mitsuoka, T. Staphylococcus schleiferi subsp. coagulans subsp. nov., isolated from the external auditory meatus of dogs with external ear otitis. Int. J. Syst. Bacteriol. 1990, 40, 409–411. [Google Scholar] [CrossRef] [Green Version]
  8. Madhaiyan, M.; Wirth, J.S.; Saravanan, V.S. Phylogenomic analyses of the Staphylococcaceae family suggest the reclassification of five species within the genus Staphylococcus as heterotypic synonyms, the promotion of five subspecies to novel species, the taxonomic reassignment of five Staphylococcus species to Mammaliicoccus gen. nov., and the formal assignment of Nosocomiicoccus to the family Staphylococcaceae. Int. J. Syst. Evol. Microbiol. 2020, 70, 5926–5936. [Google Scholar] [CrossRef] [PubMed]
  9. Griffeth, G.C.; Morris, D.O.; Abraham, J.L.; Shofer, F.S.; Rankin, S.C. Screening for skin carriage of methicillin-resistant coagulase-positive staphylococci and Staphylococcus schleiferi in dogs with healthy and inflamed skin. Vet. Dermatol. 2008, 19, 142–149. [Google Scholar] [CrossRef]
  10. Yamashita, K.; Shimizu, A.; Kawano, J.; Uchida, E.; Haruna, A.; Igimi, S. Isolation and characterization of staphylococci from external auditory meatus of dogs with or without otitis externa with special reference to Staphylococcus schleiferi subsp. coagulans isolates. J. Vet. Med. Sci. 2005, 67, 263–268. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  11. Hanselman, B.A.; Kruth, S.; Weese, J.S. Methicillin-resistant staphylococcal colonization in dogs entering a veterinary teaching hospital. Vet. Microbiol. 2008, 126, 277–281. [Google Scholar] [CrossRef] [PubMed]
  12. Abraham, J.L.; Morris, D.O.; Griffeth, G.C.; Shofer, F.S.; Rankin, S.C. Surveillance of healthy cats and cats with inflammatory skin disease for colonization of the skin by methicillin-resistant coagulase-positive staphylococci and Staphylococcus schleiferi ssp. schleiferi. Vet. Dermatol. 2007, 18, 252–259. [Google Scholar] [CrossRef]
  13. Foster, G.; Robb, A.; Paterson, G.K. Isolation and genome sequencing of Staphylococcus schleiferi subspecies coagulans from Antarctic and North Sea seals. Access Microbiol. 2020, 2, acmi000162. [Google Scholar] [CrossRef] [PubMed]
  14. Bes, M.; Freney, J.; Etienne, J.; Guerin-Faublee, V. Isolation of Staphylococcus schleiferi subspecies coagulans from two cases of canine pyoderma. Vet. Rec. 2002, 150, 487–488. [Google Scholar] [CrossRef] [PubMed]
  15. Frank, L.A.; Kania, S.A.; Hnilica, K.A.; Wilkes, R.P.; Bemis, D.A. Isolation of Staphylococcus schleiferi from dogs with pyoderma. J. Am. Vet. Med. Assoc. 2003, 222, 451–454. [Google Scholar] [CrossRef]
  16. Rich, M.; Roberts, L.; Jones, M.; Young, V. Staphylococcus schleiferi subspecies coagulans in companion animals. Vet. Rec. 2007, 161, 107. [Google Scholar] [CrossRef]
  17. Penna, B.; Varges, R.; Martins, R.; Martins, G.; Lilenbaum, W. In vitro antimicrobial resistance of staphylococci isolated from canine urinary tract infection. Can. Vet. J. 2010, 51, 738–742. [Google Scholar]
  18. Kawakami, T.; Shibata, S.; Murayama, N.; Nagathifuji, K.; Iwasaki, T.; Fukata, T. Antimicrobial susceptibility and methicillin resistance in Staphylococcus pseudintermedius and Staphylococcus schleiferi subsp. coagulans isolated from dogs with pyoderma in Japan. J. Vet. Med. Sci. 2010, 72, 1615–1619. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  19. Cain, C.; Morris, D.; O’Shea, K.; Rankin, S. Genotypic relatedness and phenotypic characterization of Staphylococcus schleiferi subspecies in clinical samples from dogs. Am. J. Vet. Res. 2011, 72, 96–102. [Google Scholar] [CrossRef]
