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Apramycin treatment affects selection and spread of a multidrug-resistant Escherichia coli strain able to colonize the human gut in the intestinal microbiota of pigs


The effect of apramycin treatment on transfer and selection of an Escherichia coli strain (E. coli 912) in the intestine of pigs was analyzed through an in vivo experiment. The strain was sequenced and assigned to the sequence type ST101 and serotype O11. It carried resistance genes to apramycin/gentamicin, sulphonamide, tetracycline, hygromycin B, β-lactams and streptomycin [aac(3)-IV, sul2, tet(X), aph(4), bla TEM-1 and strA/B], with all but tet(X) located on the same conjugative plasmid. Nineteen pigs were randomly allocated into two inoculation groups, one treated with apramycin (pen 2) and one non-treated (pen 3), along with a non-inoculated control group (pen 1). Two pigs of pen 2 and 3 were inoculated intragastrically with a rifampicin resistant variant of the strain. Apramycin treatment in pen 2 was initiated immediately after inoculation. Strain colonization was assessed in the feces from all pigs. E. coli 912 was shown to spread to non-inoculated pigs in both groups. The selective effect did not persist beyond 3 days post-treatment, and the strain was not detected from this time point in pen 2. We demonstrated that E. coli 912 was able to spread between pigs in the same pen irrespective of treatment, and apramycin treatment resulted in significantly higher counts compared to the non-treated group. This represents the first demonstration of how antimicrobial treatment affects spread of resistant bacteria in pig production. The use of apramycin may lead to enhanced spread of gentamicin-resistant E. coli. Since gentamicin is a first-choice drug for human bacteremia, this is of concern.


During the last 50 years, antibiotics have been used to treat infections in both human and veterinary medicine. In this period, use of antimicrobials has caused selective evolutionary pressures, resulting in the emergence of antimicrobial resistant bacteria [1], which in turn have caused treatment failure and increased morbidity [2]. The natural gut microbiota, consisting of commensal bacteria, represents an important reservoir for the development of antimicrobial resistance (resistome), and continuous antibiotic use could lead to the emergence of clinically problematic strains [3].

Multi-drug resistant E. coli isolates from humans and pigs have been reported worldwide [47]. These multi-drug resistant isolates harbor antimicrobial resistance (AMR) genes either on the chromosome or on mobile genetic elements, such as plasmids [8]. The presence of AMR genes on plasmids, and their subsequent horizontal transfer via conjugation, can result in their rapid spread among the susceptible bacterial populations [9]. One of the main concerns is the potential transfer of these resistant determinants to pathogenic bacteria which prolongs infections and decreases treatment options as a consequence.

Use of antibiotics in livestock is considered one of the main reasons leading to development of AMR, and such resistant bacteria can be potentially transmitted to the food chain [2]. The role of pigs in AMR transmission to the food chain must be better understood in order to prevent dissemination of multidrug-resistant strains from pigs to humans. In a previous study a multi-drug resistant strain of E. coli isolated from a healthy pig (E. coli 912) [10] was proven to be able to colonize the gut of human volunteers for 35 days [11]. The strain harbored the resistance gene aac(3)-IV conferring resistance to gentamicin/apramycin [11].

Apramycin, which is only approved for animal use, was introduced into veterinary therapy in the early 1980s in several European countries [12]. Several apramycin products were authorized for oral use in production animals in 1998 [13]. The gene aac(3)-IV is the only identified gene causing enzymatic cross-resistance between gentamicin and apramycin [12]. Apramycin resistance associated with the aac(3)-IV gene was initially reported in 1981 in France, and the gene was only found in the animal reservoir [14]. Over the next years aac(3)-IV disseminated rapidly in the animal reservoir in France, Belgium and Great Britain [14]. In 1986, the gene was first detected in Enterobacteriaceae isolated from human patients [15].

Nowadays, apramycin is widely used in farm animals, and resistant E. coli are commonly isolated from diseased pigs [10]. E. coli from pigs may be an important reservoir for transfer of apramycin/gentamicin resistance genes or bacteria to humans. Furthermore, resistance to apramycin and other aminoglycosides is usually transmissible, encoded on conjugative R-plasmids, and often linked to resistance to other antimicrobials [12].

In Denmark, detailed information on aminoglycoside use in food-producing animals is registered in the Danish veterinary drug-monitoring programme, VetStat [16]. This database contains information on consumption of all prescription drugs purchased by animal owners or used by veterinarians at farm level, including information on animal species, age group, disease group and farm identity. Importantly, gentamicin is a first-choice drug (in combination with β-lactams) for severe human infections (e.g. sepsis and endocarditis) in Danish Hospitals [17]. Therefore, spread of gentamicin-resistant E. coli strains to humans is of great concern.

Several studies have evaluated the impacts of antimicrobial treatment on selection for resistance [1823], however, only a few reports have considered the impact of treatment on the spread of resistant microorganisms among animals [24, 25]. Here, we quantify for the first time the effect of treatment on the transmission of resistant strains among pigs in vivo. In this study, the effect of apramycin treatment on the selection of the E. coli 912 inoculated into nursery pigs was assessed. Derived results provided information of the consequence of antibiotic treatment in the development and spread of resistant bacteria between pigs in production-like conditions (regular farm conditions), where pigs are housed closely together.

