- Research article
- Open Access
The presence of antibiotic-resistant Staphylococcus spp. and Escherichia coli in smallholder pig farms in Uganda
BMC Veterinary Research volume 17, Article number: 31 (2021)
The development of antimicrobial resistance is of global concern, and is commonly monitored by the analysis of certain bacteria. The aim of the present study was to study the antibiotic susceptibility in isolates of Staphylococcus spp. and Escherichia (E.) coli obtained from healthy pigs originating from nineteen herds enrolled in a study on herd health management in Lira district, northern Uganda. Skin and nasal swabs were analyzed for the presence of Staphylococcus spp., and selectively cultivated to investigate the presence of methicillin-resistant Staphylococcus (S.) aureus (MRSA), and rectal swabs were analyzed for the presence of E. coli. Antibiotic susceptibility was tested by broth micro-dilution. Information on the antibiotic usage and treatment regimens during the previous year was gathered using structured interviews and longitudinal data.
In Staphylococcus spp., resistance to penicillin (10/19 isolates; 53%), fusidic acid (42%) and tetracycline (37%) were most commonly found. In E. coli, resistance to sulfamethoxazole (46/52 isolates; 88%), tetracycline (54%) and trimethoprim (17%) was most frequent. Methicillin-resistant S. aureus was found in one sample (1/50; 2%). Multi-drug resistant isolates of Staphylococcus spp. and E. coli were found in 54 and 47% of the herds, respectively. At the herd level, no associations could be made between antibiotic resistance and herd size or treatment regimens for either of the bacteria.
In conclusion, resistance to important antibiotics frequently used in animals in Uganda was common, and the presence of MRSA was demonstrated, in Ugandan pig herds.
Antimicrobial resistance (AMR) is a threat to public as well as to animal health [1, 2]. In some bacterial species, the AMR may be intrinsic, but might also develop following the extensive use of antibiotics [3, 4]. Thus, high levels of antibiotic resistance generally correlates with high antibiotic usage [5, 6], and antibiotics are still used in many countries for regular prophylactic treatments or as growth promoters in food-producing animals .
Different Staphylococcus spp. are a part of the commensal microbiota on e.g. the skin and nares in healthy humans and animals [8, 9], but may also cause disease ranging from abscesses and mastitis to septicemia [10, 11]. In response to antibiotic treatment, the bacteria may develop resistance , and methicillin-resistant Staphylococcus (S.) aureus (MRSA) have emerged as one of the most common antibiotic-resistant pathogens worldwide . Further, in the last decades, livestock-associated MRSA have been found in healthy domestic animals, including pigs, posing a risk especially to humans with occupational contact with livestock [9, 14].
To monitor the development of antibiotic resistance, indicator bacteria such as Escherichia (E.) coli may be used [15, 16]. Escherichia coli are commensal, or potentially opportunistic pathogens that are common in the intestinal tract of animals and humans. Besides being used as indicator bacteria, resistance in E. coli may be important since resistance genes may be transferred to other, pathogenic, strains of E. coli, or to other bacteria.
In Uganda, information on antibiotic usage and AMR in livestock is scarce due to the lack of national surveillance programs . Most large pig farms routinely use antibiotic prophylactic treatments  but the usage does not seem to be as common in smallholder farms , where most of the Ugandan pigs are found . While scientific studies on MRSA are scarce in Uganda , a previous study on pig herd health found antibiotic resistance in clinical isolates of S. sciuri and E. coli  and thus, further investigations were warranted.
The aim of this study was to investigate the presence and antibiotic resistance of Staphylococcus spp., including MRSA, and E. coli isolated from pigs in smallholder farms in Lira district, northern Uganda, by bacterial cultivation of swab samples and determination of antibiotic susceptibility by broth micro-dilution.
Materials and methods
The study was conducted in the four sub-counties closest to Lira town, Lira district, in the northern region of Uganda. A list of 250 pig farmers were obtained from the District Veterinary Office. From this list, 20 herds, meeting the inclusion criteria of having at least one sow and keeping the pigs confined or tethered, were selected by simple randomization. One farmer had sold his pigs prior to the visit, and thus, 19 herds remained in the study. As categorized by Ouma et al. , herds with less or equal to three sows/year were termed small, while those with more than three sows/year were termed large.