  20. Kumar, D.; Cawley, J.; Irizarry-Alvarado, J.; Alvarez, A.; Alvarez, S. Case of Staphylococcus schleiferi subspecies coagulans endocarditis and metastatic infection in an immune compromised host. Transpl. Infect. Dis. 2007, 9, 336–338. [Google Scholar] [CrossRef]
  21. Thibodeau, E.; Boucher, H.; DeNofrio, D.; Pham, D.; Snydman, D. First report of a left ventricular assist device infection caused by Staphylococcus schleiferi subspecies coagulans: A coagulase-positive organism. Diagn. Microbiol. Infect. Dis. 2012, 74, 68–69. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  22. Tzamalis, A.; Chalvatzis, N.; Anastasopoulos, E.; Tzetzi, D.; Dimitrakos, S. Acute postoperative Staphylococcus schleiferi endophthalmitis following uncomplicated cataract surgery: First report in the literature. Eur. J. Ophthalmol. 2013, 23, 427–430. [Google Scholar] [CrossRef] [PubMed]
  23. Jindal, A.; Shivpuri, D.; Sood, S. Staphylococcus schleiferi meningitis in a child. Pediatr. Infect. Dis. J. 2015, 34, 329. [Google Scholar] [CrossRef] [PubMed]
  24. Yarbrough, M.; Hamad, Y.; Burnham, C.; George, I. The brief case: Bacteremia and vertebral osteomyelitis due to Staphylococcus schleiferi. J. Clin. Microbiol. 2017, 55, 3157–3161. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  25. Pomba, C.; Rantala, M.; Greko, C.; Baptiste, K.E.; Catry, B.; van Duijkeren, E.; Mateus, A.; Moreno, M.A.; Pyörälä, S.; Ružauskas, M.; et al. Public health risk of antimicrobial resistance transfer from companion animals. J. Antimicrob. Chemother. 2017, 72, 957–968. [Google Scholar] [CrossRef]
  26. Conner, J.; Smith, J.; Erol, E.; Locke, S.; Phillips, E.; Carter, C.; Odoi, A. Temporal trends and predictors of antimicrobial resistance among Staphylococcus spp. isolated from canine specimens submitted to a diagnostic laboratory. PLoS ONE 2018, 13, e0200719. [Google Scholar] [CrossRef] [Green Version]
  27. Kania, S.; Williamson, N.; Frank, L.; Wilkes, R.; Jones, R.; Bemis, D. Methicillin resistance of staphylococci isolated from the skin of dogs with pyoderma. Am. J. Vet. Res. 2004, 65, 1265–1268. [Google Scholar] [CrossRef] [PubMed]
  28. May, E.R.; Hnilica, K.A.; Frank, L.A.; Jones, R.D.; Bemis, D.A. Isolation of Staphylococcus schleiferi from healthy dogs and dogs with otitis, pyoderma, or both. J. Am. Vet. Med. Assoc. 2005, 227, 928–931. [Google Scholar] [CrossRef]
  29. Roberts, S.; O’Shea, K.; Morris, D.; Robb, A.; Morrison, D.; Rankin, S. A real-time PCR assay to detect the Panton Valentine Leukocidin toxin in staphylococci: Screening Staphylococcus schleiferi subspecies coagulans strains from companion animals. Vet. Microbiol. 2005, 107, 139–144. [Google Scholar] [CrossRef]
  30. Morris, D.; Rook, K.; Shofer, F.; Rankin, S. Screening of Staphylococcus aureus, Staphylococcus intermedius, and Staphylococcus schleiferi isolates obtained from small companion animals for antimicrobial resistance: A retrospective review of 749 isolates (2003-04). Vet. Dermatol. 2006, 17, 332–337. [Google Scholar] [CrossRef]
  31. Jones, R.; Kania, S.; Rohrbach, B.; Frank, L.; Bemis, D. Prevalence of oxacillin- and multidrug-resistant staphylococci in clinical samples from dogs: 1772 samples (2001–2005). J. Am. Vet. Med. Assoc. 2007, 230, 221–227. [Google Scholar] [CrossRef] [PubMed]