Materials and methods

Animals, housing conditions, and ethical issues

Three to 4 weeks nursery cross-bred sex-mixed pigs with weights ranging from 6 to 9 kg were purchased from a specific-pathogen-free farm in Denmark. The animals were housed in a level 1 isolation unit (individual disinfected pens in a same room of the building) at the Faculty of Health and Medical Sciences, University of Copenhagen and weighed at least once a week. All procedures regarding the animal experiments were carried out in agreement with the Animals Scientific Act and performed under the license and approval of the Danish National Animal Experiment Inspectorate (license no. 2009/561-1675). Occurrence of any clinical sign, such as changes in behavior and decrease in food and water intake, was surveyed twice a day. At the end of the experiment (3 weeks of duration), the animals were euthanized by captive bolt pistol penetration followed by exsanguination.

Bacterial strain

The bacterial strain E. coli 912 used to inoculate the pigs was previously proven to be resistant to gentamicin/apramycin and sulphonamide by determination of minimum inhibitory concentration [10, 11]. It was isolated from the feces of a healthy pig [10, 11]. The strain harbored the genes aac(3)-IV and sul2 on a conjugative plasmid (not shown) [11]. A rifampicin (RIF) resistant mutant was obtained by serial plating on nutrient agar with rifampicin. The RIF-resistance (MIC ≥ 250 μg/mL) was used as a marker to distinguish the inoculated strain from gentamicin/sulphonamide-resistant coliforms that could preexist in the intestinal microbiota or that emerged during the experiment as a result of horizontal gene transfer. Growth of both wild-type and the isogenic RIF-resistant mutant strain was analysed and compared. The isolates were grown at 37 °C, 200 rpm for 16 h in Luria–Bertani broth before sub-culturing into fresh media at a 40 fold dilution and further grown with assessments every 15 min for 18 h using Bioscreen C. Growth curves were obtained (Additional file 1).

Whole genome sequencing, analysis of genome sequence for virulence, resistance, serotype, plasmid associated genes, and multilocus sequence typing (MLST)

Genomic DNA was extracted from the isolate E. coli 912 using the Invitrogen Easy-DNATM Kit (Invitrogen) and DNA concentrations were determined using the Qubit dsDNA BR assay kit (Invitrogen). The genomic DNA was prepared for Illumina pair-end sequencing using the Illumina (Illumina) NexteraXT® Guide 150319425031942 following the protocol revision C [26]. A sample of the pooled NexteraXT Libraries was loaded onto an Illumina MiSeq reagent cartridge using MiSeq Reagent Kit v2 and 500 cycles with a Standard Flow Cell. The libraries were sequenced using an Illumina platform and MiSeq Control Software The isolate was pair-end sequenced.

The raw reads were assembled using the Assemble pipeline (version 1.0) available from the Center for Genomic Epidemiology (CGE) [27] which is based on the Velvet algorithms for de novo short reads assembly. The assembled genome was submitted and annotated at NCBI [28] under accession number JWJM00000000.

The assembled sequences were analyzed to confirm the species and E. coli serotype using the CGE pipelines; K-merFinder (version 2) [29] and SeroTypeFinder (version 1.1). Following the confirmation, the MLST sequence type (ST) for E. coli, plasmid replicons, and acquired antimicrobial resistance genes, and virulence genes were identified with a selected threshold equal to 98% identity using the pipelines; MLST (version 1.8) [30], PlasmidFinder (version 1.3) [31], ResFinder (version 2.1) [32], and VirulenceFinder (version 1.4) [33] also available from CGE.

Plasmid analysis and Southern blot

Plasmid DNA from E. coli 912 was isolated with the MidiPrep plasmid kit (Invitrogen) following the protocol suggested by the manufacturer. DIG-labelled DNA molecular weight marker II (Roche) was used as molecular size standard and control in Southern blot hybridization. The obtained plasmid profile was subsequently hybridized with probes specific for the sul2, aac(3)-IV, tet(X), bla TEM-1 and strA/B genes by using the kit DIG wash and block buffer set (Roche) and manufacturers indications from the DIG application manual for filter hybridization. The probes were obtained from E. coli 912 by PCR amplification using the PCR DIG labelling mix (Roche). The sequences of the primers used for PCR are listed in Table 1.

Table 1 Primers used in this study.

Challenge experimental setup

Pigs were divided into three groups housed in three well-separated pens avoiding any contact among pigs from different pens. Only airflow between pens was possible. The untreated control group (n = 3) was isolated in pen 1. The two inoculated groups, group 2 (pen 2) and group 3 (pen 3) included eight pigs each. After 1 week of acclimatization, two pigs from each of groups 2 and 3 were inoculated with 109 CFU/mL of the E. coli 912 strain suspended in 10 mL of a saline suspension using an endogastric tube after sedation. The four inoculated pigs were isolated in an individual pen for 2 days in order to allow the bacterial colonization of the gut and then replaced in their original groups.