Collection of data on the antibiotic usage
Information on the antibiotic usage during September 2018–September 2019 was gathered by several methods applied in all herds. In September 2019, a structured interview was conducted (see Additional file 1). In a separate study, the farms had previously been visited once a month for a period of one year . During these visits, information on treatments and antibiotic usage was gathered by semi-structured interviews, including the reasons for the treatments, the drugs and dosage used, and the number of treatments, and by observations on the drugs available on the farms. Further, farmers were asked to continuously record treatment information, as also investigated through the interviews. The farmers’ records were constructed in the local language, and the questions and answers in the interviews were continuously translated to and from the local language by either of two local animal health workers, and were recorded in English.
Since information on the number of pigs treated at each occasion was often missing, a treatment occasion (TO) was defined as one reported antibiotic treatment in a herd, regardless of whether one or many pigs were treated. The number of treatment occasions per pig was calculated as the number of TO in a herd during September 2018 to September 2019, divided by the average number of pigs of all age categories in that herd during the same period.
The results were analyzed at herd level using Fisher’s exact test (https://epitools.ausvet.com.au/twobytwotable) comparing resistance (Yes/No) to any of the antibiotics included in the panels, resistance to single selected antibiotic substances (tetracycline and penicillin/ampicillin) and the presence of multi-drug resistance, to the herd size and treatment regimens (see Additional file 2).
Pigs of approximately two months of age were targeted for sampling of Staphylococcus spp., as MRSA is reported to be more common in this age category [24, 25]. In the sampling of E. coli, pigs of approximately six months of age were targeted, in accordance with previously reported surveillance programs . If the targeted age-categories were not available at the sampling occasions, pigs as close to the desired age as possible were instead selected, giving a median age in the sampled pigs of five and seven months for Staphylococcus spp. and E. coli, respectively. The number of pigs sampled in each herd depended on the herd size, and the sampling was performed as described in Table 1.
For the analysis of Staphylococcus spp., each pig was sampled using a single swab (Transystem™, Copan Diagnostics Inc., Murrieta, California, USA) to swab the nasal cavity, behind the ears and around the perineum, as multiple-site sampling has been shown to increase the detection rate of MRSA . When possible, additional individual samples were taken from the targeted age category, and later pooled two-three together per pen or group at the laboratory, to enhance the possibility of detecting MRSA . Individual rectal swabs were taken from each pig for the analysis of E. coli. All swabs were transported on ice and stored in Amies medium with charcoal at + 4 to+ 10 °C until being cultivated at the District Veterinary Office Laboratory in Lira. However, since the incubator in Lira broke down towards the end of the farm visits, and to be able to perform all cultivation steps in one laboratory, samples collected during the final days of field work were instead stored at + 4 to + 10 °C and analyzed at the Central Diagnostic Laboratory at Makerere University in Kampala.
Bacterial cultivation of Staphylococcus spp.
Individual swabs, or two-three pooled swabs, were submerged in 10 mL non-selective Mueller Hinton broth (MHB; National Veterinary Institute, SVA, Uppsala, Sweden) within 0–6 days (median 2), and incubated for 24 h at 37 °C. The incubated broth was immediately analyzed for MRSA by a two-step enrichment method , and the remaining broth was stored at + 4 to + 10 °C before being analyzed for the presence of other Staphylococcus spp.
In the analysis of MRSA, 1 mL of the incubated MHB was transferred to 9 mL selective Tryptic Soy broth supplemented with azotrenam 72 mg/L and cefoxitin 3.8 mg/L (SVA, Uppsala, Sweden), and incubated for 24 h at 37 °C. The samples were vortexed and 20 μL were streaked onto selective chromogenic Oxoid Brilliance MRSA 2 agar (Oxoid, Basingstoke, England), and incubated at 37 °C. The growth was assessed after 24 and 48 h. If present, up to five suspected, light blue, colonies were streaked onto 5% bovine blood agar plates (SVA, Uppsala, Sweden), and incubated at 37 °C for 24 h. Pure-cultured isolates having a morphology suspected to be MRSA were tested for catalase production and KOH reactivity (SVA, Uppsala, Sweden). Isolates with the correct morphology, with α- and/or β-hemolysis, and that were catalase-positive and KOH-negative, were preliminary identified as MRSA.