  32. Detwiler, A.; Bloom, P.; Petersen, A.; Rosser, E. Multi-drug and methicillin resistance of staphylococci from canine patients at a veterinary teaching hospital (2006–2011). Vet. Q. 2013, 33, 60–67. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  33. Kunder, D.; Cain, C.; O’Shea, K.; Cole, S.; Rankin, S. Genotypic relatedness and antimicrobial resistance of Staphylococcus schleiferi in clinical samples from dogs in different geographic regions of the United States. Vet. Dermatol. 2015, 26, 406-e94. [Google Scholar] [CrossRef] [PubMed]
  34. Cain, C.; Morris, D.; Rankin, S. Clinical characterization of Staphylococcus schleiferi infections and identification of risk factors for acquisition of oxacillin-resistant strains in dogs: 225 cases (2003–2009). J. Am. Vet. Med. Assoc. 2011, 39, 1566–1573. [Google Scholar] [CrossRef]
  35. Zdovc, I.; Ocepek, M.; Pirs, T.; Krt, B.; Pinter, L. Staphylococcus schleiferi subsp. coagulans, isolated from dogs and possible misidentification with other canine coagulase-positive staphylococci. J. Vet. Med. B Infect. Dis. Vet. Public Health 2004, 51, 449–454. [Google Scholar] [CrossRef]
  36. Foster, G.; Barley, J. Staphylococcus schleiferi subspecies coagulans in dogs. Vet. Rec. 2007, 161, 496. [Google Scholar] [CrossRef]
  37. Vanni, M.; Tognetti, R.; Pretti, C.; Crema, F.; Soldani, G.; Meucci, V.; Intorre, L. Antimicrobial susceptibility of Staphylococcus intermedius and Staphylococcus schleiferi isolated from dogs. Res. Vet. Sci. 2009, 87, 192–195. [Google Scholar] [CrossRef]
  38. Couto, N.; Monchique, C.; Belas, A.; Marques, C.; Gama, L.T.; Pomba, C. Trends and molecular mechanisms of antimicrobial resistance in clinical staphylococci isolated from companion animals over a 16 year period. J. Antimicrob. Chemother. 2016, 71, 1479–1487. [Google Scholar] [CrossRef]
  39. Ravens, P.; Vogelnest, L.; Ewen, E.; Bosward, K.; Norris, J. Canine superficial bacterial pyoderma: Evaluation of skin surface sampling methods and antimicrobial susceptibility of causal Staphylococcus isolates. Aust. Vet. J. 2014, 92, 149–155. [Google Scholar] [CrossRef] [PubMed]
  40. Penna, B.; Varges, R.; Medeiros, L.; Martins, G.; Martins, R.; Lilenbaum, W. Species distribution and antimicrobial susceptibility of staphylococci isolated from canine otitis externa. Vet. Dermatol. 2010, 21, 292–296. [Google Scholar] [CrossRef]
  41. Lee, G.; Lee, H.; Hwang, S.; Hong, J.; Lyoo, K.; Yang, S. Carriage of Staphylococcus schleiferi from canine otitis externa: Antimicrobial resistance profiles and virulence factors associated with skin infection. J. Vet. Sci. 2019, 20, e6. [Google Scholar] [CrossRef] [PubMed]
  42. Nakaminami, H.; Okamura, Y.; Tanaka, S.; Wajima, T.; Murayama, N.; Noguchi, N. Prevalence of antimicrobial-resistant staphylococci in nares and affected sites of pet dogs with superficial pyoderma. J. Vet. Med. Sci. 2021, 83, 214–219. [Google Scholar] [CrossRef] [PubMed]
  43. Chanchaithong, P.; Perreten, V.; Schwendener, S.; Tribuddharat, C.; Chongthaleong, A.; Niyomtham, W.; Prapasarakul, N. Strain typing and antimicrobial susceptibility of methicillin-resistant coagulase-positive staphylococcal species in dogs and people associated with dogs in Thailand. J. Appl. Microbiol. 2014, 117, 572–586. [Google Scholar] [CrossRef] [Green Version]
  44. Huse, H.K.; Miller, S.A.; Chandrasekaran, S.; Hindler, J.A.; Lawhon, S.D.; Bemis, D.A.; Westblade, L.F.; Humphries, R.M. Evaluation of oxacillin and cefoxitin disk diffusion and MIC breakpoints established by the Clinical and Laboratory Standards Institute for detection of mecA-mediated oxacillin resistance in Staphylococcus schleiferi. J. Clin. Microbiol. 2018, 56, e01653-17. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  45. Intorre, L.; Vanni, M.; Di Bello, D.; Pretti, C.; Meucci, V.; Tognetti, R.; Soldani, G.; Cardini, G.; Jousson, O. Antimicrobial susceptibility and mechanism of resistance to fluoroquinolones in Staphylococcus intermedius and Staphylococcus schleiferi. J. Vet. Pharmacol. Ther. 2007, 30, 464–469. [Google Scholar] [CrossRef]
