Next Article in Journal
Antimicrobial Resistance in New Zealand—A One Health Perspective
Next Article in Special Issue
A Retrospective Study of Antimicrobial Resistant Bacteria Associated with Feline and Canine Urinary Tract Infection in Hong Kong SAR, China—A Case Study on Implication of First-Line Antibiotics Use
Previous Article in Journal
Characterization of β-Lactamases and Multidrug Resistance Mechanisms in Enterobacterales from Hospital Effluents and Wastewater Treatment Plant
Previous Article in Special Issue
Use of Antibiotics against Bacterial Infections on Dairy Sheep and Goat Farms: Patterns of Usage and Associations with Health Management and Human Resources

Survey on Carbapenem-Resistant Bacteria in Pigs at Slaughter and Comparison with Human Clinical Isolates in Italy

Department of Veterinary Science, University of Parma, 43126 Parma, Italy
Food Safety Unit, Department of Agricultural and Food Sciences Alma Mater Studiorum, University of Bologna, 40064 Ozzano dell’Emilia, Italy
Istituto Zooprofilattico Sperimentale della Puglia e della Basilicata, 70017 Putignano, Italy
Nephrology Unit, Parma University-Hospital, Department of Medicine and Surgery, Parma University, 43126 Parma, Italy
National Veterinary Service, 43126 Parma, Italy
Author to whom correspondence should be addressed.
Academic Editor: Dimitris C. Chatzopoulos
Antibiotics 2022, 11(6), 777;
Received: 4 May 2022 / Revised: 30 May 2022 / Accepted: 6 June 2022 / Published: 7 June 2022
(This article belongs to the Special Issue Antibiotic Resistance in Companion and Food-Producing Animals)


This study is focused on resistance to carbapenems and third-generation cephalosporins in Gram-negative microorganisms isolated from swine, whose transmission to humans via pork consumption cannot be excluded. In addition, the common carriage of carbapenem-resistant (CR) bacteria between humans and pigs was evaluated. Sampling involved 300 faecal samples collected from slaughtered pigs and 300 urine samples collected from 187 hospitalised patients in Parma Province (Italy). In swine, MIC testing confirmed resistance to meropenem for isolates of Pseudomonas aeruginosa and Pseudomonas oryzihabitans and resistance to cefotaxime and ceftazidime for Escherichia coli, Ewingella americana, Enterobacter agglomerans, and Citrobacter freundii. For Acinetobacter lwoffii, Aeromonas hydrofila, Burkolderia cepacia, Corynebacterium indologenes, Flavobacterium odoratum, and Stenotrophomonas maltophilia, no EUCAST MIC breakpoints were available. However, ESBL genes (blaCTXM-1, blaCTX-M-2, blaTEM-1, and blaSHV) and AmpC genes (blaCIT, blaACC, and blaEBC) were found in 38 and 16 isolates, respectively. P. aeruginosa was the only CR species shared by pigs (4/300 pigs; 1.3%) and patients (2/187; 1.1%). P. aeruginosa ST938 carrying blaPAO and blaOXA396 was detected in one pig as well as an 83-year-old patient. Although no direct epidemiological link was demonstrable, SNP calling and cgMLST showed a genetic relationship of the isolates (86 SNPs and 661 allele difference), thus suggesting possible circulation of CR bacteria between swine and humans.
Keywords: carbapenem resistance; ESBLs; OXA genes; antimicrobial resistance; Pseudomonas aeruginosa; pigs carbapenem resistance; ESBLs; OXA genes; antimicrobial resistance; Pseudomonas aeruginosa; pigs

1. Introduction

Antimicrobial resistance (AMR) represents an important field of One Health, a concept based on the definition of communication spaces among different environments and hosts, such as humans, animals, plants, water, and soil [1]. Among antimicrobials, resistance to carbapenems is of great concern since they are the “last-line defence” to treat human infections by multiresistant Gram-negative bacilli [2,3,4,5]. Carbapenems are not licenced for use in food-producing animals in the EU [6], but other β-lactams are commonly used, such as extended-spectrum cephalosporins, which could provide a selection pressure favouring the expression of carbapenem resistance (CR) [7]. In recent decades, intensive farming has been frequently associated with the use/abuse of antimicrobials, and AMR is common among microorganisms isolated from food-producing animals, with subsequent possible transmission to humans via direct contact with animals or ingestion of derived food products [8]. Furthermore, carbapenem-resistant (CR) and carbapenemase-producing (CP) microorganisms of human origin could be transmitted to livestock from environmental sources (e.g., hospital sewage and wastewater treatment plants contaminating water and soil) [9,10,11].
CR bacteria may deactivate the carbapenems through two main mechanisms: (i) acquisition of genes that encode for enzymes capable of hydrolysing the carbapenems, called carbapenemases; (ii) reduction in the accumulation of antibiotics due to porin deficiency combined with expression of β-lactamases with a poor affinity for carbapenems, as AmpC-β-lactamases or extended-spectrum β-lactamases (ESBLs) [4,12]. Different classes of carbapenemases are found in CP microorganisms. Class A KPC enzymes can hydrolyse all β-lactams in use but ceftaroline/avibactam [13]. Class B enzymes belonging to the IMP, VIM, and NDM families show the highest carbapenemase activity [2]. Class D carbapenem-hydrolysing oxacillinases (OXAs) have emerged in several bacterial species as responsible for carbapenem resistance [14].
In pigs, CR was observed in microorganisms belonging to different bacterial species, such as Escherichia coli harbouring blaVIM-1 [15], blaOXA-181 [16], or blaIMP-27 [7], and Salmonella Infantis harbouring blaVIM-1 [17]. The gene blaIMP-27 was identified in microorganisms isolated from swine faecal and environmental samples, such as Klebsiella oxytoca, Proteus mirabilis, Proteus vulgaris, Proteus rettgeri, Enterobacter cloacae, and Morganella morganii [7]. Despite these interesting findings assessing the dissemination of carbapenemases to microorganisms detected in swine, further studies are needed to understand the role of swine in the epidemiology of CR Gram-negative infections in humans.
CR may also result from the synthesis of ESBL and/or AmpC β-lactamase enzymes in association with quantitative and/or qualitative deficiency in the expression of outer membrane porins [18]. ESBLs are inhibitor-susceptible β-lactamases that hydrolyse penicillins, cephalosporins, and aztreonam but show a weak affinity for carbapenems. They are encoded by mobile genes, mostly belonging to SHV, TEM, and CTX m families [19]. Notably, the CTX m gene family is the most frequently detected in bacteria carried by food-producing animals and humans [20]. ESBLs, in addition to carbapenemases, have compromised the activity of almost all penicillins and cephalosporins, leading to the development of combination therapy with other β-lactams, β-lactamase inhibitors, or antibiotics from other classes [21].
Among cephalosporinases, transmissible plasmid-mediated AmpC β-lactamases commonly hydrolyse narrow-, broad-, and extended-spectrum cephalosporins and cephamycins and resist inhibition by clavulanate, sulbactam, and tazobactam. The most common plasmid-mediated AmpC β-lactamases belong to the CMY, FOX, and DHA families. These enzymes have been detected in different microorganisms, such as Klebsiella spp., Salmonella spp., Citrobacter freundii, Enterobacter aerogenes, P. mirabilis, and E. coli [22], which are often classified as multidrug-resistant [19].
Since a decade ago, resistance to third- and fourth-generation cephalosporins in ESBL/AmpC-producing E. coli of animal origin has been showing an increasing trend in the European countries, probably due to the antimicrobial treatments in livestock. Their transmission to humans poses a threat, and a worrying association of ESBL/AmpC-producing E. coli strains between fattening pigs and pig farmers has been assessed [23,24,25]. Given the importance of cephalosporins in human medicine and the emergence and distribution of resistant bacteria, monitoring of ESBL/AmpC-producing E. coli from food-producing animals and food thereof has been mandatory in the EU since 2014 [26]. Such monitoring is of crucial importance to human health because the expression of ESBL/AmpC genes in microorganisms showing porin deficiencies may be related to resistance to carbapenems [18].
The main objective of this study was focused on the One Health concept that CR bacteria could be shared between the animal and human compartments. In this perspective, meropenem was the carbapenem selected for the antimicrobial sensitivity testing because of its potency and wide antimicrobial spectrum, including Gram-negative and Gram-positive bacteria [27,28,29]. Globally, the aims of the study were (i) the detection of CR microorganisms in faecal samples collected from pigs at slaughter; (ii) the evaluation of their phenotypical resistance to carbapenems; (iii) the distribution of carbapenemase-producing genes in the porcine isolates; (iv) the genomic comparison of CR porcine microorganisms with CR bacteria isolated from hospitalised patients in the same geographical area of northern Italy. In addition, (v) resistance to third-generation cephalosporins (cefotaxime and ceftazidime) was tested, followed by detection of ESBL/AmpC genes which can contribute to CR in microbial isolates.