The presence of additional Staphylococcus spp. were analyzed within 5–14 days (median 5) at the laboratory in Kampala, by culturing 20 μL from the remaining MHB onto blood agar plates supplemented with 5% bovine blood, and incubated at 37 °C for 24 h. From each sample, up to five suspected, opaque, white or yellow, medium-sized, colonies with or without hemolysis were cultivated on blood agar plates as described above. In the case of bacterial swarming, the sample was re-cultured onto Cysteine Lactose Electrolyte Deficient (CLED) agar plates (Oxoid, Basingstoke, England) since CLED agar is electrolyte (salt) deficient, and prevent the swarming of bacteria. The identification of Staphylococcus spp. was based on the colony morphology and the production of catalase, but no reaction in KOH.
Further identification of Staphylococcus spp
All isolates identified as Staphylococcus spp. were later transported to Sweden in Amies transport medium with charcoal and analyzed by Matrix-Assisted Laser Desorption/Ionization Time of Flight Mass Spectrometry (MALDI-TOF MS; Microflex LT System, Bruker Daltonik GmbH, Bremen, Germany) for species identification. Isolates presumed to be MRSA and confirmed as S. aureus by MALDI-TOF MS were also prepared according to Capurro et al.  and analyzed for the presence of mecA, mecC, nuc and pvl genes by a real-time quadruplex PCR according to Pichon et al. . Briefly, pure-cultured colony material was suspended in lysostaphin, incubated at 37 °C for 10 min, proteinase K and Tris-HCL were added and the mixture was incubated at 54 °C for an additional 10 min. After boiling for 5 min, the samples were cooled and centrifuged, and the supernatant was frozen at − 20 °C before PCR. The PCR assay used a 20-μL reaction volume with 0.5 mM primers targeting the sequences according to Pichon et al. . The amplification included an initial denaturation of 95 °C for 5 min., followed by 40 cycles of denaturation at 94 °C for 15 s. and 40 s. of annealing at 58 °C. Staphylococcus aures subsp. aureus CCUG 60578 (nuc positive, mecA positive, pvl positive) and Staphylococcus aures subsp. aureus CCUG 63582 (nuc positive, mecA negative, mecC positive) were used as quality control.
Bacterial cultivation of E. coli
Individual swabs were streaked on CLED agar plates within 0–4 days (median 0), and incubated for 24 h at 37 °C. Up to five suspected, greyish-white, opaque, medium-sized, lactose-fermenting colonies were re-cultured onto 5% horse blood agar plates (SVA, Uppsala, Sweden), and incubated at 37 °C for 24 h. The isolates were analyzed for biochemical reactions with oxidase (Becton, Dickinson and Company, Franklin Lakes, NJ, USA), KOH and the spot indole test (SVA, Uppsala, Sweden). Isolates with correct morphology, without hemolysis or displaying α-hemolysis, and that were oxidase-negative, indole-positive and KOH-negative, were identified as E. coli. One colony per sample was randomly selected for further analyses.
Antimicrobial susceptibility testing
Antimicrobial susceptibility testing of the E. coli isolates was performed by broth micro-dilution at the Makerere University, Kampala, and at the Swedish University of Agriculture on isolates of MRSA and other Staphylococcus spp. following identification by MALDI-TOF MS and PCR. Commercial plates for Staphylococcus spp. (VetMIC™ STAF/STREP, SVA, Uppsala, Sweden), and for E. coli (Sensititre™ EU Surveillance Salmonella/E. coli EUVSEC Plate, Thermo Fisher Scientific, Waltham, Massachusetts, USA) were used in the analyses according to the manufacturer’s instructions. Briefly, the colony material from one pure-cultured isolate was incubated in 5 mL of cation-adjusted Mueller Hinton broth (CAMHB; SVA, Uppsala, Sweden) for 3 h at 37 °C. The sample was vortexed and 10 μL was transferred into 10 mL of CAMHB. After vortexing, 50 μL was transferred into each well of a micro-titer plate and incubated for 18 h at 37 °C. The minimum inhibitory concentration (MIC) was determined as the concentration in the first well where visible growth was inhibited. The antibiotics and concentrations tested for each commercial plate are shown in Table 2 and Table 3. The strains ATCC 29213 (S. aureus) and ATCC 25922 (E. coli) were included as controls. Density and purity controls were included in each sample.