  46. Davis, M.F.; Cain, C.L.; Brazil, A.M.; Rankin, S.C. Two coagulase-negative staphylococci emerging as potential zoonotic pathogens: Wolves in sheep’s clothing? Front. Microbiol. 2013, 4, 123. [Google Scholar] [CrossRef] [Green Version]
  47. Sasaki, T.; Tsubakishita, S.; Tanaka, Y.; Sakusabe, A.; Ohtsuka, M.; Hirotaki, S.; Kawakami, T.; Fukata, T.; Hiramatsu, K. Multiplex-PCR method for species identification of coagulase-positive staphylococci. J. Clin. Microbiol. 2010, 48, 765–769. [Google Scholar] [CrossRef] [Green Version]
  48. Clinical and Laboratory Standards Institute (CLSI). Performance Standards for Antimicrobial Disk and Dilution Susceptibility Tests for Bacteria Isolated from Animals, 5th ed.; CLSI Supplement VET01S; Clinical and Laboratory Standards Institute (CLSI): Wayne, PA, USA, 2020. [Google Scholar]
  49. Clinical and Laboratory Standards Institute (CLSI). Performance Standards for Antimicrobial Susceptibility Testing, 30th ed.; CLSI Supplement M100; Clinical and Laboratory Standards Institute (CLSI): Wayne, PA, USA, 2020. [Google Scholar]
  50. European Committee on Antimicrobial Susceptibility Testing (EUCAST). Breakpoint Tables for Interpretation of MICs and Zone Diameters, v11.0. 2021. Available online: http://www.eucast.org (accessed on 25 January 2021).
  51. Kronvall, G.; Kahlmeter, G.; Myhre, E.; Galas, M.F. A new method for normalized interpretation of antimicrobial resistance from disk test results for comparative purposes. Clin. Microbiol. Infect. 2003, 9, 120–132. [Google Scholar] [CrossRef] [Green Version]
  52. Beck, K.M.; Waisglass, S.E.; Dick, H.L.; Weese, J.S. Prevalence of meticillin-resistant Staphylococcus pseudintermedius (MRSP) from skin and carriage sites of dogs after treatment of their meticillin-resistant or meticillin-sensitive staphylococcal pyoderma. Vet. Dermatol. 2012, 23, 369-e67. [Google Scholar] [CrossRef]
  53. Penna, B.; Mendes, W.; Rabello, R.; Lilenbaum, W. Carriage of methicillin susceptible and resistant Staphylococcus schleiferi among dog with or without topic infections. Vet. Microbiol. 2013, 162, 298–299. [Google Scholar] [CrossRef]
  54. May, E.R.; Kinyon, J.M.; Noxon, J.O. Nasal carriage of Staphylococcus schleiferi from healthy dogs and dogs with otitis, pyoderma or both. Vet. Microbiol. 2012, 160, 443–448. [Google Scholar] [CrossRef]
  55. Hamilton, E.; Kruger, J.M.; Schall, W.; Beal, M.; Manning, S.D.; Kaneene, J.B. Acquisition and persistence of antimicrobial-resistant bacteria isolated from dogs and cats admitted to a veterinary teaching hospital. J. Am. Vet. Med. Assoc. 2013, 243, 990–1000. [Google Scholar] [CrossRef] [Green Version]
  56. Schwarz, S.; Feßler, A.T.; Loncaric, I.; Wu, C.; Kadlec, K.; Wang, Y.; Shen, J. Antimicrobial resistance among staphylococci of animal origin. Microbiol. Spectr. 2018, 6. [Google Scholar] [CrossRef]
  57. Oliveira, A.; Devesa, J.; Hill, P.; Silva, V.; Poeta, P. Treatment of selected canine dermatological conditions in Portugal—A research survey. J. Vet. Res. 2018, 62, 563–570. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  58. European Medicine Agency (EMA). Surveillance of Veterinary Antimicrobial Consumption, 2020. ‘Sales of Veterinary Antimicrobial agents in 31 European Countries in 2018′. (EMA/24309/2020); European Medicine Agency (EMA): Amsterdam, The Netherlands, 2020. [Google Scholar]