2. Results

2.1. Phenotypical Antimicrobial Resistance in Pig Isolates

A total of 38 Gram-negative isolates from pig faeces were selected based on the Kirby–Bauer test. They belonged to different species—namely, Acinetobacter lwoffii (n = 1), Aeromonas hydrophila (n = 2), Burkolderia cepacia (n = 3), Citrobacter freundii (n = 1), Cryseobacterium indologenes (n = 1), Enterobacter agglomerans (n = 1), Escherichia coli (n = 4), Ewingella americana (n = 1), Flavobacterium odoratum (n = 1), Pseudomonas aeruginosa (n = 4), Pseudomonas oryzihabitans (n = 1), and Stenotrophomonas maltophilia (n = 18).
Based on EUCAST guidelines [30], minimal inhibitory concentration (MIC) for sensitivity to meropenem (MEM), cefotaxime (CAZ), and ceftazidime (CTX) could be assessed for Enterobacterales, Pseudomonas spp. and Acinetobacter spp., because specific breakpoints were available. To differentiate between sensitive and resistant isolates, quantitative MICs were converted into binary qualitative values (sensitive/resistant) using the cut-off values provided by EUCAST [30]. A third category (sensitive, increased exposure) was recently introduced, in substitution of the former “intermediate” category, referring to the likelihood of therapeutic success when the dosing regimen of the antimicrobial or its concentration at the site of infection is increased. In addition, the epidemiological cut-off (ECOFF) values were used to distinguish between microorganisms with and without acquired resistance mechanisms. Conversely, for bacterial species not included in the EUCAST guide [30], only quantitative MICs values to MEM, CTX, and CAZ were recorded.
As shown in Table 1 and Table 2, resistant values to MEM were observed in strains of P. aeruginosa and P. oryzihabitans. In addition, one E. coli and one E. americana strain showed MICs for MEM higher than the ECOFF (value (>0.125 μg/mL).
Among Enterobacterales, resistance to CAZ was detected in 50% of the isolates (4/8; E. agglomerans, E. coli, and E. americana) and resistance to CTX in 62.5% of the isolates (5/8; C. freundii, E. agglomerans, E. coli, and E. americana) (Table 1). Resistance to CAZ was detected for P. oryzihabitans, while P. aeruginosa isolates were categorised as “sensitive, increased exposure”. MIC breakpoints for CAZ and CTX were not available for the other species found in pig faeces.

2.2. Phenotypical Antimicrobial Resistance in Human Isolates

The only bacterial species shared by humans and pigs was P. aeruginosa. Two isolates were detected from the human clinical samples (2/187; 1.1%). One strain (NEF 23) was resistant to MEM (MICMEM 16 μg/mL), and the other (NEF 156) was classified as “sensitive, increased exposure” (MICMEM 8 μg/mL). The two isolates were considered “sensitive, increased exposure” to CAZ (MICCAZ 4 μg/mL). Even if the sensitivity to CTX could not be evaluated, due to the absence of the clinical breakpoint, the MIC values were high for both strains (128 μg/mL and 64 μg/mL, respectively).

2.3. Whole-Genome Sequencing (WGS) of Porcine and Human Isolates

According to the aims of the present study, P. aeruginosa isolates from pigs and patients were sequenced by using MiSeq Illumina Platform (Illumina, Milan, Italy). In pigs, the carriers of four CR P. aeruginosa strains (apparent prevalence 1.3%; 95% CI 0.5–3.4) were reared on four farms in the Lombardy Region, northern Italy. As shown in Table 2, P. aeruginosa strains belonged to four sequence types—namely, ST274, ST782, ST885, and ST938. All of the isolates harboured the blaPAO gene. In addition, blaOXA-50 (ST782 and ST885), blaOXA-396 (ST938), and blaOXA-486 (ST274) genes were found, together with genes for resistance to aminoglycosides (aph(3′)-IIb), chloramphenicol (catB7), ciprofloxacin (crpP), and fosfomycin (fosA).
Results on de novo assembly statistics are reported in Table 3 and Supplementary Table S1. Genome sizes (from 6,396,234 to 7,099,705 bp) and GC content (from 65.85% to 66.83%) confirmed the P. aeruginosa species identification of the newly sequenced genomes [31]. The number of contigs ranged from 124 to 317, N50 (the length of the shortest contig of the 50% of the assembly including equal or longer contigs) ranged from 38,674 to 126,411, and the maximum contig length from 223,278 to 561,477. These values highlight the high quality of de novo assemblies in terms of contiguity as reported previously on both P. aeruginosa genomes and bacterial genomes of similar size [32,33]. The sequencing coverage is a parameter related to the number of times each nucleotide of a given genome is sequenced starting from the assumption that reads are randomly distributed. The average depth of sequencing coverage is equal to LN/G, where L and N are the length and the number of reads, respectively, and G is the length of the haploid genome [34]. A coverage higher than 50× is generally recommended to allow reliable calling of single nucleotide variants (SNVs) such as single nucleotide polymorphisms (SNPs). In the present study, the coverage ranged from 76.6 to 105.2×.
SNP calling confirmed results of MLST typing with a higher level of discriminatory power (Figure 1A). Based on the maximum likelihood phylogenetic tree built on 68790 SNPs, newly sequenced genomes were distantly related except for ST938 isolates CRE 102 and NEF 23 of porcine and human origin, respectively. P. aeruginosa genomes CRE 153, CRE 295, CRE 98, and NEF 156 showed pairwise SNPs distances ranging from 25,928 to 33,748, whereas CRE 102 and NEF 23 showed 86 SNPs of difference confirming their genetic relationship (Table S2). NEF 23 was collected from an 83-year-old male patient suffering from an episode of acute kidney insufficiency due to sepsis, on previous chronic kidney disease. Not surprisingly, comparing genomes of different ST-types (ST274, ST782, ST885, ST395) the genetic distance increased with pairwise SNPs differences (Table S2). The genetic relatedness between CRE 102 and NEF 23 was reinforced by cgMLST results, which identified 661 allelic differences corresponding to the 25% on a total of 2653 alleles of the cgMLST scheme (Figure 1B). The other genomes showed allelic differences ranging from 2133 to 2219 corresponding on average to 82% of the scheme.
As shown in Table 2, the porcine and human isolates were characterised by an identical resistome consisting of five antimicrobial genes conferring decreased susceptibility to β-lactams and meropenem (blaOXA-396, blaPAO) as well as resistance to aminoglycosides (aph(3′)-IIb), chloramphenicol (catB7), and fosfomycin (fosA). Epidemiological links between the carrier pig (reared in Cremona Province, Lombardy Region) and the patient (living in Parma Province, Emilia–Romagna Region) were not investigated because of the lack of information about the patient’s eating habits, pig exposure, or living environment.
The other P. aeruginosa strain (NEF 156) isolated from a 52-year-old female patient suffering from acute kidney insufficiency belonged to ST395 and harboured blaPAO and blaOXA-488 genes, thus differing from the porcine isolates detected in the study. Its resistome consisted of six determinants conferring decreased susceptibility to β-lactams and carbapenems (blaOXA-488, blaPAO) and resistance to aminoglycosides (aph(3′)-IIb), chloramphenicol (catB7), ciprofloxacin (crpP), and fosfomycin (fosA) (Table 2).

2.4. Localisation of Carbapenemase-Encoding Genes

Based on RAST and PROKKA annotation results and confirming previous data, blaOXA and blaPAO genes showed genetic environments which did not show any specific sequence of mobilisable genetic elements (MGEs) (Figure 2 and Figure 3).

2.5. Detection of Carbapenemases, β-Lactamases, and AmpC Genes in Other Pig Isolates

PCR testing of the strains detected in pigs revealed negative results for blaKPC, blaIMP, blaVIM, and blaNDM genes. blaTEM-1 and blaCTX-M1 were found in 100% and 26.3% (10/38) of the isolates, respectively. blaSHV was detected in 5.3% (2/38) of the isolates, and precisely in one E. coli strain resistant to CTX and CAZ and in one B. cepacia showing high MIC values for CTX and CAZ. Among plasmidic AmpC genes, blaMOX, blaDHA, and blaFOX were never detected. blaCIT was found in 34.2% (13/38) of the isolates and exactly in a MEM-sensitive C. freundii and in 12 S. maltophilia. blaACC and blaEBC were found in one (2.6%) and two (5.3%) S. maltophilia isolates, respectively (Table 1).

3. Discussion

In recent years, the concept of One Health has been reformulated underlying the role of geographically close ecosystems in the occurrence of traits which have an impact on the human, animal, plant, and environmental health, such as AMR. Therefore, the studies of CR in microorganisms shared by food-producing animals and humans are crucial to assessing the contribution of animals to CIA resistance transmission. AMR bacteria in food-producing animals can be transmitted to humans via food-borne routes, as demonstrated for some zoonotic microorganisms (e.g., thermotolerant Campylobacter, Salmonella, Shiga toxin-producing Escherichia coli). At slaughter, carcass contamination by microorganisms shed by pigs can occur [35,36,37], thus causing their spread to consumers via ingestion of raw and undercooked pork and products thereof. Transmission of AMR bacteria from animals to humans may also occur through environmental contamination and direct animal contact. In addition, the commensal bacterial flora can act as a reservoir of AMR genes, which may be transferred to microorganisms capable of causing disease in both humans and animals [38].