The MIC values were compared to epidemiological cut-off values (ECOFF) , and isolates with reduced susceptibility were classified as non-wild type. In agreement with the Swedish Veterinary Antibiotic Resistance Monitoring report, non-wild type isolates are referred to as resistant . However, it should be noted that this does not necessarily imply clinical resistance. An isolate was classified as multi-drug resistant (MDR) if it exhibited resistance to at least three classes of antibiotics . The MIC50 and MIC90 values were calculated for E. coli according to Schwarz et al. .
Seventeen farmers stated that they had treated at least one pig with antibiotics during the last 12 months, mainly using oxytetracycline (OTC) and/or a combination of penicillin and streptomycin, by “injections”. Single farmers also occasionally used trimethoprim-sulfamethoxazole or tylosine injections, sulfamidine tablets or oxytetracycline spray. The number of TO per herd during the previous year varied between one and 13 (median 3), and the number of TO per pig and herd varied between 0.1 and 1.4 (median 0.4). The antibiotics were administered up to five times per TO, but at 31 out of the 65 TO where information was provided, only one treatment was given. In 12 herds, the treatments had been performed by paraveterinarians, i.e. paraprofessional animal health workers, and in five herds by the farmers themselves.
In nine herds, antibiotics had been used as “routine” or “preventive” treatments at least once, while in the other 8 herds, antibiotics had been used solely for the treatment of sick pigs. The three farmers who stated the reasons for these “routine” treatments, reported that it was due to fear of “outbreaks”.
Bacteriological cultivation and antibiotic resistance
A total number of 50 samples from 83 individual pigs were analyzed for the detection of Staphylococcus spp., and 53 individual samples were analyzed for E. coli.
Nineteen strains of Staphylococcus spp. were isolated from 18 samples (18/50; 36%), originating from 13 herds. The isolates were identified as S. aureus (n=4), S. simulans (5), S. cohnii (2), S. chromogenes (2), S. sciurii (2), S. lentus (1), S. petrasii (1), S. epidermidis (1) and S. hyicus (1). Resistance to penicillin was most commonly found, followed by resistance to fusidic acid, and to tetracycline (Table 2). Resistance to at least one antibiotic substance was found in all 13 herds and eight isolates (42%) from seven (54%) herds exhibited MDR. None of the isolates exhibited resistance to enrofloxacin or nitrofurantoin. One isolate (S. simulans) was susceptible to all tested antibiotics. No associations could be made between antibiotic resistance and herd size, treatment regimens or preventive medication strategies (see Additional file 2).
One of the S. aureus isolates was confirmed as MRSA by PCR (1/50; 2% of the samples), positive for the nuc, pvl and mecA genes, resulting in an occurrence at herd level of 5% (1/19). The isolate originated from a small farm situated in a village densely populated with both pigs and humans. In this farm, the pigs had received antibiotic treatments from a paraveterinarian on three occasions in the previous year, both as a routine and to treat sick pigs, resulting in 0.7 TO per pig. At two of the treatment occasions, OTC was used, and at one TO, tylosine was used, at all occasions as single injections.
Escherichia coli was isolated from 52 out of 53 samples (98.1%), and the full MIC results of all isolates are given in Additional file 3. Resistance to sulfamethoxazole was most commonly found, followed by resistance to tetracycline and to trimethoprim (Table 3). Four isolates each (7.7%) exhibited resistance to ciprofloxacin and cefotaxime, respectively, while no resistance to carbapenems was found. Resistance to at least one antibiotic substance was found in isolates from at least one pig in all 19 herds. Fourteen isolates (26.9%) from nine herds (47%) exhibited MDR, and five isolates (9.6%) were susceptible to all tested antibiotics. No associations could be made between resistance and herd size, treatment regimens or preventive medication strategies (see Additional file 2).
Antibiotic resistance was commonly found in isolates of both Staphylococcus spp. and E. coli. It is worrying that nine herds had used antibiotics for the treatment of healthy pigs to e.g. prevent outbreaks, which in Ugandan smallholder pig farms commonly refers to African swine fever, a devastating endemic viral disease that is not susceptible to antibiotics. Further, to avoid the development of resistance, antibiotic treatment of healthy animals should be avoided.