  59. Alexopoulou, K.; Foka, A.; Petinaki, E.; Jelastopulu, E.; Dimitracopoulos, G.; Spiliopoulou, I. Comparison of two commercial methods with PCR restriction fragment lengt polymorphism of the tuf gene in the identification of coagulase-negative staphylococci. Lett. Appl. Microbiol. 2006, 43, 450–454. [Google Scholar] [CrossRef] [PubMed]
  60. Sweeney, M.T.; Lubbers, B.V.; Schwarz, S.; Watts, J.L. Applying definitions for multidrug resistance, extensive drug resistance and pandrug resistance to clinically significant livestock and companion animal bacterial pathogens. J. Antimicrob. Chemother. 2018, 73, 1460–1463. [Google Scholar] [CrossRef]
  61. Kronvall, G.; Smith, P. Normalized resistance interpretation, the NRI method: Review of NRI disc test applications and guide to calculations. Apmis 2016, 124, 1023–1030. [Google Scholar] [CrossRef]
  62. The European Committee on Antimicrobial Susceptibility Testing (EUCAST). MIC Distributions and Epidemiological Cut-Off Values (ECOFF) Setting; EUCAST SOP 10.1; The European Committee on Antimicrobial Susceptibility Testing (EUCAST): Växjö, Sweden, 2019. [Google Scholar]
  63. Chung, M.; de Lencastre, H.; Matthews, P.; Tomasz, A.; Adamsson, I.; Aires de Sousa, M.; Camou, T.; Cocuzza, C.; Corso, A.; Couto, I.; et al. Multilaboratory Project Collaborators. Molecular typing of methicillin-resistant Staphylococcus aureus by pulsed-field gel electrophoresis: Comparison of results obtained in a multilaboratory effort using identical protocols and MRSA strains. Microb. Drug Resist. 2000, 6, 189–198. [Google Scholar] [CrossRef]
  64. Carriço, J.A.; Pinto, F.R.; Simas, C.; Nunes, S.; Sousa, N.G.; Frazão, N.; de Lencastre, H.; Almeida, J.S. Assessment of band-based similarity coefficients for automatic type and subtype classification of microbial isolates analyzed by pulsed-field gel electrophoresis. J. Clin. Microbiol. 2005, 43, 5483–5490. [Google Scholar] [CrossRef] [Green Version]
  65. Carriço, J.A.; Silva-Costa, C.; Melo-Cristino, J.; Pinto, F.R.; de Lencastre, H.; Almeida, J.S.; Ramirez, M. Illustration of a common framework for relating multiple typing methods by application to macrolide-resistant Streptococcus pyogenes. J. Clin. Microbiol. 2006, 44, 2524–2532. [Google Scholar] [CrossRef] [Green Version]
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Figure 1. SmaI-PFGE macrorestriction profile analysis of the 27 S. coagulans and 1 S. schleiferi isolates associated with canine skin infections and their correlation with plasmid profiles, as well as their phenotypic and genotypic resistance traits. The symbol (#) indicates the S. schleiferi isolate. The symbol (*) highlights the two S. coagulans isolates collected from the same dog. The dendrogram was built using Bionumerics and the UPGMA algorithm, using the Dice coefficient, and an optimization of 0.5% and tolerance of band of 1%. The dashed lines correspond to the similarity criteria for considering isolates belonging to the same PFGE type (≥81%) or subtype (≥97%). PFGE: pulsed-field gel electrophoresis; PEN: penicillin; CIP: ciprofloxacin; ENR: enrofloxacin; MXF: moxifloxacin; ERY: erythromycin; CLI: clindamycin; FUS: fusidic acid; TET: tetracycline; (I) intermediate phenotype; QRDR: quinolone-resistance determining region; S: serine; I: isoleucine; E: glutamic acid; A: alanine; R: arginine; F: phenylalanine; G: glycine; Y: tyrosine; WT: wild-type.