The antimicrobial drug, Apralan Vet 10% solution, was purchased as veterinary medical product. All pigs in group 2 were individually treated with 5 mg/kg of the antibiotic after the replacement of the two previously inoculated pigs, and the antimicrobial product was administered once a day for 3 days orally in nutri-drink ensuring that everything was taken up. The administration was performed according to the standard treatment recommended when administering the drug product in pigs.

Collection and microbiological analysis of fecal samples

Fecal samples of about 5 g were collected from the rectum of all the pigs prior to inoculation of the strain (day −2), 1 day after inoculation (day −1), prior to antimicrobial treatment in pen 2 (day 0) and on days 2, 4, 6, 8, and 10 after day 0 (days corresponding last day of treatment-day 2- and 2, 4, 6 and 8 days after the end of the treatment). Except for day −1, where CFU counts were only performed for the four inoculated pigs, fecal samples were taken from all the 19 pigs and CFU counts were carried out. Serial tenfold dilutions were used to count the numbers of colony forming (CFU) coliforms on MacConkey agar (Merck), CFU of RIF-resistant coliforms on MacConkey agar supplemented with 50 μg/mL RIF, and CFU of the inoculated sulphonamide-gentamicin/apramycin (SUL-GEN/APRA) resistant strain on MacConkey agar supplemented with 50 μg/mL RIF, 150 μg/mL SUL and 25 μg/mL GEN. All counts were determined by the spot method [34]. Briefly, 30 μL of each dilution was inoculated as a spot in duplicate (on two plates containing every specific antibiotic or combination, and without antibiotic), followed by 24 h of incubation at 37 °C. This method allowed the detection of the coliforms and the quantification of the coliforms at greater than or equal to 500 CFU/g (2.7 log CFU/g) of feces.

On all days except -1, colonies were isolated from the selective plates containing RIF or RIF-SUL-GEN. All isolates were identified as E. coli by the indole, methyl red, Voges-Proskauer, and citrate tests. Isolates confirmed to be E. coli were tested for the presence of the aac(3)-IV gene by PCR (Table 1). In order to enable a comparison of the isolates obtained at different time points and the inoculated strain, all the RIF or RIF-SUL-GEN resistant isolates obtained from each animal of each group at all the sampling times were further characterized by pulsed-field gel electrophoresis (PFGE) with XbaI (Roche) digestion as previously described [35].

Statistical analysis

The log CFU counts were compared by one-way ANOVA with pair-wise comparison of means at the different time points using Tukey’s multiple comparison test, while accounting for repeated measurements. A P value <0.05 was considered significant.

All occurrences in the individual pig on specific test days were further dichotomized (above or below detection level), which also enabled the estimation of incidence and recovery rates. For each of the time periods 0–2, 2–4, 4–6, 6–8 and 8–10 days post inoculation, the incidence rate (IR) was estimated using the formula [36]:

$$ IR = \frac{no.\;of\;cases}{{\left( {no.\;of\;pigs\;at\;risk\;at\;start\;of\;study\;period\; - \;0.5\; \times \;no.\;of\;pigs\;aquiring\;resistance\;in\;period} \right)\; \times \;time}} $$

The recovery rates (RR) were calculated similarly:

$$ RR = \frac{no.\;of\;recovered}{{\left( {no.\;of\;pigs\;at\;without\;resistance \;at\;start\;of\;study\; - \;0.5\; \times \;no.\;of\;pigs\;losing\;resistance\;in\;period} \right)\; \times \;time}} $$


Traits of the strain E. coli 912

First the inoculated strain E. coli 912 was characterized in order to obtain information that could explain its high ability to colonize the gut of humans, as reported [11]. The strain was sequenced and found to contain additional resistance genes to the ones previously reported [11]. The additional genes encoded resistance to tetracycline [tet(X)], hygromycin B [aph(4)], β-lactams (bla TEM-1) and streptomycin (strA/B). This genotype complied with the phenotypic resistance results. The strain was shown to belong to MLST-type ST101 and serotype O11:H12. E. coli 912 also harbored the virulence genes mchB, mchF, mcmA (involved in microcin synthesis) iroN (iron uptake), tsh (hemoglobin binding protease), cnf1 (toxin synthesis), lpfA, prfB (fimbriae synthesis) and iss (increased serum survival) (Table 2) and two plasmids belonging to the incompatibility groups incF1 and incFII. Since genome sequencing did not reveal information about the location of the resistance genes, plasmid purification followed by Southern blot hybridization was performed. Results showed that the genes aph(4), bla TEM-1 and strA/B were plasmid located as it was previously found for sul2 and acc(3)-IV [11]. Furthermore, all the five genes were harbored in the same resistance plasmid (not shown).

Table 2 Features of the strain. E. coli 912.