To the best of our knowledge, this is the first report in international literature on the occurrence of MRSA in pigs in Uganda. In line with other studies from other sub-Saharan countries [34, 35], the occurrence seems to be low, since only one MRSA isolate found, carrying both the mecA and the virulence factor pvl genes. The farm of origin was small (n=1.4 sows/year) and had conducted slightly more TO per pig (n=0.7) than the average herd in the study. It was also the only herd that had used tylosine in the treatments, and the isolate was also resistant to macrolids. In Uganda, animals and humans sometimes live closely together, and free-ranging pigs are common . Transfer of bacteria and/or resistance genes between humans and pigs is thus not unlikely. However, since no further genetic characterization of the isolate was performed, the molecular epidemiology and origin of the isolate is unknown.
The high number of antibiotic-resistant isolates of both Staphylococcus spp. and E. coli, in particular displaying resistance to tetracycline, penicillins and sulfonamides, are important findings since these antibiotics are commonly used to treat livestock in Uganda  and are critically or highly important to both human and veterinary medicine [37, 38]. Further, resistance to other high priority critically important antimicrobials such as macrolides, quinolones and third generation cephalosporins was found in several isolates. While no further analyzes were performed, the results also suggest the possible presence of extended spectrum β-lactamase (ESBL) producing E. coli.
No associations between antibiotic resistance and herd size or treatment regimens were detected for any of the bacteria, regardless of whether the animals had been treated routinely for prophylactic purposes, or upon clinical signs of disease only, however, the sample size was small. Thus, future studies may include more herds to increase the possibility of detecting any such associations, and, if possible, also include investigations on bacterial isolates collected from the farmers and animal care-takers. Nevertheless, the number of resistant E. coli isolates in this study were slightly lower than previously reported in studies from other low- and middle-income countries . However, different sampling and culturing methods and differences in the presentation of the results make the outcomes from various studies difficult to compare [21, 33]. The number of isolates from each species of Staphylococcus was too low to allow any conclusions to be drawn on species-level, however, S. cohnii seems to be more prone to develop resistance as compared to e.g. S. simulans, as previously noted by Ouba et al. .
In some of the herds where resistance to tetracycline in E. coli was detected, tetracycline resistance has previously been demonstrated in isolates from clinical cases of post-weaning diarrhea . Further, isolates of S. sciuri from a healthy pig in this study exhibited similar antibiotic resistance pattern as an isolates of S. sciuri previously recovered from a clinical case of exudative epidermitis in the same herd (data not shown).
In the present study, minor practical-methodological challenges were faced such as slightly fluctuating incubator temperatures, pipettes with unclear calibration status and autoclaved pipette tips. Thus, it cannot be excluded that this might have affected the results, however, the antibiotic-susceptibility profiles of the control strains were within the pre-determined limits. Further, in the interpretation of the levels of sulfamethoxazole resistance in E. coli, growth was only assessed as “growth” or “no growth”, whereas the method allows for up to 20% growth to be assessed as negative according to the manufacturer’s instructions. The level of resistance to trimethoprim was much lower than to sulfamethoxazole, as previously noted in a study of other Enterobacteriacae in Uganda . This could be related to either the potential methodological short-comings in the analysis of sulfamethoxazole as described above, or resulting from co-selection as sulphonamide resistance may be linked to other types of resistance, e.g. through association with class 1 integrons . Further, it might possibly also be explained by the common use of sulfonamides without being combined with trimethoprim . The use of sulfonamide tablets was only mentioned by one farmer, but it is possible that others also used them but failed to report this usage during the interviews, as these were not given as “injections” and may thus not have been regarded as a treatment. In support of this hypothesis, many farmers also reported the use of various drugs, mainly anthelmintics and endectocides, when asked about their use of antibiotics. This lack of knowledge about drugs might have confounded the results, if such treatment occasions were misinterpreted as e.g. preventive antibiotic use. However, since the interviews were complemented by longitudinal data and the names of the drugs were retrieved in most cases, these results were likely reliable.