Figure 1. SmaI-PFGE macrorestriction profile analysis of the 27 S. coagulans and 1 S. schleiferi isolates associated with canine skin infections and their correlation with plasmid profiles, as well as their phenotypic and genotypic resistance traits. The symbol (#) indicates the S. schleiferi isolate. The symbol (*) highlights the two S. coagulans isolates collected from the same dog. The dendrogram was built using Bionumerics and the UPGMA algorithm, using the Dice coefficient, and an optimization of 0.5% and tolerance of band of 1%. The dashed lines correspond to the similarity criteria for considering isolates belonging to the same PFGE type (≥81%) or subtype (≥97%). PFGE: pulsed-field gel electrophoresis; PEN: penicillin; CIP: ciprofloxacin; ENR: enrofloxacin; MXF: moxifloxacin; ERY: erythromycin; CLI: clindamycin; FUS: fusidic acid; TET: tetracycline; (I) intermediate phenotype; QRDR: quinolone-resistance determining region; S: serine; I: isoleucine; E: glutamic acid; A: alanine; R: arginine; F: phenylalanine; G: glycine; Y: tyrosine; WT: wild-type.
Antibiotics 10 00518 g001
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Figure 2. Distributions of inhibition zone diameters for six antibiotics with no established breakpoints for S. coagulans and corresponding cut-off value (COWT). The COWT value (dashed orange lines) was calculated using the Normalized Resistance Interpretation (NRI) method. Grey columns represent the distribution of zone diameters; the green line indicates the NRI-generated normalized distribution of the putative WT populations.
Figure 2. Distributions of inhibition zone diameters for six antibiotics with no established breakpoints for S. coagulans and corresponding cut-off value (COWT). The COWT value (dashed orange lines) was calculated using the Normalized Resistance Interpretation (NRI) method. Grey columns represent the distribution of zone diameters; the green line indicates the NRI-generated normalized distribution of the putative WT populations.
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Table
Table 1. Antibiotic susceptibility profiles and antibiotic resistance genes detected for the 27 canine pyoderma associated S. coagulans isolates studied. Data are only presented for antibiotics with established breakpoints.
Table 1. Antibiotic susceptibility profiles and antibiotic resistance genes detected for the 27 canine pyoderma associated S. coagulans isolates studied. Data are only presented for antibiotics with established breakpoints.
AntibioticZD BreakpointNumber of Isolates (%)Resistance Determinants (No. Isolates)
S (mm)R (mm)SIR
Penicillin **≥29 a≤28 a10 (37.0%)-17 (63.0%)blaZ (16) and/or mecA (2)
Oxacillin **≥18≤1725 (92.6%)-2 (7.4%)mecA (2)
Enrofloxacin *≥23≤1616 (59.3%)2 (7.4%)9 (33.3%)QRDR mutations: GrlA [S80I, S80R, S80G]; GyrA [S80F, S80Y, E88A, E88G]
Ciprofloxacin **≥21≤1517 (63.0%)4 (14.8%)6 (22.2%)
Moxifloxacin **≥24≤2021 (77.8%)2 (7.4%)4 (14.8%)
Erythromycin **≥23≤1324 (88.9%)2 (7.4%)1 (3.7%)erm(B) (1)
Clindamycin *≥21≤1424 (88.9%)0 (0%)3 (11.1%)erm(B) (1)
Quinupristin-dalfopristin ***≥21<1827 (100%)0 (0%)0 (0%)-
Tetracycline *≥23≤1726 (96.3%)0 (0%)1 (3.7%)-
Minocycline **≥19≤1427 (100%)0 (0%)0 (0%)-
Tigecycline ***≥19<1927 (100%)0 (0%)0 (0%)
Fusidic acid ***≥24<2425 (92.6%)-2 (7.4%)-
Linezolid **≥21≤2027 (100%)-0 (0%)-
Chloramphenicol **≥18≤1227 (100%)0 (0%)0 (0%)-
Trimethoprim-sulfamethoxazole **≥16≤1027 (100%)0 (0%)0 (0%)-
Rifampicin **≥20≤1627 (100%)0 (0%)0 (0%)-
Gentamicin **≥15≤1227 (100%)0 (0%)0 (0%)-
Amikacin ***≥18<1827 (100%)-0 (0%)-
Tobramycin ***≥18<1827 (100%)-0 (0%)-
Kanamycin ***≥18<1827 (100%)-0 (0%)-
ZD: zone inhibition diameter; S: susceptible; I: intermediate; R: resistant; * Breakpoint established by CLSI for staphylococci isolated from animals, document VET01S ED5 [48]; ** Breakpoint established by CLSI for staphylococci isolated from humans, document M100-S30 [49]; *** Breakpoint established by EUCAST [50]; a Isolates with a ZD towards penicillin > 29 mm, but with a sharp inhibition border were considered producers of beta-lactamase and thus resistant to penicillin [48].