3.1. CR P. aeruginosa in Pigs and Humans

Our study was focused on the detection of CR microorganisms in pigs entering the slaughter line, with a special interest in those bacterial species contemporarily found in patients hospitalised in the same geographical area. To the best of our knowledge, this is the first report of a CR P. aeruginosa ST938 strain carrying blaOXA-396 and blaPAO genes isolated from pigs and humans in northern Italy (MICMEM 16 µg/mL). No epidemiological links were demonstrable between the animal (slaughtered in 2018) and the patient (hospitalised in 2019) so we could not hypothesise any role of pigs or pork in its transmission. In fact, anamnestic data collected from the patients did not include any information on their eating habits or professional/family association with pigs or the pork industry. Nevertheless, we could not exclude that, in some circumstances, pigs, pork, and products thereof could be a source of CR microorganism transmission to humans.
As is well known, P. aeruginosa is intrinsically resistant to most antimicrobials due to its ability to prevent penetration or to extrude different molecules from the cell by expressing several efflux pump systems and to the chromosomally encoded AmpC β-lactamase [39,40,41]. However, it can acquire resistance through chromosomal mutations as well as the acquisition of AMR genes via horizontal transfer [42]. Its ability to acquire resistance to antimicrobials and to adapt to different environmental conditions are the bases for its increasing prevalence in nosocomial infections worldwide [43,44]. The occurrence of CR P. aeruginosa in human patients varies in prevalence in the European countries, ranging from below 5% to more than 50% [45].
In pigs, other three isolates of P. aeruginosa carrying blaPAO, together with blaOXA-50, blaOXA-486, and blaOXA-488, genes were detected from animals reared on different farms. blaOXA-50 is an intrinsic oxacillinase, which can confer decreased susceptibility to ampicillin, ticarcillin, and meropenem [46]. Specifically, following the RAST annotation [47], the OXA-50 family comprises also the blaOXA-396, blaOXA-486, and blaOXA-488 genes. The MDR nature of P. aeruginosa isolates is assessed by the presence of resistance determinants to aminoglycosides, ciprofloxacin, and fosfomycin, which are critically important antimicrobials (CIAs) for human medicine, as well as resistance to chloramphenicol, which is a highly important antimicrobial in human treatments [48]. In parallel with blaPAO and blaOXA genes, genes with resistance to aminoglycosides, ciprofloxacin, chloramphenicol, and fosfomycin were also shown in the human P. aeruginosa ST938 and ST395 strains.
In most cases, P. aeruginosa does not have a primary role in pig infections but is frequently reported by laboratories because of its easiness of identification [49]. Although its role in the pathogenesis of atrophic rhinitis has been suggested, it seems to be unable to initiate disease in the nasal cavities of specific-pathogen-free pigs [50]. Some P. aeruginosa strains of porcine origin produce enterotoxins that involve fluid accumulation [51], while others can be involved in cystitis, vaginal infections, mastitis, and septicemias in newborn pigs caused by ascending infections [49]. In humans, P. aeruginosa is considered an opportunistic pathogen, causing severe infections in patients with impaired health status [52], and the emergence of CR P. aeruginosa is a significant contributor to patient morbidity and mortality [53].

3.2. ESBL/AmpC Genes Harbouring Porcine Isolates

The absence of clinical breakpoints and ECOFF values for most of the microorganisms detected in this study made it impossible to assess their resistance to carbapenems or deviation from “wild-type” phenotypes. For this reason, since their phenotypical resistance to carbapenems was only putative based on breakpoints set up for other species, all isolates were tested for carbapenemase genes. In addition, since decreased sensitivity to carbapenems could be caused by ESBL and AmpC β-lactamases associated with outer membrane porin loss [18,54,55], the isolates were tested both for phenotypical resistance to third-generation cephalosporins—commonly used in pig husbandry—and the presence of cephalosporinase encoding genes [56].
Among Enterobacterales, E. coli was the most common species detected in the study. Despite carbapenemase-producing genes having been detected in E. coli of porcine origin in different countries [15,57,58,59,60], our isolates lacked blaKPC, blaIMP, blaVIM, and blaNDM genes. They harboured blaTEM-1 (100%), alone or in combination with blaCTX-M1 (25%) or blaSHV (25%). Our findings suggest a different distribution of ESBL genes from those reported by Rega et al. [61], which detected blaCTX-M1 in 89% and blaTEM-1 in 57% of E. coli strains of pork origin. MICs for meropenem were lower than the ECOFF in all the isolates, except in one strain (4 µg/mL) harbouring blaTEM-1. The same result was obtained for an isolate of E. americana (MICMEM 4 µg/mL), which was resistant to CAZ (MICCAZ 32 µg/mL) and CTX (MICCTX 16 µg/mL) and harboured blaTEM-1 and blaCTX-M1 genes. Interestingly, since E. americana is a rare but true human pathogen, able to cause serious invasive infections such as meningitis [62,63], its carriage by pigs is of concern. Globally, the contemporary presence of blaTEM-1 and blaCTX-M1, or blaTEM-1 and blaSHV, in members of the Enterobacterales was always associated with resistance to CAZ and CTX, while detection of only blaTEM-1 (100% of the isolates) was not.
Among Pseudomonas spp., P. oryzihabitans showed resistance to MEM (256 µg/mL) as well as to CAZ (256 µg/mL) and harboured blaTEM-1. This species is rarely isolated both from pigs and humans; regarding the latter, it can cause bacteriemia and peritonitis in immunocompromised patients [64,65].
The only species belonging to Acinetobacter spp. found in pig faeces was A. lwoffii. The isolate was sensitive to MEM according to the MIC testing and carried blaTEM-1, but its sensitivity to CAZ and CTX could not be evaluated for the absence of MIC breakpoints.
blaTEM-1 and blaCTX-M1 genes were detected in other species, such as A. hydrophila, B. cepacia, C. indologenes, and F. odoratum. Overall, MICs for MEM ranged from 4 µg/mL to 16 µg/mL, MICs for CAZ from 8 µg/mL to 512 µg/mL, and MICs for CTX varied between 16 µg/mL and 256 µg/mL. No relationship between cephalosporinase genes and level of resistance was found, since B. cepacia harbouring blaTEM-1, blaCTXM-1, and blaSHV showed lower MIC values than C. indologenes carrying only blaTEM-1. These findings suggest that detection of cephalosporinase genes alone could not be indicative of resistance since other mechanisms are interrelated and contribute to AMR.
Interestingly, B. cepacia and C. indologenes are human opportunistic pathogens in immunocompromised patients [66,67], and their carriage by pigs is of concern. Another isolate carrying blaTEM-1 and blaCTX-M1 was A. hydrophila, which can cause diarrhoea in piglets [68], and is resistant to a wide range of antimicrobials [69] and an opportunist pathogen in immunocompromised people [70]. Concerning blaTEM-1-positive F. odoratum, Flavobacterium spp. are reported as nosocomial-acquired opportunistic pathogens, due to their occurrence in patients with advanced immunodeficiency and resistance to many antimicrobials [71].
Lastly, the most common species detected in pig faeces was Stenotrophomonas maltophilia, an environmental multidrug-resistant (MDR) microorganism which exhibits resistance to several classes of antimicrobials, including β-lactams, cephalosporins, carbapenems, trimethoprim/sulfamethoxazole, macrolides, fluoroquinolones, aminoglycosides, chloramphenicol, tetracyclines, and polymyxins [72]. S. maltophilia is an opportunistic pathogen responsible for nosocomial infections, diseases in immunocompromised people, and chronic pulmonary infections in patients with cystic fibrosis [73,74]. Most S. maltophilia isolates (77.8%) carried blaTEM-1, and the remaining ones carried blaTEM-1 and blaCTX-M1. Their MICs values for MEM, CAZ, and CTX could not be interpreted as resistant or susceptible in absence of EUCAST clinical breakpoints.
Globally speaking, the emergence and distribution of CR Gram-negative pathogens, with a special interest in Enterobacterales, influences the outcome of human infections [75,76] because CR Gram-negative bacilli remain a threat, as few antimicrobial agents are reliably active.

4. Materials and Methods

4.1. Sample Collection

From January 2017 to March 2018, 300 finishing pigs were randomly selected during 23 visits to a slaughterhouse in Parma Province. The animals belonged to 300 batches and were reared on 95 farms in northern Italy, including the regions of Lombardy, Veneto, Emilia–Romagna, Piedmont, and Tuscany. The maximum distance between farms was 477 km, and the minimum distance was 3.5 km, with an average of 21 km. Most farms (72/95) were in the Lombardy Region, where pig husbandry has the highest density in the country. The faecal material was aseptically collected from the caecum of pigs immediately after evisceration and placed in sterile containers, stored at 4 °C, and transported to the laboratory on the day of sampling.

4.2. Sample Testing

The faecal samples were tested following the method proposed by the Technical University of Denmark [77] for the detection of ESBL-, AmpC-, and carbapenemase-producing E. coli, with some modifications. A 10 g aliquot of caecal material was suspended in 90 mL of buffered peptone water (BPW; Biolife Italiana, Milan, Italy) and incubated at 37 ± 1 °C for 18–22 h. After enrichment, cultures were tested as follows: (i) first, 100 µL were seeded onto MacConkey agar (Oxoid, Basingstoke, UK) plates aseptically added with a 10 µg meropenem disk (Oxoid), and then (ii) 10 µL were plated onto Brilliance CRE agar (Oxoid), a chromogenic selective medium which provides presumptive identification of CR microorganisms, such as E. coli (pale pink colonies), the Klebsiella, Enterobacter, Serratia, and Citrobacter (KESC) group (blue colonies) and Acinetobacter spp. (white to naturally pigmented colonies). Plates were incubated aerobically at 35 ± 2 °C for 18–24 h. Brilliance CRE negative plates were incubated for an additional 24 h before being discharged.
Each colony grown in Brilliance CRE agar plates was selected regardless of its colour and shape, and we considered both lactose-fermenting and non-fermenting colonies grown in the proximity of the meropenem disk in MacConkey agar plates. The selected colonies were subcultured onto trypticase soy agar plates (TSA; Oxoid). After incubation at 37 ± 1 °C for 18–22 h, pure cultures were Gram-stained. Gram-positive cultures were discharged.