A growth curve for each of the strains was obtained through in vitro studies and growth was not significantly different between the mutant and WT strains reaching the stationary phase after approximately 6–8 h post-inoculation (Additional file 1).

The influence of apramycin treatment on spread and selection of the tested strain

All experimental animals maintained good health status throughout the experiment, and their weights increased from 6–9 kg to 12–16 kg (average daily weight gain, 309 ± 0.052 g). The outline of the study is shown in Additional file 3 with the status of the individual pig at each time point. No significant differences in the average counts of total coliforms were observed between the treated group, the non-treated group and the control group (Figure 1A). Prior to inoculation, the feces of the 19 pigs did not contain neither RIF nor RIF-SUL-GEN resistant strains (strains growing after 18 h of growth at 37 °C). The counts of RIF and RIF-SUL-GEN resistant coliforms were significantly higher in the treated group (pen 2) than in the non-treated group (pen 3) from day 2 to day 6 after day 0 (start of treatment) (Figure 1B). The effect of treatment was evident until day 6 (4 days after the end of treatment which corresponded to day 2) and the highest peak was reached on the last day of treatment (2 days after day 0) (Figures 1B and C; Additional file 3). A higher number of pigs (up to seven out of eight-treated group vs. two out of eight-untreated group) tested positive for the strain when apramycin was administered (pen 2) (Additional file 3). Using plates with RIF-SUL-GEN for detection, the strain was observed in five and three pigs in the treated and the untreated group (Additional file 3B), respectively, while seven vs. four pigs were shown to excrete the strain when only RIF was used in the plate (Additional file 3A). RIF-SUL-GEN-positive strains were not recovered after day 6 (compared to day 0) in both groups, except that E. coli 912 was found in two pigs from pen 3 (untreated group) when only RIF was used for selection (Figure 1B; Additional file 3) on day 8 (with regards to day 0) but at very low numbers (<1 × 103 cfu/mL). The presence of E. coli 912 was confirmed by PFGE. Thirty-six RIF and 36 RIF-SUL-GEN resistant isolates from days 0 (when the treatment was started and corresponding only to the inoculated pigs), 2 (last day of treatment), 4 (2 days after the end of treatment), 6 (4 days after the end of treatment) and 8 (6 days after the end of treatment) were identified as E. coli, and the presence of aac(3)-IV in all of them was confirmed by PCR. All isolates had the same XbaI-profile by PFGE, which corresponded to the profile of E. coli 912 (Additional file 2), thereby confirming that the counts on these selective agar plates were representative of the inoculated strain. None of the pigs in the unexposed groups showed RIF or RIF-SUL-GEN resistant bacteria.

Figure 1

Mean counts [log(x + 1) CFU/g] of coliforms. Counts of total coliforms (A), RIF-resistant coliforms (RIF-res) (B), and RIF-GEN-SUL-resistant coliforms (RIF-GEN-SUL-res) (C) in feces of pigs treated with apramycin, feces of untreated pigs and feces of pigs non-treated and non-inoculated (control). The vertical dashed lines indicate the treatment period (days 0–2) and the post treatment window (days 3–10). The horizontal dashed lines indicate the detection limit of the method used (500 CFU/g).

The resulting incidence and recovery rates are displayed in Figures 2A and B, respectively. The specific rates are listed in Table 3. The incidence rate was high in the first time step for both RIF and RIF-GEN-SUL (Figure 2A), but 0 in both control groups. Recovery appeared almost identical in all groups, irrespective of the time points (Figure 2B). Statistical testing was not done because there was only one pen with each treatment and the separation in resistant and non-resistant counts was reasonably clear. Even though no significant difference was identified, the spread of E. coli 912 among pigs in the Apramycin treated group appeared higher than in the not treated group (Additional file 3).

Figure 2

Incidence and recovery rates. Incidence rates (A) and recovery rates (B) for the different time periods, control groups and experiments.

Table 3 Incidence rates (IR) and recovery rates (RR) for each time step in the treatment group and the control group


There is overwhelming evidence that the continuous use of antibiotics in food animals increases the number of resistant bacteria in their intestine [5, 6, 8, 1823]. However, it remains to be shown whether this is caused by selection of resistant bacteria, already present in treated animals only, or whether treatment also promotes colonization of more animals with resistant bacteria. This has not been previously analyzed in pigs, and it represented the main goal of the present work.

In a previous study the strain E. coli 912, of pig origin, was orally administered to human volunteers and results showed that, even though the sulphonamide resistance encoded by the isolate was not found to be transferred to the commensal microbiota, the strain was able to colonize the human gut. It was also proven that once in the intestine, the bacteria could survive for a long period, enabling the possible transfer of resistance genes to the commensal bacteria in the gastrointestinal human tract [11]. In this study we analyzed the potential spread of the same strain during an in vivo experiment in pigs treated and non-treated with apramycin in order to elucidate how the selection force of antibiotic treatment affects spread of resistant bacteria. The plasmid-located gene responsible for apramycin resistance in this strain was aac(3)-IV. The experiment was performed only once, which represents a study limitation, and therefore the statistical assessment carried out can be only descriptive in nature. The incidence rates appeared lower in the non-treated groups compared to the treated groups (Table 2), however, no statistical testing could be performed to confirm the trend. A larger-scale study including more animals per group would be required to prove whether the incidence rates are indeed different. Recovery did not appear to be different, which is an effect of the removal of the antimicrobial.