Table
Table 2. Cut-off (COWT) values of S. coagulans for six antibiotics that have no breakpoints established by CLSI or EUCAST. The COWT values were determined based on the distributions of inhibition zone diameters for 27 S. coagulans isolates by the NRI method.
Table 2. Cut-off (COWT) values of S. coagulans for six antibiotics that have no breakpoints established by CLSI or EUCAST. The COWT values were determined based on the distributions of inhibition zone diameters for 27 S. coagulans isolates by the NRI method.
COWT
(mm)		SD
(mm)		WT Population
(mm)		NWT Population
(mm)
Apramycin182.11≥18<18
Bacitracin131.85≥13<13
Florfenicol222.64≥22<22
Mupirocin323.21≥32<32
Neomycin182.20≥18<18
Novobiocin301.53≥30<30
SD: standard deviation; WT: wild-type; NWT: non-wild-type.
Table
Table 3. Brief description of the S. coagulans (n = 27) and S. schleiferi (n = 1) isolates associated with canine skin infections.
Table 3. Brief description of the S. coagulans (n = 27) and S. schleiferi (n = 1) isolates associated with canine skin infections.
IsolateIdentificationBiological SampleYearLaboratory
BIOS-V1 *S. coagulansskin swab2015Lab1
BIOS-V2S. coagulansskin swab2012Lab1
BIOS-V3S. coagulansskin swab2014Lab1
BIOS-V9S. coagulansskin swab2018Lab1
BIOS-V35S. coagulansskin swab2018Lab1
BIOS-V41S. coagulansperianal skin swab2018Lab1
BIOS-V42S. coagulansskin swab2001Lab1
BIOS-V43S. coagulansskin swab2004Lab1
BIOS-V44S. coagulansskin swab2005Lab1
BIOS-V45S. coagulansperianal fistula swab2008Lab1
BIOS-V46S. coagulansskin swab1999Lab1
BIOS-V47S. coagulansskin swab2003Lab1
BIOS-V51S. coagulansskin swab2007Lab1
BIOS-V91S. coagulansaxillar skin swab2004Lab1
BIOS-V93S. coagulansskin swab2007Lab1
BIOS-V94S. coagulansskin swab2007Lab1
BIOS-V95S. coagulansskin swab2013Lab1
BIOS-V98S. coagulansskin swab2015Lab1
BIOS-V107S. coagulansskin swab2015Lab1
BIOS-V126 *S. coagulansskin swab2016Lab1
BIOS-V139S. schleiferiskin swab2016Lab1
BIOS-V191S. coagulansskin swab2018Lab2
BIOS-V205S. coagulansskin swab2018Lab2
BIOS-V209S. coagulansskin swab2018Lab2
BIOS-V232S. coagulansepidermal collarette2018Lab2
BIOS-V243S. coagulansskin swab2018Lab2
BIOS-V265S. coagulansskin swab2018Lab2
BIOS-V289S. coagulansInterdigital skin swab2018Lab2
* Isolates collected from the same dog.
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Costa, S.S.; Oliveira, V.; Serrano, M.; Pomba, C.; Couto, I. Phenotypic and Molecular Traits of Staphylococcus coagulans Associated with Canine Skin Infections in Portugal. Antibiotics 2021, 10, 518. https://doi.org/10.3390/antibiotics10050518

AMA Style

Costa SS, Oliveira V, Serrano M, Pomba C, Couto I. Phenotypic and Molecular Traits of Staphylococcus coagulans Associated with Canine Skin Infections in Portugal. Antibiotics. 2021; 10(5):518. https://doi.org/10.3390/antibiotics10050518

Chicago/Turabian Style

Costa, Sofia Santos, Valéria Oliveira, Maria Serrano, Constança Pomba, and Isabel Couto. 2021. "Phenotypic and Molecular Traits of Staphylococcus coagulans Associated with Canine Skin Infections in Portugal" Antibiotics 10, no. 5: 518. https://doi.org/10.3390/antibiotics10050518

APA Style

Costa, S. S., Oliveira, V., Serrano, M., Pomba, C., & Couto, I. (2021). Phenotypic and Molecular Traits of Staphylococcus coagulans Associated with Canine Skin Infections in Portugal. Antibiotics, 10(5), 518. https://doi.org/10.3390/antibiotics10050518

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