4.3. Isolate Screening and Species Identification

Gram-negative isolates were tested for oxidase activity and screened for resistance to MEM using the Kirby–Bauer disk diffusion susceptibility test following the European Committee on Antimicrobial Susceptibility Testing (EUCAST) recommendations [78]. Zone inhibition diameters of oxidase-negative strains were evaluated on the bases of the clinical and ECOFF breakpoints proposed for the Enterobacterales [79]. For oxidase-positive isolates, the clinical breakpoints for Pseudomonas were followed, as they were the only ones available. Resistant isolates or isolates with zone diameters smaller than the ECOFF value (available for Enterobacterales only) were identified at the species level by using API® 20 E system (bioMérieux, Marcy l’Etoile, France) or API® 20 NE system (bioMérieux). After identification, the isolates were frozen at −80 °C for further testing.

4.4. MIC Testing

The conserved cultures were revitalised via inoculation in non-selective BPW at 37 °C overnight. The minimal inhibitory concentration (MIC) test for sensitivity to MEM, CAZ, and CTX was carried out following EUCAST guidelines [80]. Briefly, 96-well plates were used to perform a 2-fold serial dilution of the antibiotics tested. The bacterial suspension was added at the final concentration of 5 × 105 CFU mL−1, and each test was repeated 3 times. The MIC values were determined by wide-eye reading. Results were recorded as the lowest concentration of antimicrobial agent that completely inhibits visible bacterial growth expressed in μg/mL. E. coli ATCC 25922 (ATCC, Manassas, VA, USA) was tested periodically as a quality-control microorganism.
Concerning Enterobacterales [81], both the MEM-resistance clinical breakpoint (>8 µg/mL) and the ECOFF value (>0.125 µg/mL) were available. For Pseudomonas spp. and Acinetobacter spp., MEM-resistance clinical breakpoints were different in case of meningitis (>2 μg/mL) or other clinical indications (>8 μg/mL). Following the purpose of the study, MIC > 8 μg/mL was considered indicative of resistance.
Even in absence of MIC breakpoints for most of the species detected in swine, all of the isolates were tested for sensitivity to MEM, CAZ, and CTX.

4.5. Comparison with CR Human Isolates

After performing the study on pigs, a survey on 187 patients affected by renal diseases hospitalised at the Parma University Hospital was conducted in 2019. Three hundred urine samples were collected from indwelling bladder catheters. Most patients (mean age 77 years (range 58–88)) were tested more than once because of prolonged hospitalisation and had been admitted with a diagnosis of acute kidney injury (97/187, 51.9%) or kidney transplant (90/187, 48.1%). The selection of patients was based on their willingness to participate in the study and their capacity to urinate. Urine aliquots of 1 mL were analysed following the protocol of the Center for Disease Control and Prevention [82], with some modifications. Following the purpose of the study, a comparison between the CR human isolates which belonged to the same species detected in pigs was performed by sequencing their entire genome.

4.6. Genotypic Confirmation Test

The isolates belonging to bacterial species not shared by pigs and humans were not analysed by WGS but were tested via PCR for carbapenemase-, ESBL-, and AmpC-producing genes.
A multiplex end-point PCR was used for the detection of blaKPC, blaNDM, blaVIM, blaIMP, and blaOXA-48-like genes. Five colonies of overnight bacterial culture on TSA (Oxoid) were diluted in 1 mL of sterile distilled water. DNA extraction was performed by heating at 95 °C for 10 min, and cellular debris was removed via 15,000 rpm centrifugation for 5 min. The supernatant was used for amplification after proper quantification with Biospectrometer Basic Eppendorf (Eppendorf, Milan, Italy). The primer sequences used are the ones described by Doyle et al. [83], as well as those indicated in the multiplex PCR protocol, with some modifications. The amplification was carried out with a GoTaq G2 Flexi DNA Polymerase Kit (Promega Italia, Milan, Italy). The master mix was prepared for 50 μL of final volume reaction containing 5× Green GoTaq Flexi Buffer at a final concentration of 1×, 2 mM of MgCl2, 0.2 mM of dNTPs, and 2 U of GoTaq G2 Flexi DNA Polymerase. blaKPC, blaVIM, and blaIMP primers were added at a final concentration of 0.3 μM, blaNDM at 0.4 μM, and blaOXA-48-like at 0.5 μM. A total of 1 μL of sample lysate was added to the reaction mixture and nuclease-free water to the final volume. The PCR protocol consists of an initial denaturation of 95 °C for 5 min, followed by 35 cycles of DNA denaturation at 95 °C for 45 s, primer annealing at 62 °C for 45 s, and extension at 72 °C for 1 min. The final extension was performed at 72 °C for 8 min. PCR products were evaluated by electrophoresis with 1.5% agarose gels stained with SYBR Safe DNA gel stain (Invitrogen, Carlsbad, CA, USA) and visualised via UV light. A 100 bp DNA ladder from Promega (Milan, Italy) was used as a marker. Positive, negative, and no-template controls were included.
The ESBL genes blaCTX-M1, blaCTX-M2, blaTEM-1, and blaSHV were detected following the real-time PCR protocol described by Roschansky et al. [84], with some modifications. DNA extraction was performed as previously described. Real-time amplifications were performed in 20 μL reactions containing 10 μL Gotaq qPCR Mix 2× (Promega Italia) at a final concentration of 1×. Forward and reverse primers were added at a final concentration of 0.3 μM. Each gene was tested individually. Supplemental CXR reference dye was added at 300 nM. A total of 1 μL of sample lysate was added to the reaction mixture and nuclease-free water to the final volume. The amplification protocol included a denaturation step (95 °C for 3 min) and 39 repeated cycles (95 °C for 15 s; 50 °C for 15 s; and 72 °C for 20 s). Fluorescence signals were collected in every cycle, and each sample was tested twice. Positive, negative, and no-template controls were included.
AmpC resistance genes (blaMOX, blaCIT, blaDHA, blaACC, blaEBC, and blaFOX) were tested following the multiplex PCR protocol described by Pérez-Pérez and Hanson [85], with some modifications. The multiplex PCR master mix was prepared as described for carbapenemases, with the exception of primer final concentration (blaMOX, blaCIT, and blaDHA at concentrations of 0.6 μM, blaACC and blaEBC at 0.5 μM, and blaFOX at 0.4μM) and 1.25 U of GoTaq G2 Flexi DNA Polymerase. The PCR amplification protocol consisted of an initial denaturation of 94 °C for 3 min, followed by 25 cycles of DNA denaturation at 94 °C for 30 s, primer annealing at 64 °C for 30 s, and extension at 72 °C for 1 min. The final extension was performed at 72 °C for 7 min. PCR products were evaluated via electrophoresis with 2% agarose gels stained with SYBR Safe DNA gel stain (Invitrogen) and visualised via UV light. A 100 bp DNA ladder from Promega was used as a marker. Positive, negative, and no-template controls were included.

4.7. Whole-Genome Sequencing

Whole-genomic DNA of the porcine and human P. aeruginosa isolates was extracted using the MagAttract HMW DNA Kit (QIAGEN, Hilden, Germany). The purified DNA concentration and the quality parameter ratio 260/280 were measured via BioSpectrometer fluorescence (Eppendorf). Whole genomes were sequenced on the Illumina MiSeq platform (Nextera library, paired-end reads). The INNUca v3.2 pipeline was used to quality check and de novo assemble reads into contigs [86]. The pipeline includes SPAdes v3.11 as a de novo assembler and provides multilocus sequence typing (MLST) profiles. Standard descriptive statistics of contig sequences were estimated with contig_info v2.01 [87].
SNP calling was performed on reads using snippy v4.0.5 pipeline with default settings and Pseudomonas aeruginosa PAO1 (NCBI Ref Seq NC_002516.2) was selected as reference genomes [88]. The reference was selected based on a high nucleotide-level genomic similarity (>99% of average nucleotide identity, ANI) in pairwise comparison with other P. aeruginosa genomes, assessed with FastANI v1.33 [89]. A maximum likelihood (ML) phylogeny was inferred on the core SNP alignments using RAxML v8.2.12, applying the GTRGAMMA evolutionary model [90]. Branch support was estimated using 1000 bootstrap replicates. The resulting ML tree was visualised using iTOL v4.2.3 software [91]. Furthermore, a cgMLST analysis was carried out with the chewBBACA suite v2.8.5 [92] using an available 2653 loci scheme [93]. A minimum spanning tree was obtained with the Phyloviz online software [94], based on P. aeruginosa cgMLST allelic profiles using the implemented eBURST algorithm.
Analysis of resistome of genomes was performed using ABRicate [95]. With this tool, a BLAST search of genes included in the Resfinder database was performed on de novo assemblies [96]. De novo assemblies were annotated using Prokka v1.13.3 [97] and RAST version 2.0 [47]. Gbk files were used as input files for visualisation of the genetic environment of carbapenemase-encoding genes by SnapGene [98]. Assembled sequences are available at the National Center for Biotechnology Information [99] BioProject PRJNA587603.