Results from our study revealed selection from treatment with apramycin in the intestinal microbiota of treated pigs, leading to significantly higher counts of resistant strains than in pigs that did not receive the antibiotic. On average, selection resulted in differences in CFU of E. coli 912 in the feces of apramycin-treated and non-treated pigs of around 100-fold. Unlike reported by Trobos et al. [11] for human volunteers, we found that the strain was relatively poor in colonizing the gut of the pigs, in the sense that the peak in CFU was reached already on day 3 of treatment (day 2) in both groups. Several factors might have contributed to the rapid loss of E. coli 912. Even though the rifampicin resistance mutation does not affect the fitness of the mutant strain “in vitro”, there could be a fitness cost “in vivo” due to this mutation as previously described [37]. Further experiments where both wild type and RIF-R strains are administered to pigs should be performed in order to elucidate this premise. It has previously been observed that predominant E. coli clones normally associated with the individual intestinal microbiota make it difficult for introduced strains to establish themselves permanently [3842]. Interestingly, in a previous study performed in calves, natural conjugative apramycin resistance plasmid isolated from commensal organisms of newborn calves was found to confer a fitness advantage on new hosts cells [43]. However, the methodology in the current study did not allow for estimation of plasmid transfer to other bacteria. Cavaco et al. [34] also demonstrated that the administration of several β-lactams (ceftiofur, cefquinome and amoxicillin) led to significantly higher counts of antimicrobial resistant strains compared to the control group. However, contrary to our results, the study which was set up very similar to ours, showed that the selective effects exerted by these antibiotics persisted for longer periods and cefotaxime-nalidixic resistant strains were detected up to 15–20 days after inoculation of the strain in all the groups, no matter whether the antibiotic was administered or not.

In a previous study it was concluded that apramycin administration is most probably driving the increasing occurrence of apramycin/gentamicin cross-resistance in swine [44]. Moreover, this increasing occurrence in animals is of concern and should be under close surveillance. Resistance to apramycin and gentamicin in Enterobacteriaceae and other enteric pathogens usually remains low in pigs at slaughter and in food at retail [44]. Notably, several studies from Great Britain have shown that ca. 26% of the gentamicin-resistant pathogenic E. coli strains from humans were carrying the aac(3)-IV gene [45, 46].

Strain E. coli 912 has now been well characterized with respect to colonization of both pigs and humans, which might make it a suitable challenge strain in studies on aspects of E. coli microbiota of pigs. To deeply study the main features of this strain whole genome sequencing was performed. Apart from the genes aac(3)-IV and sul2, sequencing revealed that the strain also harbored the genes bla TEM-1, strA/B, aph(4) and tet(X). Southern blot hybridization analysis showed that all the resistance genes but tet(X) were carried in the same plasmid that was proven to be conjugative (not shown). Thus, treatment with any of the antibiotics for which the strain is resistant may co-select for the selection and spread of all the resistance genes as a whole since they can be transmitted within the same transferable element. With this knowledge, this strain also constitutes a suitable candidate for studies of how resistance plasmids contribute to the distribution of resistance genes in the intestine, as well as for the analysis of rates and mechanisms of transfer of such plasmids.

Whole genome sequencing also revealed that E. coli 912 harbors virulence genes, encoding functions related to microcin synthesis (mchB/C/F and mcmA), toxin production (cnf1), fimbriae synthesis (lpfA, prfb), iron uptake (iroN), increased serum survival (iss) and hemoglobin-binding protease (tsh) (Table 2). Since virulence genes responsible for pathogenicity are often located on transmissible genetic elements [47], E. coli 912 may represent a source of such virulence determinants, which could disseminate to pathogenic subgroups of E. coli. However, it is important to stress that the strain has been given to both humans and pigs without sign of symptoms, indicating that it is a well-characterized strain which can be safely used in future studies.

Other studies have reported that antibiotic treatment influences selection, spread and persistence of resistant bacterial members of the family Enterobacteriaceae [48, 49]. A prospective in vivo/in situ study demonstrated that the administration of low-dose in-feed oxytetracycline of chickens and farm dwellers did not only lead to colonization of the intestinal microbiota of chickens with tetracycline-resistant E. coli strains but also acquisition of such resistance in E. coli in the gut of the farm family [50].