In conclusion, antibiotic resistance to frequently used and critically or highly important antibiotics to both human and veterinary medicine, such as e.g. tetracycline, was commonly found in isolates of Staphylococcus spp. and E. coli from Ugandan pigs. Further, several farmers used antibiotics for the purpose of “preventive” or “routine” treatments, however, this did not seem to influence the level of resistance in single herds. Methicillin-resistant S. aureus carrying the mecA and the virulence factor pvl genes were found in one of the investigated pigs.
Availability of data and materials
The datasets generated and/or analyzed during the current study are available from the corresponding author on reasonable request.
Bengtsson B, Greko C. Antibiotic resistance--consequences for animal health, welfare, and food production. Ups J Med Sci. 2014;119(2):96–102.
WHO. Global action plan on antimicrobial resistance. Geneva: World Health Organization; 2015.
Malhotra-Kumar S, Lammens C, Coenen S, Van Herck K, Goossens H. Effect of azithromycin and clarithromycin therapy on pharyngeal carriage of macrolide-resistant streptococci in healthy volunteers: a randomised, double-blind, placebo-controlled study. Lancet. 2007;369(9560):482–90.
Bronzwaer SL, Cars O, Buchholz U, Molstad S, Goettsch W, Veldhuijzen IK, Kool JL, Sprenger MJ, Degener JE. A European study on the relationship between antimicrobial use and antimicrobial resistance. Emerg Infect Dis. 2002;8(3):278–82.
Dunlop RH, McEwen SA, Meek AH, Clarke RC, Black WD, Friendship RM. Associations among antimicrobial drug treatments and antimicrobial resistance of fecal Escherichia coli of swine on 34 farrow-to-finish farms in Ontario, Canada. Prev Vet Med. 1998;34(4):283–305.
Chantziaras I, Boyen F, Callens B, Dewulf J. Correlation between veterinary antimicrobial use and antimicrobial resistance in food-producing animals: a report on seven countries. J Antimicrob Chemother. 2013;69(3):827–34.
OIE: OIE Annual report on antimicrobial agents intended for use in animals. In., vol. Third report: World Organisation for Animal Health; 2018.
Chen C-J, Hsu K-H, Lin T-Y, Hwang K-P, Chen P-Y, Huang Y-C. Factors Associated with Nasal Colonization of Methicillin-Resistant Staphylococcus aureus among Healthy Children in Taiwan. J Clin Microbiol. 2011;49(1):131–7.
Oppliger A, Moreillon P, Charriere N, Giddey M, Morisset D, Sakwinska O. Antimicrobial resistance of Staphylococcus aureus strains acquired by pig farmers from pigs. Appl Environ Microbiol. 2012;78(22):8010–4.
Becker K, Ballhausen B, Kahl BC, Köck R. The clinical impact of livestock-associated methicillin-resistant Staphylococcus aureus of the clonal complex 398 for humans. Vet Microbiol. 2017;200:33–8.
Taponen S, Simojoki H, Haveri M, Larsen HD, Pyörälä S. Clinical characteristics and persistence of bovine mastitis caused by different species of coagulase-negative staphylococci identified with API or AFLP. Vet Microbiol. 2006;115(1):199–207.
Livermore DM. Antibiotic resistance in staphylococci. Int J Antimicrob Agents. 2000;16:3–10.
Grundmann H, Aires-de-Sousa M, Boyce J, Tiemersma E. Emergence and resurgence of meticillin-resistant Staphylococcus aureus as a public-health threat. Lancet. 2006;368(9538):874–85.
Goerge T, Lorenz MB, van Alen S, Hübner N-O, Becker K, Köck R. MRSA colonization and infection among persons with occupational livestock exposure in Europe: Prevalence, preventive options and evidence. Vet Microbiol. 2017;200:6–12.
EFSA, Aerts M, Battisti A, Hendriksen R, Kempf I, Teale C, Tenhagen BA, Veldman K, Wasyl D, Guerra B, et al. Technical specifications on harmonised monitoring of antimicrobial resistance in zoonotic and indicator bacteria from food-producing animals and food. Efsa J. 2019;17(6):122.
WHO. Integrated surveillance of antimicrobial resistance in foodborne bacteria: application of a One Health approach. Geneva: World Health Organization; 2017.