5. Conclusions

In our study, an MDR P. aeruginosa ST938 strain carrying blaOXA-396 and blaPAO was the only CP microorganism shared by pigs and humans. An epidemiological investigation was not conducted because the anamnestic data collected from the P. aeruginosa ST938—positive patient at the hospital did not include any information on his eating habits or professional/familiar personal association with pigs or the pork industry. Nevertheless, our finding suggests that swine and their derivative products probably play minor roles in the transmission of CP bacteria to humans in the area of the study.
The absence of clinical breakpoints for most of the bacterial species detected in pigs hampered the evaluation of their phenotypical resistance to carbapenems, thus requiring genomic testing. Although carbapenemase-producing genes were not found in microorganisms relevant to human health, such as E. coli, Ewingella americana, and Stenotrophomonas maltophilia, a wide range of ESBL- and AmpC-producing genes were detected. Such findings are of concern because, in case of porin deficiencies, expression of ESBL- and AmpC-producing genes could be co-responsible for resistance to carbapenems.
Another interesting finding of the study in pigs is their carriage of AMR human opportunistic pathogens (Stenotrophomonas maltophilia, Burkolderia cepacia, Criseobacterium indologenes, Aeromonas hydrophila, and Flavobacterium odoratum), as well as the carriage of a true human pathogen (Ewingella americana). These data could shed new light on the possible transmission of bacterial pathogens between pigs and humans, thus improving our knowledge of the epidemiology of some human infections.

Supplementary Materials

The following supporting information can be downloaded at:, Table S1: Statistics of de novo genome assembly; Table S2: SNP distance matrix

Author Contributions

Conceptualisation, S.B., E.F. and F.P.; methodology, S.B., F.P. and C.S.C.; software, C.C. and F.P.; formal analysis, A.P., M.R., A.S., C.S., M.I. and F.R.; writing—original draft preparation, S.B.; writing—review and editing, G.M., F.P, E.F., S.C. and C.B.; funding acquisition, S.B. All authors have read and agreed to the published version of the manuscript.


This research was funded by Fondazione Cariparma, grants number No 2016.0108 and No 2018.0176, and by FIL-2019 University of Parma.

Institutional Review Board Statement

This study was conducted in accordance with the Declaration of Helsinki and approved by the Ethics Committee of Area Vasta Emilia Nord (protocol code 24497 approved on 10 June 2019).

Informed Consent Statement

Informed consent was obtained from all subjects involved in the study or their closest relatives.

Data Availability Statement

Assembled sequences are available at the National Center for Biotechnology Information (NCBI) BioProject PRJNA587603.

Conflicts of Interest

The authors declare no conflict of interest.