The quantitative data generated by this study might be useful for assessment of the risk of acquisition of antimicrobial resistance from aminoglycosides use in pig production. Besides, this is the first study providing evidence that the selection of resistant bacteria by treatment translates into spread between pigs and that antibiotic administration enhances the risk of transfer among treated animals. Further large-scale studies including more pigs per group, analysis of the immune status of the pigs, and analysis of the E. coli resistance gene pool in the gut of the pigs at the start of the experiments as well as analysis of the variation of both aspects between piglets and between pens should be performed to confirm our conclusions. All these factors might have an impact on strain colonization, shedding and spread of the strain, as well as on emergence and spread of antimicrobial resistance. As mentioned, gentamicin is used for treatment of critical human systemic infections, such as bacteremia. Due to the risk of transfer of gentamicin resistance genes or gentamicin-resistant E. coli from animals to humans and the consequent risk of difficulty in treating infections with gentamicin-resistant E. coli, the selective force conferred by apramycin for presence of gentamicin-resistant E. coli in animals and the potential enhanced spread among them is of great concern.


  1. 1.

    Wellington EM, Boxall AB, Cross P, Feil EJ, Gaze WH, Hawkey PM, Johnson-Rollings AS, Jones DL, Lee NM, Otten W, Thomas CM, Williams AP (2013) The role of the natural environment in the emergence of antibiotic resistance in gram-negative bacteria. Lancet Infect Dis 13:155–165

    PubMed  Article  CAS  Google Scholar 

  2. 2.

    World Health Organization (WHO) (2012) The evolving threat of antimicrobial resistance: options for action. Accessed 22 Dec 2015

  3. 3.

    Wardwell LH, Huttenhower C, Garrett WS (2011) Current concepts of the intestinal microbiota and the pathogenesis of infection. Curr Infect Dis Rep 13:28–34

    PubMed  PubMed Central  Article  Google Scholar 

  4. 4.

    Centers for Disease Control and Prevention (2013) Antibiotic resistance threats in the United States, 2013. Centers for Disease Control and Prevention, Atlanta, GA. Accessed 22 Dec 2015

  5. 5.

    Carmo LP, Nielsen LR, da Costa PM, Alban L (2014) Exposure assessment of extended-spectrum beta-lactamases/AmpC beta-lactamases-producing Escherichia coli in meat in Denmark. Infect Ecol Epidemiol 4:22924

    Google Scholar 

  6. 6.

    Li P, Wu D, Liu K, Suolang S, He T, Liu X, Wu C, Wang Y, Lin D (2014) Investigation of antimicrobial resistance in Escherichia coli and enterococci isolated from Tibetan pigs. PLoS One 9:e95623

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  7. 7.

    Rajkhowa S, Sarma DK (2014) Prevalence and antimicrobial resistance of porcine O157 and non-O157 Shiga toxin-producing Escherichia coli from India. Trop Anim Health Prod 46:931–937

    PubMed  Article  Google Scholar 

  8. 8.

    Aarestrup FM, Duran CO, Burch DG (2008) Antimicrobial resistance in swine production. Anim Health Res Rev 9:135–148

    PubMed  Article  Google Scholar 

  9. 9.

    Juhas M (2015) Horizontal gene transfer in human pathogens. Crit Rev Microbiol 41:101–108

    PubMed  Article  CAS  Google Scholar 

  10. 10.

    The Danish Integrated Antimicrobial Resistance Monitoring and Research Programme (DANMAP). Use of antimicrobial agents and occurrence of antimicrobial resistance in bacteria from food animals, Foods and Humans in Denmark (2003, 2004, 2005, 2006). Accessed 22 Dec 2015

  11. 11.

    Trobos M, Lester CH, Olsen JE, Frimodt-Møller N, Hammerum AM (2008) Natural transfer of sulphonamide and ampicillin resistance between Escherichia coli residing in the human intestine. J Antimicrob Chemother 63:80–86

    PubMed  Article  CAS  Google Scholar 

  12. 12.

    Chaslus-Dancla E, Pohl P, Meurisse M, High Marin M, Lafont JP (1991) Genetic homology between plasmids of human and animal origins conferring resistance to the aminoglycosides gentamicin and apramycin. Antimicrob Agents Chemother 35:590–593

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  13. 13.

    Danish Medicines Agency. Veterinary SPC’s. Accessed 26 July 2015

  14. 14.

    Chaslus-Dancla E, Martel JL, Carlier C, Lafont JP, Courvalin P (1986) Emergence of aminoglycoside 3-N-acetyltransferase IV in Escherichia coli and Salmonella typhimurium isolated from animals in France. Antimicrob Agents Chemother 29:239–243

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  15. 15.

    Chaslus-Dancla E, Glupcznski Y, Gerbaud G, Lagorce M, Lafont JP, Courvalin P (1989) Detection of apramycin resistant Enterobacteriaceae in hospital isolates. FEMS Microbiol Lett 52:261–265

    PubMed  Article  CAS  Google Scholar 

  16. 16.

    Stege H, Bager F, Jacobsen E, Thougaard A (2003) VETSTAT-the Danish system for surveillance of the veterinary use of drugs for production animals. Prev Vet Med 57:105–115

    PubMed  Article  CAS  Google Scholar 

  17. 17.

    Dansk Lægemiddel Information A/S. Lægemiddelkataloget®. Accessed 24 Apr 2014

  18. 18.