Ball TA, Monte DF, Aidara-Kane A, Matheu-Alvarez J, Ru H, Thakur S, Horovitz J, Ejobi F, Lacher DW, Fedorka-Cray PJ. Phenotypic and Genotypic Characterization of Escherichia coli and Salmonella enterica from Dairy Cattle Farms in the Wakiso District, Uganda: A Cross-Sectional Study. Foodborne Pathog Dis. 2019;16(1):54–9.
Okello E, Moonens K, Erume J, De Greve H. Enterotoxigenic Escherichia coli strains are highly prevalent in Ugandan piggeries but disease outbreaks are masked by antibiotic prophylaxis. Trop Anim Health Prod. 2015;47(1):117–22.
Dione MM, Ouma EA, Roesel K, Kungu J, Lule P, Pezo D. Participatory assessment of animal health and husbandry practices in smallholder pig production systems in three high poverty districts in Uganda. Prev Vet Med. 2014;117(3–4):565–76.
Ikwap K, Jacobson M, Lundeheim N, Owiny DO, Nasinyama GW, Fellstrom C, Erume J. Characterization of pig production in Gulu and Soroti districts in northern and eastern Uganda. Livestock Res Rural Dev. 2014;26(4):74.
Lozano C, Gharsa H, Ben Slama K, Zarazaga M, Torres C. Staphylococcus aureus in Animals and Food: Methicillin Resistance, Prevalence and Population Structure. A Review in the African Continent. Microorganisms. 2016;4(1):12.
Gertzell E. Veterinary Herd Health Management in Ugandan smallholder pig farms. Uppsala: Swedish University of Agricultural Sciences; 2020.
Ouma E, Dione M, Birungi R, Lule P, Mayega L, Dizyee K. African swine fever control and market integration in Ugandan peri-urban smallholder pig value chains: An ex-ante impact assessment of interventions and their interaction. Prev Vet Med. 2018;151:29–39.
Moon DC, Jeong SK, Hyun BH, Lim SK. Prevalence and Characteristics of Methicillin-Resistant Staphylococcus aureus Isolates in Pigs and Pig Farmers in Korea. Foodborne Pathog Dis. 2019;16(4):256–61.
Bangerter PD, Sidler X, Perreten V, Overesch G. Longitudinal study on the colonisation and transmission of methicillin-resistant Staphylococcus aureus in pig farms. Vet Microbiol. 2016;183:125–34.
Pletinckx LJ, De Bleecker Y, Dewulf J, Rasschaert G, Goddeeris BM, De Man I. Evaluation of salt concentrations, chromogenic media and anatomical sampling sites for detection of methicillin-resistant Staphylococcus aureus in pigs. Vet Microbiol. 2012;154(3):363–8.
Friese A, Schulz J, Hoehle L, Fetsch A, Tenhagen B-A, Hartung J, Roesler U. Occurrence of MRSA in air and housing environment of pig barns. Vet Microbiol. 2012;158(1):129–35.
Nemeghaire S, Argudín MA, Haesebrouck F, Butaye P. Epidemiology and molecular characterization of methicillin-resistant Staphylococcus aureusnasal carriage isolates from bovines. BMC Vet Res. 2014;10(1):153.
Capurro A, Artursson K, Waller KP, Bengtsson B, Ericsson-Unnerstad H, Aspan A. Comparison of a commercialized phenotyping system, antimicrobial susceptibility testing, and tuf gene sequence-based genotyping for species-level identification of coagulase-negative staphylococci isolated from cases of bovine mastitis. Vet Microbiol. 2009;134(3–4):327–33.
Pichon B, Hill R, Laurent F, Larsen AR, Skov RL, Holmes M, Edwards GF, Teale C, Kearns AM. Development of a real-time quadruplex PCR assay for simultaneous detection of nuc, Panton-Valentine leucocidin (PVL), mecA and homologue mecALGA251. J Antimicrob Chemother. 2012;67(10):2338–41.
EUCAST: Data from the European Commitee on Antimicrobial Susceptibility Testing (EUCAST), MIC distribution website [https://mic.eucast.org/Eucast2/] Accessed January 2020. In.; 2020.
Swedres-Svarm: Consumption of antibiotics and occurence of resistance in Sweden. In. Solna/Uppsala: Public Health Agency of Sweden and National Veterinary Institute; 2018.