  1. Baquero, F.; Coque, T.M.; Martinez, J.-L.; Aracil-Gisbert, S.; Lanza, V.F. Gene transmission in the One Health microbiosphere and the channels of antimicrobial resistance. Front. Microbiol. 2019, 10, 2892. [Google Scholar] [CrossRef][Green Version]
  2. Nordmann, P.; Naas, T.; Poirel, L. Global spread of carbapenemase producing Enterobacteriaceae. Emerg. Infect. Dis. 2011, 17, 1791–1798. [Google Scholar] [CrossRef]
  3. Nordmann, P.; Dortet, L.; Poirel, L. Carbapenem resistance in Enterobacteriaceae: Here is the storm! Trends Mol. Med. 2012, 18, 263–272. [Google Scholar] [CrossRef] [PubMed]
  4. Patel, G.; Bonomo, R.A. “Stormy waters ahead”: Global emergence of carbapenemases. Front. Microbiol. 2013, 4, 48. [Google Scholar] [CrossRef][Green Version]
  5. Zhanel, G.G.; Wiebe, R.; Dilay, L.; Thomson, K.; Rubinstein, E.; Hoban, D.J.; Noreddin, A.M.; Karlowsky, J.A. Comparative review of the carbapenems. Drugs 2007, 67, 1027–1052. [Google Scholar] [CrossRef]
  6. Roschanski, N.; Friese, A.; von Salviati-Claudius, C.; Hering, J.; Kaesbohrer, A.; Kreienbrock, L.; Roesler, U. Prevalence of carbapenemase producing Enterobacteriaceae isolated from German pig-fattening farms during the years 2011–2013. Vet. Microbiol. 2017, 200, 124–129. [Google Scholar] [CrossRef] [PubMed]
  7. Mollenkopf, D.F.; Stull, J.W.; Mathys, D.A.; Bowman, A.S.; Feicht, S.M.; Grooters, S.V.; Daniels, J.B.; Wittuma, T.E. Carbapenemase-Producing Enterobacteriaceae Recovered from the Environment of a Swine Farrow-to-Finish Operation in the United States. Antimicrob. Agents Chemother. 2017, 61, e01298-16. [Google Scholar] [CrossRef][Green Version]
  8. FAO; OIE; WHO (Food and Agriculture Organization of the United Nations, World Organization for Animal Health, World Health Organization). Monitoring and Evaluation of the Global Action Plan on Antimicrobial Resistance: Framework and Recommended Indicators. 2019. Available online: (accessed on 1 December 2021).
  9. Hoelle, J.; Johnson, J.R.; Johnston, B.D.; Kinkle, B.; Boczek, L.; Ryu, H.; Hayes, S. Survey of US wastewater for carbapenem-resistant Enterobacteriaceae. J. Water Health 2019, 17, 219–226. [Google Scholar] [CrossRef]
  10. Hu, Z.; Chen, W.; Guo, G.; Dong, C.; Shen, Y.; Qin, S.; Chen, L.; Zhang, W. An Escherichia coli isolate from hospital sewage carries bla(NDM-1) and bla(oxa-10). Arch. Microbiol. 2021, 203, 4427–4432. [Google Scholar] [CrossRef]
  11. Yao, Y.; Lazaro-Perona, F.; Falgenhauer, L.; Valverde, A.; Imirzalioglu, C.; Dominguez, L.; Cantón, R.; Mingorance, J.; Chakraborty, T. Insights into a Novel bla(KPC-2)-Encoding IncP-6 Plasmid Reveal Carbapenem-Resistance Circulation in Several Enterobacteriaceae Species from Wastewater and a Hospital Source in Spain. Front. Microbiol. 2017, 8, 1–7. [Google Scholar] [CrossRef]
  12. Jeong, J.H.; Lee, J.H.; Lee, J.J.; Park, K.S.; Karim, A.M.; Lee, C.R.; Jeong, B.C.; Lee, S.H. Structural basis for carbapenem-hydrolyzing mechanisms of carbapenemases conferring antibiotic resistance. Int. J. Mol. Sci. 2015, 16, 9654–9692. [Google Scholar] [CrossRef] [PubMed]
  13. Castanheira, M.; Sader, H.S.; Farrell, D.J.; Mendes, R.E.; Jones, R.N. Activity of ceftaroline-avibactam tested against Gram-negative organism populations, including strains expressing one or more β-lactamases and methicillin-resistant Staphylococcus aureus carrying various staphylococcal cassette chromosome mec types. Antimicrob. Agents Chemother. 2012, 56, 4779–4785. [Google Scholar] [CrossRef] [PubMed][Green Version]
  14. Naas, T.; Oueslati, S.; Bonnin, R.A.; Dabos, M.L.; Zavala, A.; Dortet, L.; Retailleau, P.; Iorga, B.I. Beta-lactamase database (BLDB) -structure and function. J. Enzym. Inhib. Med. Chem. 2017, 32, 917–919. [Google Scholar] [CrossRef]
  15. Fischer, J.; Rodríguez, I.; Schmoger, S.; Friese, A.; Roesler, U.; Helmuth, R.; Guerra, B. Escherichia coli producing VIM-1 carbapenemase isolated on a pig farm. J. Antimicrob. Chemother. 2012, 67, 1793–1795. [Google Scholar] [CrossRef]
  16. Pulss, S.; Semmler, T.; Prenger-Berninghoff, E.; Bauerfeind, R.; Ewers, C. First report of an Escherichia coli strain from swine carrying and OXA-181 carbapenemase and the colisitin determinant MCR-1. Int. J. Antimicrob. Agents 2017, 50, 232–236. [Google Scholar] [CrossRef]
  17. Fischer, J.; Rodríguez, I.; Schmoger, S.; Friese, A.; Roesler, U.; Helmuth, R.; Guerra, B. Salmonella enterica subsp. enterica producing VIM-1 carbapenemase isolated from livestock farms. J. Antimicrob. Chemother. 2013, 68, 478–480. [Google Scholar] [CrossRef][Green Version]
  18. Martínez- Martínez, L. Extended spectrum β-lactamase and the permeability barrier. Clin. Microbiol. Infect. 2008, 14 (Suppl. 1), 82–89. [Google Scholar] [CrossRef][Green Version]
  19. Thomson, K.S. Extended-spectrum-β-lactamase, AmpC, and carbapenemase issues. J. Clin. Microbiol. 2010, 48, 1019–1025. [Google Scholar] [CrossRef] [PubMed][Green Version]
  20. von Salviati, C.; Laube, H.; Guerra, B.; Roesler, U.; Friese, A. Emission of ESBL/AmpC-producing Escherichia coli from pig fattening farms to surrounding areas. Vet. Microbiol. 2015, 175, 77–84. [Google Scholar] [CrossRef]
  21. Bush, K.; Bradford, P.A. β-lactams and β-lactamase inhibitors: An overview. Cold Spring Harb. Perspect. Med. 2016, 6, a025247. [Google Scholar] [CrossRef]
  22. Jacoby, G.A. AmpC beta-lactamases. Clin. Microbiol. Rev. 2009, 22, 161–182. [Google Scholar] [CrossRef] [PubMed][Green Version]
  23. Bergšpica, I.; Kaprou, G.; Alexa, E.A.; Prieto, M.; Alvarez-Ordóñez, A. Extended Spectrum β-Lactamase (ESBL) Producing Escherichia coli in Pigs and Pork Meat in the European Union. Antibiotics 2020, 9, 678. [Google Scholar] [CrossRef]
  24. Dohmen, W.; Bonten, M.J.M.; Bos, M.E.H.; van Marm, S.; Scharringa, J.; Wagenaar, J.A.; Heederik, D.J.J. Carriage of extended spectrum β-lactamases in pig farmers is associated with occurrence in pigs. Clin. Microbiol. Infect. 2015, 21, 917–923. [Google Scholar] [CrossRef][Green Version]
  25. Hounmanou, Y.M.G.; Bortolaia, V.; Thanh Dang, S.T.; Truong, D.; Olsen, J.E.; Dalsgaard, A. ESBL and AmpC β-Lactamase Encoding Genes in E. coli From Pig and Pig Farm Workers in Vietnam and Their Association with Mobile Genetic Elements. Front. Microbiol. 2021, 12, 629139. [Google Scholar] [CrossRef]
  26. Commission Implementing Decision 2013/652/EU of 12 November 2013 on the monitoring and reporting of antimicrobial resistance in zoonotic and commensal bacteria. Off. J. Eur. Union 2013, L303, 26–39.
  27. Jorgensen, J.H.; Maher, L.A.; Howell, A.W. Activity of meropenem against antibiotic-resistant or infrequently encountered Gram-negative bacilli. Antimicrob. Agents Chemother. 1991, 35, 2410–2414. [Google Scholar] [CrossRef][Green Version]
  28. Neu, H.C.; Novelli, A.; Chin, N.X. In vitro activity and beta-lactamase stability of a new carbapenem, SM-7338. Antimicrob. Agents Chemother. 1989, 33, 1009–1018. [Google Scholar] [CrossRef] [PubMed][Green Version]
  29. Riera, E.; Cabot, G.; Mulet, X.; Garcıa-Castillo, M.; del Campo, R.; Juan, C.; Canton, R.; Oliver, A. Pseudomonas aeruginosa carbapenem resistance mechanisms in Spain: Impact on the activity of imipenem, meropenem and doripenem. J. Antimicrob. Chemother. 2011, 66, 2022–2027. [Google Scholar] [CrossRef] [PubMed]
  30. EUCAST (European Commettee on Antimicrobial Susceptibility Testing). Breakpoint Tables for Interpretations of MICs and Zone Diameters; Version 12.0; EUCAST: Växjö, Sweden, 2021; Available online: (accessed on 3 March 2021).
  31. Klockgether, J.; Cramer, N.; Wiehlmann, L.; Davenport, C.; Tümmler, B. Pseudomonas aeruginosa Genomic Structure and Diversity. Front. Microbiol. 2011, 2, 150. [Google Scholar] [CrossRef][Green Version]
  32. Molina-Mora, J.A.; Campos-Sánchez, R.; Rodríguez, C.; Shi, L.; García, F. High quality 3C de novo assembly and annotation of a multidrug resistant ST-111 Pseudomonas aeruginosa genome: Benchmark of hybrid and non-hybrid assemblers. Sci. Rep. 2020, 10, 1392. [Google Scholar] [CrossRef]
  33. Timme, R.E.; Wolfgang, W.J.; Balkey, M.; Gubbala Venkata, S.L.; Randolph, R.; Allard, M.; Strain, E. Optimizing Open Data to Support One Health: Best Practices to Ensure Interoperability of Genomic Data from Microbial Pathogens. One Health Outlook 2020, 2, 20. [Google Scholar] [CrossRef]
  34. Sims, D.; Sudbery, I.; Ilott, N.E.; Heger, A.; Ponting, C.P. Sequencing depth and coverage: Key considerations in genomic analyses. Nat. Rev. Genet. 2014, 15, 121–132. [Google Scholar] [CrossRef] [PubMed]
  35. Berends, B.R.; Van Knapen, F.; Snijeders, J.M.A.; Mossel, D.A.A. Identification and quantification of risk factors associated with Salmonella contamination on pork carcasses. Int. J. Food Microbiol. 1997, 36, 199–206. [Google Scholar] [CrossRef]
  36. Biasino, W.; De Zutter, L.; Mattheus, W.; Bertrand, S.; Uyttendaele, M.; Van Damme, I. Correlation between slaughter practices and the distribution of Salmonella and hygiene indicator bacteria on pig carcasses during slaughter. Food Microbiol. 2018, 70, 192–199. [Google Scholar] [CrossRef]