    Hiramatsu K (1998) Vancomycin resistance in Staphylococci. Drug Resist Updat 1:135–150

    PubMed  Article  CAS  Google Scholar 

  19. 19.

    Schjørring S, Struve C, Krogfelt KA (2008) Transfer of antimicrobial resistance plasmids from Klebsiella pneumoniae to Escherichia coli in the mouse intestine. J Antimicrob Chemother 62:1086–1093

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  20. 20.

    Daniels JB, Call DR, Hancock D, Sischo WM, Baker K, Besser TE (2009) Role of ceftiofur in selection and dissemination of blaCMY-2-mediated cephalosporin resistance in Salmonella enterica and commensal Escherichia coli isolates from cattle. Appl Environ Microbiol 75:3648–3655

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  21. 21.

    Cuzon G, Naas T, Guibert M, Nordmann P (2010) In vivo selection of imipenem-resistant Klebsiella pneumoniae producing extended-spectrum beta-lactamase CTX-M-15 and plasmid-encoded DHA-1 cephalosporinase. Int J Antimicrob Agents 35:265–268

    PubMed  Article  CAS  Google Scholar 

  22. 22.

    Jakobsen L, Cattoir V, Jensen KS, Hammerum AM, Nordmann P, Frimodt-Møller N (2012) Impact of low-level fluoroquinolone resistance genes qnrA1, qnrB19 and qnrS1 on ciprofloxacin treatment of isogenic Escherichia coli strains in a murine urinary tract infection model. J Antimicrob Chemother 67:2438–2444

    PubMed  Article  CAS  Google Scholar 

  23. 23.

    Subbiah M, Shah DH, Besser TE, Ullman JL, Call DR (2012) Urine from treated cattle drives selection for cephalosporin resistant Escherichia coli in soil. PLoS One 7:e48919

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  24. 24.

    Levy SB, FitzGerald GB, Macone AB (1976) Spread of antibiotic-resistant plasmids from chicken to chicken and from chicken to man. Nature 260:40–42

    PubMed  Article  CAS  Google Scholar 

  25. 25.

    Levy SB, FitzGerald GB, Macone AB (1976) Changes in intestinal microbiota of farm personnel after introduction of a tetracycline-supplemented feed on a farm. N Engl J Med 295:583–588

    PubMed  Article  CAS  Google Scholar 

  26. 26.

    Illumina NexteraXT® Guide 150319425031942, protocol revision C. Accessed 13 August 2015

  27. 27.

    Centre for Genomic Epidemiology. Accessed 21 August 2015

  28. 28.

    NCBI. Accessed 25 Sept 2015

  29. 29.

    Hasman H, Saputra D, Sicheritz-Pontén T, Lund O, Svendsen CA, Frimodt-Møller N, Aarestrup FM (2014) Rapid whole-genome sequencing for detection and characterization of microorganisms directly from clinical samples. J Clin Microbiol 52:139–146

    PubMed  PubMed Central  Article  Google Scholar 

  30. 30.

    Larsen MV, Cosentino S, Rasmussen S, Friis C, Hasman H, Marvig RL, Jelsbak L, Sicheritz-Pontén T, Ussery DW, Aarestrup FM, Lund O (2012) Multilocus sequence typing of total genome sequenced bacteria. J Clin Microbiol 50:1355–1361

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  31. 31.

    Carattoli A, Zankari E, Garcia-Fernandez A, Volby Larsen M, Lund O, Villa L, Aarestrup FM, Hasman H (2014) PlasmidFinder and pMLST: in silico detection and typing of plasmids. Antimicrob Agents Chemother 58:3895–3903

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  32. 32.

    Zankari E, Hasman H, Cosentino S, Vestergaard M, Rasmussen S, Lund O, Aarestrup FM, Larsen MV (2012) Identification of acquired antimicrobial resistance genes. J Antimicrob Chemother 67:2640–2644

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  33. 33.

    Joensen KG, Scheutz F, Lund O, Hasman H, Kaas RS, Nielsen EM, Aarestrup FM (2014) Real-time whole-genome sequencing for routine typing, surveillance, and outbreak detection of verotoxigenic Escherichia coli. J Clin Microbiol 52:1501–1510

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  34. 34.

    Cavaco LM, Abatih E, Aarestrup FM, Guardabassi L (2008) Selection and persistence of CTX-M-producing Escherichia coli in the intestinal microbiota of pigs treated with amoxicillin, ceftiofur, or cefquinome. Antimicrob Agents Chemother 52:3612–3616

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  35. 35.

    Herrero A, Mendoza MC, Threlfall EJ, Rodicio MR (2009) Detection of Salmonella enterica serovar Typhimurium with pUO-StVR2-like virulence-resistance hybrid plasmids in the United Kingdom. Eur J Clin Microbiol Infect Dis 28:1087–1093

    PubMed  Article  CAS  Google Scholar 

  36. 36.

    Dohoo I, Martin W, Stryhn H (2009) Veterinary epidemiologic research, 2nd edn. VER Inc., Charlottetown

    Google Scholar 

  37. 37.