Schwarz S, Silley P, Simjee S, Woodford N, van Duijkeren E, Johnson AP, Gaastra W. Assessing the antimicrobial susceptibility of bacteria obtained from animals. Vet Microbiol. 2010;141(1):1–4.
Van Lochem S, Thompson PN, Annandale CH. Prevalence of methicillin-resistant Staphylococcus aureus among large commercial pig herds in South Africa. Onderstepoort J Vet Res. 2018;85(1):a1561.
Otalu OJ, Kwaga JKP, Okolocha EC, Islam MZ, Moodley A. High Genetic Similarity of MRSA ST88 Isolated From Pigs and Humans in Kogi State, Nigeria. Front Microbiol. 2018;9:3098.
Okubo T, Yossapol M, Maruyama F, Wampande EM, Kakooza S, Ohya K, Tsuchida S, Asai T, Kabasa JD, Ushida K. Phenotypic and genotypic analyses of antimicrobial resistant bacteria in livestock in Uganda. Transbound Emerg Dis. 2019;66(1):317–26.
WHO: Critically Important Antimicrobials for Human Medicine, 6th revision. . In.; 2018.
OIE: OIE List of Antimicrobial Agents of Veterinary Importance. In.; 2018.
Van Boeckel TP, Pires J, Silvester R, Zhao C, Song J, Criscuolo NG, Gilbert M, Bonhoeffer S, Laxminarayan R. Global trends in antimicrobial resistance in animals in low- and middle-income countries. Science. 2019;365:eaaw 1944.
Ouoba LII, Vouidibio Mbozo AB, Anyogu A, Obioha PI, Lingani-Sawadogo H, Sutherland JP, Jespersen L, Ghoddusi HB. Environmental heterogeneity of Staphylococcus species from alkaline fermented foods and associated toxins and antimicrobial resistance genetic elements. Int J Food Microbiol. 2019;311:108356.
Ikwap K, Erume J, Owiny DO, Nasinyama GW, Melin L, Bengtsson B, Lundeheim N, Fellstrom C, Jacobson M. Salmonella species in piglets and weaners from Uganda: Prevalence, antimicrobial resistance and herd-level risk factors. Prev Vet Med. 2014;115(1–2):39–47.
Deng Y, Bao X, Ji L, Chen L, Liu J, Miao J, Chen D, Bian H, Li Y, Yu G. Resistance integrons: class 1, 2 and 3 integrons. Ann Clin Microbiol Antimicrob. 2015;14:45–5.
The pig farmers in Lira are acknowledged for allowing us to interview them and sampling their pigs, and The District Veterinary Office in Lira is acknowledged for practical assistance during field work. The authors are also grateful to Lise-Lotte Fernström and the staff at the Central Diagnostic Laboratory for their technical assistance.
This study was supported by Minor Field Study grants from the Swedish International Development Cooperation Agency to LD and KS, and by the CGIAR Research Program on Livestock. Open Access funding provided by Swedish University of Agricultural Sciences.
Ethics approval and consent to participate
Ethical permissions were obtained from the College of Veterinary Medicine, Animal Resources and Biosecurity at Makerere University (ref SBLS/REC/18/005), and from the Uganda National Council for Science and Technology (ref A591). Written and oral informed consent was obtained from the farmers before the beginning of the study.
Consent for publication
The authors declare that they have no competing interests.
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Structured interview. Structured interview conducted in September 2019 in all studied herds, on the antibiotic usage during the last 12 months.
Statistics. Herd level statistical analyzes using one-tailed Fisher’s exact test, comparing resistance (Yes/No) to any of the antibiotics included in the panels, resistance to single selected antibiotic substances (tetracycline and penicillin/ampicillin) and the presence of multi-drug resistance, to the herd size and treatment regimens.
Antibiotic resistance of E. coli. Minimum inhibitory concentrations (mg/L) of the 52 E. coli isolates.
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Ikwap, K., Gertzell, E., Hansson, I. et al. The presence of antibiotic-resistant Staphylococcus spp. and Escherichia coli in smallholder pig farms in Uganda. BMC Vet Res 17, 31 (2021). https://doi.org/10.1186/s12917-020-02727-3
- Anti-microbial resistance
- Broth micro-dilution
- Veterinary medicine