  37. Bonardi, S.; Bassi, L.; Brindani, F.; D’Incau, M.; Barco, L.; Carra, E.; Pongolini, S. Prevalence, characterization and antimicrobial susceptibility of Salmonella enterica and Yersinia enterocolitica in pigs at slaughter in Italy. Int. J. Food Microbiol. 2013, 163, 248–257. [Google Scholar] [CrossRef]
  38. EFSA (European Food Safety Authority). Report from the Task Force on Zoonoses Data Collection including guidance for harmonized monitoring and reporting of antimicrobial resistance in commensal Escherichia coli and Enterococcus spp. from food animals. EFSA J. 2008, 6, 141–144. [CrossRef]
  39. Livermore, D.M. Multiple mechanisms of antimicrobial resistance in Pseudomonas aeruginosa: Our worst nightmare? Clin. Infect. Dis. 2002, 34, 634–640. [Google Scholar] [CrossRef][Green Version]
  40. Strateva, T.; Yordanov, D. Pseudomonas aeruginosa—A phenomenon of bacterial resistance. J. Med. Microbiol. 2009, 58, 1133–1148. [Google Scholar] [CrossRef][Green Version]
  41. Wolter, D.J.; Lister, P.D. Mechanisms of β-lactam resistance among Pseudomonas aeruginosa. Curr. Pharm. Des. 2013, 19, 209–222. [Google Scholar] [CrossRef]
  42. Botelho, J.; Grosso, F.; Peixe, L. Antibiotic resistance in Pseudomonas aeruginosa—Mechanisms, epidemiology and evolution. Drug Resist. Updat. 2019, 44, 100640. [Google Scholar] [CrossRef] [PubMed]
  43. Micek, S.T.; Wunderink, R.G.; Kollef, M.H.; Chen, C.; Rello, J.; Chastre, J.; Antonelli, M.; Welte, T.; Clair, B.; Ostermann, H.; et al. An international multicenter retrospective study of Pseudomonas aeruginosa nosocomial pneumonia: Impact of multidrug resistance. Crit. Care 2015, 19, 219. [Google Scholar] [CrossRef][Green Version]
  44. Zilberberg, M.D.; Shorr, A.F. Prevalence of multidrug-resistant Pseudomonas aeruginosa and carbapenem-resistant Enterobacteriaceae among specimens from hospitalized patients with pneumonia and bloodstream infections in the United States from 2000 to 2009. J. Hosp. Med. 2013, 8, 559–563. [Google Scholar] [CrossRef] [PubMed]
  45. WHO Regional Office for Europe and European Centre for Disease Prevention and Control. Surveillance of Antimicrobial Resistance in Europe, 2020 Data. Executive Summary; WHO Regional Office for Europe: Copenhagen, Denmark, 2021. [Google Scholar]
  46. Girlich, D.; Naas, T.; Nordmann, P. Biochemical characterization of the naturally occurring oxacillinase OXA-50 of Pseudomonas aeruginosa. Antimicrob. Agents Chemother. 2004, 48, 2043–2048. [Google Scholar] [CrossRef][Green Version]
  47. Overbeek, R.; Olson, R.; Pusch, G.D.; Olsen, G.J.; Davis, J.J.; Disz, T.; Edwards, R.A.; Gerdes, S.; Parrello, B.; Shukla, M.; et al. The SEED and the Rapid Annotation of microbial genomes using Subsystems Technology (RAST). Nucleic Acids Res. 2014, 42, D206–D214. [Google Scholar] [CrossRef]
  48. OIE (World Organization for Animal Health). OIE List of Antimicrobial Agents of Veterinary Importance. 2018. Available online: (accessed on 21 March 2022).
  49. Leman, A.D.; Straw, B.E.; Mengeling, W.L.; Sylvie, D.; Taylor, D.J. Diseases of Swine, 7th ed.; Iowa State University Press: Ames, Iowa, 1992. [Google Scholar]
  50. Miniats, O.P.; Johnson, J.A. Experimental atrophic rhinitis in gnotobiotic pigs. Can. J. Comp. Med. 1980, 44, 358–365. Available online: (accessed on 10 April 2022).
  51. Baljer, G.; Barrett, J.T. Nachweis von enterotoxinbildenden Pseudomonas aeruginosa-Stämmen im Darmligaturtest beim Ferkel. J. Vet. Med. 2010, 26, 740–747. [Google Scholar] [CrossRef]
  52. ECDC (European Centre for Disease Prevention and Control). Surveillance of Antimicrobial Resistance in Europe, 2017 Data. Annual Report of the European Antimicrobial Resistance Surveillance Network (EARS-Net) 2017; ECDC: Stockholm, Sweden, 2018.
  53. Lautenbach, E.; Synnestvedt, M.; Weiner, M.G.; Bilker, W.B.; Vo, L.; Schein, J.; Kim, M. Imipenem resistance in Pseudomonas aeruginosa: Emergence, epidemiology, and impact on clinical and economic outcomes. Infect Control. Hosp. Epidemiol. 2010, 31, 47–53. [Google Scholar] [CrossRef]
  54. Venditti, C.; Butera, O.; Proia, A.; Rigacci, L.; Mariani, B.; Parisi, G.; Messina, F.; Capone, A.; Nisii, C.; Di Caro, A. Reduced susceptibility to carbapenems in a Klebsiella pneumoniae clinical isolate producing SCO-1 and CTX-M-15 β lactamases together with OmpK35 and OmpK36 porin deficiency. Antimicrob. Agents Chemother. 2020, 64, e00556-20. [Google Scholar] [CrossRef] [PubMed]
  55. Wise, M.G.; Horvath, E.; Young, K.; Sahm, D.F.; Kazmierczak, K.M. Global survey of Klebsiella pneumoniae major porins from ertapenem non-susceptible isolates lacking carbapenemases. J. Med. Microbiol. 2018, 67, 289–295. [Google Scholar] [CrossRef]
  56. Andersen, V.D.; Jensen, V.F.; Vigre, H.; Andreasen, M.; Agersø, Y. The use of third and fourth generation cephalosporins affects the occurrence of extended-spectrum cephalosporinase-producing Escherichia coli in Danish pig herds. Vet. J. 2015, 204, 345–350. [Google Scholar] [CrossRef] [PubMed]
  57. Pauly, N.; Hammerl, J.A.; Grobbel, M.; Käsbohrer, A.; Tenhagen, B.A.; Malorny, B.; Schwarz, S.; Meemken, D.; Irrgang, A. Identification of a bla(VIM-1)-Carrying IncA/C(2) Multiresistance Plasmid in an Escherichia coli Isolate Recovered from the German Food Chain. Microorganisms 2020, 9, 29. [Google Scholar] [CrossRef]
  58. Irrgang, A.; Tausch, S.H.; Pauly, N.; Grobbel, M.; Kaesbohrer, A.; Hammerl, J.A. First Detection of GES-5-Producing Escherichia coli from Livestock-An Increasing Diversity of Carbapenemases Recognized from German Pig Production. Microorganisms 2020, 8, 1593. [Google Scholar] [CrossRef]
  59. Irrgang, A.; Pauly, N.; Tenhagen, B.A.; Grobbel, M.; Kaesbohrer, A.; Hammerl, A.J.A. Spill-Over from Public Health? First Detection of an OXA-48-Producing Escherichia coli in a German Pig Farm. Microorganisms 2020, 8, 855. [Google Scholar] [CrossRef]
  60. Diaconu, E.L.; Carfora, V.; Alba, P.; Di Matteo, P.; Stravino, F.; Buccella, C.; Dell’Aira, E.; Onorati, R.; Sorbara, L.; Battisti, A.; et al. Novel IncFII plasmid harbouring blaNDM-4 in a carbapenem-resistant Escherichia coli of pig origin, Italy. J. Antimicrob. Chemother. 2020, 75, 3475–3479. [Google Scholar] [CrossRef]
  61. Rega, M.; Carmosino, I.; Bonilauri, P.; Frascolla, V.; Vismarra, A.; Bacci, C. Prevalence of ESβL, AmpC and Colistin-Resistant, E. coli in Meat: A Comparison between Pork and Wild Boar. Microorganisms 2021, 9, 214. [Google Scholar] [CrossRef]
  62. Hassan, S.; Amer, S.; Mittal, C.; Sharma, R. Ewingella americana: An emerging true pathogen. Case Rep. Infect. Dis. 2012, 2012, 730720. [Google Scholar] [CrossRef][Green Version]
  63. Meisler, S.; Kamity, R.; Noor, A.; Krilov, L.; Tiozzo, C. First Case of Ewingella americana Meningitis in a Term Newborn: A Rare but Real Pathogen. Front. Pediatr. 2020, 8, 308. [Google Scholar] [CrossRef]
  64. Esteban, J.; Martin, J.; Ortiz, A.; Santos-O’Connor, F.; Cabria, F.; Reyero, A. Pseudomonas oryzihabitans peritonitis in a patient on continuous ambulatory peritoneal dialysis. Clin. Microbiol. Infect. 2002, 8, 607–608. [Google Scholar] [CrossRef][Green Version]
  65. Nei, T.; Sonobe, K.; Onodera, A.; Itabashi, T.; Yamaguchi, H.; Maeda, M.; Saito, R. Two cases with bacteremia suspected to be due to relatively rare Pseudomonas (Flavimonas) oryzihabitans. J. Infect. Chemother. 2015, 21, 751–755. [Google Scholar] [CrossRef]
  66. Govan, J.R.; Hughes, J.E.; Vandamme, P. 19 Burkholderia cepacia: Medical, taxonomic and ecological isues. J. Med. Microbiol. 1996, 45, 395–407. [Google Scholar] [CrossRef][Green Version]
  67. Mukerji, R.; Kakarala, R.; Smith, S.J.; Kusz, H.G. Chryseobacterium indologenes: An emerging infection in the USA. BMJ Case Rep. 2016, 2016, bcr2016214486. [Google Scholar] [CrossRef][Green Version]
  68. Poole, T.L.; Schlosser, W.D.; Anderson, R.C.; Norman, K.N.; Beier, R.C.; Nisbet, D.J. Whole-Genome Sequence of Aeromonas hydrophila CVM861 Isolated from Diarrhetic Neonatal Swine. Microorganisms 2020, 8, 1648. [Google Scholar] [CrossRef]
  69. Igbinosa, I.H.; Igbinosa, E.O.; Okoh, A.I. Antibiogram characterization and putative virulence genes in Aeromonas species isolated from pig fecal samples. Environ. Sci. Pollut. Res. Int. 2016, 23, 12199–12205. [Google Scholar] [CrossRef] [PubMed]
  70. Janda, J.M.; Abbott, S.L. The Genus Aeromonas: Taxonomy, Pathogenicity, and Infection. Clin. Micro. Rev. 2010, 23, 35–73. [Google Scholar] [CrossRef][Green Version]
  71. Manfredi, R.; Nanetti, A.; Ferri, M.; Mastroianni, A.; Coronado, O.V.; Chiodo, F. Flavobacterium spp. organisms as opportunistic bacterial pathogens during advanced HIV disease. J. Infect. 1999, 39, 146–152. [Google Scholar] [CrossRef]
  72. Brooke, J.S. Stenotrophomonas maltophilia: An emerging global opportunistic pathogen. Clin. Microbiol. Rev. 2012, 25, 2–41. [Google Scholar] [CrossRef][Green Version]
  73. Abbott, I.J.; Slavin, M.A.; Turnidge, J.D.; Thursky, K.A.; Worth, L.J. Stenotrophomonas maltophilia: Emerging disease patterns and challenges for treatment. Expert Rev. Anti. Infect. Ther. 2011, 9, 471–488. [Google Scholar] [CrossRef] [PubMed]