    Kruse H, Sørum H (1994) Transfer of multiple drug resistance plasmids between bacteria of diverse origins in natural microenvironments. Appl Environ Microbiol 60:4015–4021

    PubMed  PubMed Central  CAS  Google Scholar 

  38. 38.

    Guarner F, Malagelada J (2003) Gut microbiota in health and disease. Lancet 360:512–519

    Article  Google Scholar 

  39. 39.

    Deneke H, Mengistu MY, Hoffner SE, Andersson DI (2004) Effect of rpoB mutations conferring Rifampin resistance on fitness of Mycobacterium tuberculosis. Antimicrob Agents Chemother 48:1289–1294

    Article  CAS  Google Scholar 

  40. 40.

    O’Hara AM, Shanahan F (2006) The gut microbiota as a forgotten organ. EMBO Rep 7:688–693

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  41. 41.

    Dogi CA, Galdeano CM, Perdigón G (2008) Gut immune stimulation by non pathogenic gram (+) and gram (−) bacteria. Comparison with a probiotic strain. Cytokine 41:223–231

    PubMed  Article  CAS  Google Scholar 

  42. 42.

    Stecher B, Hardt W (2008) The role of microbiota in infectious disease. Trends Microbiol 16:107–114

    PubMed  Article  CAS  Google Scholar 

  43. 43.

    Yates CM, Shaw DJ, Roe AJ, Woolhouse ME, Amyes SG (2006) Enhancement of bacterial competitive fitness by apramycin resistance plasmids from non-pathogenic Escherichia coli. Biol Lett 2:463–465

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  44. 44.

    Jensen VF, Jakobsen L, Emborg HD, Seyfarth AM, Hammerum AM (2006) Correlation between apramycin and gentamicin use in pigs and an increasing reservoir of gentamicin-resistant Escherichia coli. J Antimicrob Chemother 58:101–107

    PubMed  Article  CAS  Google Scholar 

  45. 45.

    Hunter JE, Hart CA, Shelley JC, Walton JR, Bennett M (1993) Human isolates of apramycin-resistant Escherichia coli which contain the genes for the AAC(3)IV enzyme. Epidemiol Infect 110:253–259

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  46. 46.

    Johnson AP, Burns L, Woodford N, Threlfall EJ, Naidoo J, Cooke EM, George RC (1994) Gentamicin resistance in clinical isolates of Escherichia coli encoded by genes of veterinary origin. J Med Microbiol 40:221–226

    PubMed  Article  CAS  Google Scholar 

  47. 47.

    Dobrindt U, Hentschel U, Kaper JB, Hacker J (2002) Genome plasticity in pathogenic and nonpathogenic enterobacteria. Curr Top Microbiol Immunol 264:57–175

    Google Scholar 

  48. 48.

    Callens B, Faes C, Maes D, Catry B, Boyen F, Francoys D, de Jong E, Haesebrouck F, Dewulf J (2015) Presence of antimicrobial resistance and antimicrobial use in sows are risk factors for antimicrobial resistance in their offspring. Microb Drug Resist 21:50–58

    PubMed  Article  CAS  Google Scholar 

  49. 49.

    Fleury MA, Mourand G, Jouy E, Touzain F, Le Devendec L, de Boisseson C, Eono F, Cariolet R, Guérin A, Le Goff O, Blanquet-Diot S, Alric M, Kempf I (2015) Impact of ceftiofur injection on gut microbiota and Escherichia coli Resistance in Pigs. Antimicrob Agents Chemother 59:5171–5780

    PubMed  Article  CAS  Google Scholar 

  50. 50.

    Marshall MM, Levy SB (2011) Food animals and antimicrobials: impacts on human health. Clin Microbiol Rev 24:718–733

    PubMed  PubMed Central  Article  CAS  Google Scholar 

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Authors’ contributions

AHF, CZ and JEO conceived the study. AHF, MHH, and AN performed experiments. AHF, CZ and JEO, participated in study design and provided critical advice. AHF, JEO and SSN analysed the data and AHF wrote the first draft of the manuscript. RSH contributed with the sequencing of the strain. All authors read and approved the final manuscript.


Authors would like to thank, Anette M. Hammerum for providing the strain E. coli 912, Pia Rønnov Mortensen for her technical assistance and Lina Cavaco for her recommendations for the setting up of the in vivo experiment. This study has been supported by the project “Minimizing Antibiotic Resistance Development-MINIRESIST” funded by the Danish Council (DFS) Grant Number 0603-00358B.

Competing interests

The authors declare that they have no competing interests.

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Correspondence to Ana Herrero-Fresno.

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Herrero-Fresno, A., Zachariasen, C., Hansen, M.H. et al. Apramycin treatment affects selection and spread of a multidrug-resistant Escherichia coli strain able to colonize the human gut in the intestinal microbiota of pigs. Vet Res 47, 12 (2016).

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  • Resistance Gene
  • Intestinal Microbiota
  • Resistant Bacterium
  • Southern Blot Hybridization
  • MacConkey Agar