  74. Ibn Saied, W.; Merceron, S.; Schwebel, C.; Le Monnier, A.; Oziel, J.; Garrouste-Orgeas, M.; Marcotte, G.; Ruckly, S.; Souweine, B.; Darmon, M.; et al. Ventilator-associated pneumonia due to Stenotrophomonas maltophilia: Risk factors and outcome. J. Infect. 2020, 80, 279–285. [Google Scholar] [CrossRef]
  75. Marchaim, D.; Chopra, T.; Perez, F.; Hayakawa, K.; Lephart, P.R.; Bheemreddy, S.; Blunden, C.; Hujer, A.M.; Rudin, S.; Shango, M.; et al. Outcomes and genetic relatedness of carbapenem-resistant Enterobacteriaceae at Detroit medical center. Infect. Control. Hosp. Epidemiol. 2011, 32, 861–871. [Google Scholar] [CrossRef][Green Version]
  76. Xu, L.; Sun, X.; Ma, X. Systematic review and meta-analysis of mortality of patients infected with carbapenem-resistant Klebsiella pneumoniae. Ann. Clin. Microbiol. Antimicrob. 2017, 16, 18. [Google Scholar] [CrossRef] [PubMed][Green Version]
  77. DTU (Technical University of Denmark—National Food Institute). Laboratory Protocol—Isolation of ESBL, AmpC- and Carbapenemase-Producing E. coli from Caecal Samples; Version 5; DTU: Kongens Lyngby, Denmark, 2017; Available online: (accessed on 1 March 2022).
  78. EUCAST (European Committee on Antimicrobial Susceptibility Testing). EUCAST Disc Diffusion Test Methodology. 2017. Available online: (accessed on 30 November 2017).
  79. EUCAST (European Committee on Antimicrobial Susceptibility Testing). Breakpoint Tables for Interpretations of MICs and Zone Diameters, Version 8.0. 2017. Available online: (accessed on 30 November 2017).
  80. EUCAST (European Committee on Antimicrobial Susceptibility Testing). EUCAST Reading Guide for Broth Microdilution. 2021. Available online: (accessed on 3 March 2021).
  81. Adeolu, M.; Alnajar, S.; Naushad, S.; Gupta, R.S. Genome-based phylogeny and taxonomy of the ‘Enterobacteriales’: Proposal for Enterobacterales ord. nov. divided into the families Enterobacteriaceae, Erwiniaceae fam. Nov., Pectobacteriaceae fam. Nov., Yersiniaceae fam. Nov., Hafniaceae fam. Nov., Morganellaceae fam. Nov., and Budviciaceae fam Nov. Int. J. Syst. Evol. Microbiol. 2016, 65, 5575–5599. [Google Scholar] [CrossRef]
  82. CDC (Center for Disease Control and Prevention). Laboratory Protocol for Detection of Carbapenem-Resistant or Carbapenemase-Producing Klebsiella spp. and E. coli from Rectal Swabs; CDC: Atlanta, GA, USA, 2009.
  83. Doyle, D.; Peirano, G.; Lascols, C.; Lloyd, T.; Church, D.L.; Pitout, J.D. Laboratory detection of Enterobacteriaceae that produce carbapenemases. J. Clin. Microbiol. 2012, 50, 3877–3880. [Google Scholar] [CrossRef][Green Version]
  84. Roschansky, N.; Fischer, J.; Guerra, B.; Roesler, U. Development of a Multiplex Real-Time PCR for the rapid detection of the predominant Beta-Lactamase genes CTX-M, SHV, TEM and CIT type AmpCs in Enterobacteriaceae. PLoS ONE 2014, 9, e100956. [Google Scholar] [CrossRef] [PubMed]
  85. Pérez-Pérez, F.J.; Hanson, N.D. Detection of plasmid-mediated AmpC—Lactamase genes in clinical isolates by using Multiplex PCR. J. Clin. Microbiol. 2002, 40, 2153–2162. [Google Scholar] [CrossRef] [PubMed][Green Version]
  86. INNUca. 2021. Available online: (accessed on 1 December 2021).
  87. Contig_info. 2022. Available online: (accessed on 15 May 2022).
  88. Snippy. 2021. Available online: (accessed on 1 December 2021).
  89. FastANI. 2022. Available online: (accessed on 15 May 2022).
  90. RAxML. 2022. Available online: (accessed on 15 May 2022).
  91. Itol. 2021. Available online: (accessed on 1 December 2021).
  92. ChewBBACA. 2022. Available online: (accessed on 15 May 2022).
  93. de Sales, R.O.; Migliorini, L.B.; Puga, R.; Kocsis, B.; Severino, P. A core genome multilocus sequence typing scheme for Pseudomonas aeruginosa. Front. Microbiol. 2020, 11, 1049. [Google Scholar] [CrossRef] [PubMed]
  94. Phyloviz. 2022. Available online: (accessed on 15 May 2022).
  95. ABRicate. 2021. Available online: (accessed on 1 December 2021).
  96. Center for Genomic Epidemiology. 2021. Available online: (accessed on 9 March 2021).
  97. Prokka. 2022. Available online: (accessed on 15 May 2022).
  98. SnapGene. 2021. Available online: (accessed on 1 December 2021).
  99. National Center for Biotechnology Information. 2021. Available online: (accessed on 1 December 2021).
Figure 1. Phylogenetic trees showing genetic relationships among P. aeruginosa genomes included in this study: (A) core SNPs maximum likelihood tree (GTRGAMMA model) including the reference P. aeruginosa PAO1 (Ref Seq NC_002516.2), with bootstrap support labelled above branches; (B) cgMLST minimum spanning tree, in red the number of allelic variants.
Figure 1. Phylogenetic trees showing genetic relationships among P. aeruginosa genomes included in this study: (A) core SNPs maximum likelihood tree (GTRGAMMA model) including the reference P. aeruginosa PAO1 (Ref Seq NC_002516.2), with bootstrap support labelled above branches; (B) cgMLST minimum spanning tree, in red the number of allelic variants.
Antibiotics 11 00777 g001
Figure 2. Genetic environment of blaOXA-486 gene in CRE 98 (ST274). The same genetic environment was observed for all detected genes belonging to the OXA-50 family in NEF 23 (ST938), CRE 102 (ST938), CRE 153 (ST782), CRE 295 (ST885), and NEF 156 (ST395) genomes.
Figure 2. Genetic environment of blaOXA-486 gene in CRE 98 (ST274). The same genetic environment was observed for all detected genes belonging to the OXA-50 family in NEF 23 (ST938), CRE 102 (ST938), CRE 153 (ST782), CRE 295 (ST885), and NEF 156 (ST395) genomes.
Antibiotics 11 00777 g002
Figure 3. Genetic environment of blaPAO gene in CRE 98 (ST274) genome. The same genetic environment was observed in NEF 23 (ST938), CRE 102 (ST938), CRE 153 (ST782), CRE 295 (ST885), and NEF 156 (ST395) genomes.
Figure 3. Genetic environment of blaPAO gene in CRE 98 (ST274) genome. The same genetic environment was observed in NEF 23 (ST938), CRE 102 (ST938), CRE 153 (ST782), CRE 295 (ST885), and NEF 156 (ST395) genomes.
Antibiotics 11 00777 g003
Table 1. MIC values for meropenem (MEM), cefotaxime (CTX), ceftazidime (CAZ), and resistant genes tested with PCR. MICs indicative of resistance for Enterobacterales, Pseudomonas spp., and Acinetobacter spp. are shown in bold. MICs higher than the meropenem screening breakpoint (ECOFF) are shown in Italics.
Table 1. MIC values for meropenem (MEM), cefotaxime (CTX), ceftazidime (CAZ), and resistant genes tested with PCR. MICs indicative of resistance for Enterobacterales, Pseudomonas spp., and Acinetobacter spp. are shown in bold. MICs higher than the meropenem screening breakpoint (ECOFF) are shown in Italics.
SpeciesMIC Values (Lg/mL)bla GenesampC Genes
C. freundii0.01628TEM-1CIT
E. agglomerans0.032128512CTX-M-1, TEM-1
E. coli4≤0.5≤0.5TEM-1
E. coli0.0160.50.5TEM-1
E. coli0.01684CTX-M-1, TEM-1
E. coli0.01632512TEM-1, SHV
E. americana43216CTX-M-1, TEM-1
Pseudomonas (no breakpoints for CTX)
P. oryzihabitans25625632TEM-1
Acinetobacter (no breakpoints for CAZ and CTX)
A. lwoffii0.0160.58TEM-1
Species with no breakpoints
A. hydrophila43264CTX-M-1, TEM-1
A. hydrophila420.5TEM-1
B. cepacia4816TEM-1
B. cepacia81664CTX-M-1, TEM-1, SHV
B. cepacia81664CTX-M-1, TEM-1
C. indologenes16512256TEM-1
F. odoratum161664TEM-1
S. maltophilia12864256TEM-1
S. maltophilia6432256TEM-1EBC
S. maltophilia64864TEM-1EBC
S. maltophilia6464256TEM-1ACC
S. maltophilia646464TEM-1CIT
S. maltophilia64128128CTX-M-1, TEM-1CIT
S. maltophilia64128256TEM-1CIT
S. maltophilia3216256TEM-1CIT
S. maltophilia3264256CTX-M-1, TEM-1CIT
S. maltophilia32128256CTX-M-1, TEM-1CIT
S. maltophilia3264256CTX-M-1, TEM-1CIT
S. maltophilia12864256TEM-1CIT
S. maltophilia128464TEM-1CIT
S. maltophilia161664TEM-1CIT
S. maltophilia16128512TEM-1CIT
S. maltophilia864128TEM-1
S. maltophilia4216TEM-1CIT
S. maltophilia12128TEM-1
Table 2. Results from MIC testing and WGS of P. aeruginosa strains isolated from porcine and human sources. MICs indicative of resistance to meropenem (MEM) are in bold (EUCAST, 2021).
Table 2. Results from MIC testing and WGS of P. aeruginosa strains isolated from porcine and human sources. MICs indicative of resistance to meropenem (MEM) are in bold (EUCAST, 2021).
SourceID CodeMIC Values (µg/mL)Multi Locus
Sequence Typing
bla GenesAdditional Resistance Genes
pigCRE 982274OXA-486, PAOaph(3′)-IIb, crpP, fosA4, catB7
pigCRE 10216938OXA-396, PAOaph(3′)-IIb, fosA4, catB7
pigCRE 15316782OXA-50, PAOaph(3′)-IIb, crpP, fosA4, catB7
pigCRE 2952885OXA-50, PAOaph(3′)-IIb, crpP, fosA4, catB7
humanNEF 2316938OXA-396, PAOaph(3′)-IIb, fosA4, catB7
humanNEF 1568395OXA-488, PAOaph(3′)-IIb, crpP, fosA4, catB7
Table 3. Assembly statistics of sequenced genomes of P. aeruginosa.
Table 3. Assembly statistics of sequenced genomes of P. aeruginosa.
SourceGenome SizeGC%No. of ContigCoverageN50Maximum
Contig Length
NEF 23human6,436,45066.4020192.579,626377,949
CRE 98pig6,415,66466.4012499.8126,411561,477
CRE 102pig6,438,08866.4022576.675,398238,923
CRE 153pig6,396,23466.4331779.238,674223,278
CRE 295pig6,426,08366.35141105.2102,638328,392
NEF 156human7,099,70565.8517285.9123,256340,617
Publisher’s Note: MDPI stays neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Back to TopTop