- Methodology article
- Open Access
Rapid identification and quantification of Campylobacter coli and Campylobacter jejuniby real-time PCR in pure cultures and in complex samples
© Leblanc-Maridor et al; licensee BioMed Central Ltd. 2011
Received: 14 October 2010
Accepted: 22 May 2011
Published: 22 May 2011
Campylobacter spp., especially Campylobacter jejuni (C. jejuni) and Campylobacter coli (C. coli), are recognized as the leading human foodborne pathogens in developed countries. Livestock animals carrying Campylobacter pose an important risk for human contamination. Pigs are known to be frequently colonized with Campylobacter, especially C. coli, and to excrete high numbers of this pathogen in their faeces. Molecular tools, notably real-time PCR, provide an effective, rapid, and sensitive alternative to culture-based methods for the detection of C. coli and C. jejuni in various substrates. In order to serve as a diagnostic tool supporting Campylobacter epidemiology, we developed a quantitative real-time PCR method for species-specific detection and quantification of C. coli and C. jejuni directly in faecal, feed, and environmental samples.
With a sensitivity of 10 genome copies and a linear range of seven to eight orders of magnitude, the C. coli and C. jejuni real-time PCR assays allowed a precise quantification of purified DNA from C. coli and C. jejuni. The assays were highly specific and showed a 6-log-linear dynamic range of quantification with a quantitative detection limit of approximately 2.5 × 102 CFU/g of faeces, 1.3 × 102 CFU/g of feed, and 1.0 × 103 CFU/m2 for the environmental samples. Compared to the results obtained by culture, both C. coli and C. jejuni real-time PCR assays exhibited a specificity of 96.2% with a kappa of 0.94 and 0.89 respectively. For faecal samples of experimentally infected pigs, the coefficients of correlation between the C. coli or C. jejuni real-time PCR assay and culture enumeration were R2 = 0.90 and R2 = 0.93 respectively.
The C. coli and C. jejuni real-time quantitative PCR assays developed in this study provide a method capable of directly detecting and quantifying C. coli and C. jejuni in faeces, feed, and environmental samples. These assays represent a new diagnostic tool for studying the epidemiology of Campylobacter by, for instance, investigating the carriage and excretion of C. coli and C. jejuni by pigs from conventional herds.
Campylobacter spp. are recognized as the leading human foodborne pathogens in developed countries [1, 2]. Within the genus Campylobacter, the thermophilic species Campylobacter jejuni (C. jejuni) and Campylobacter coli (C. coli) are the most frequently associated with illness, accounting for over 95% of infections (respectively responsible for 80 to 85% and 10 to 15%) . These two species commonly live in the intestinal tract of birds and mammals, including food production animals and pets, without causing clinical signs . Livestock animals carrying Campylobacter pose an important risk for human infection from contamination of carcasses at slaughter, of milk, and water contaminated by livestock wastes and slurries [4–6]. Research carried out in Europe has shown the dominance of C. jejuni in animal intestinal tracts, for example, broiler chickens, cattle, and wild-living mammals and birds [2, 7, 8]. Pigs are known to be frequently infected with Campylobacter (prevalence between 50% and 100%), to exhibit high counts of this pathogen in their faeces (ranging from 102 to 107 Colony Forming Units (CFU) of Campylobacter per gram), and to show a dominance of C. coli [9–11]. Nevertheless, some studies have found a dominance of C. jejuni in pigs and of C. coli in chickens [12–15]. Given these contradictory data, the risk of foodborne disease associated with animal species is not clear. In terms of risk assessment, the ability to differentiate and quantify these two species is essential to describe more precisely the presence of Campylobacter in livestock animals.
The identification of Campylobacter using conventional methods is slow (culture-based methods can take up to five days) and problematic due to their fastidious growth requirements and biochemical inertness [16, 17]. Moreover, the detection of C. coli and/or C. jejuni in complex substrates like faeces or environmental samples is difficult as the culture conditions have to be selective enough to avoid overgrowth from competiting organisms. Additionally these bacteria may enter into a viable but nonculturable state (VBNC) . The correct differentiation of thermophilic Campylobacter spp., especially C. coli and C. jejuni, by phenotypic tests is difficult and hippurate hydrolysis test used to distinguish these two species is often problematic . Furthermore, C. jejuni may also coexist with C. coli in pigs, but at 10-100-fold lower numbers than C. coli [10, 11, 20], so C. jejuni will be less frequently isolated from such samples because only a few colonies are identified to the species level with conventional culturing and biochemical testing techniques. Molecular methods are an alternative to the bacteriological method for the detection of C. coli and C. jejuni in various substrates [1, 17, 21–24]. Real-time PCR has provided a reliable tool to detect and to quantify C. jejuni and/or C. coli in pure culture , in poultry, milk, or water [26, 27], and in complex substrates like food products [28–30] and faecal samples [20, 31–33]. However, of the real-time PCR techniques developed, none were capable of differentiating and quantifying C. coli and C. jejuni directly from pig faecal, feed, and environmental samples.
The present study aimed to develop a species-specific real-time PCR method to detect and quantify C. coli and C. jejuni directly in pig faecal, feed, and environmental samples. The first step in the development of the assay was the definition of the multiplex PCR assay to quantify C. coli and C. jejuni isolates from bacterial cultures. These real-time PCR assays were coupled with a modified DNA extraction protocol and then examined for their ability: (i) to evaluate DNA purification with different parameters (potential presence of PCR inhibitory compounds, DNA yield, and reproducibility), (ii) to measure the sensitivity and the specificity of PCR-based detection in faecal samples, and (iii) to detect C. jejuni among predominant C. coli. Finally, the last step was the application of the real-time PCR assays to detect and quantify C. coli and C. jejuni in complex substrates like feed, environmental samples, and faeces from experimentally as well as naturally infected pigs. The bacterial culture was used as a gold standard for their validation.
Specificity, sensitivity and linear range of the real-time PCR assays
List of strains used for the validation of specificity of Campylobacter coli and Campylobacter jejuni real-time PCR assays
Bacterial species (n)
Name or origin of strain
C. colireal-time PCR identification
C. jejunireal-time PCR identification
Campylobacter coli (2)
CCUG 11283, CIP 7081
C. coli pig isolates (25)
C. coli poultry isolates (25)
C. coli human isolates (25)
Campylobacter jejuni subsp jejuni (3)
CCUG 11284, NCTC 11168, NCTC 81176
C. jejuni poultry isolates (25)
C. jejuni human isolates (25)
Anses, ENVN-INRA, CNR-CH
Campylobacter fetus subsp fetus (2)
CCUG 68231, CIP 2595396
Campylobacter fetus subsp venerealis
Campylobacter lari (3)
CCUG 23947, ATCC 35222, CIP 107080
Campylobacter upsaliensis (2)
CCUG 14913, CIP 400
Helicobacter pylori (3)
CIP 103995, CIP 26695, CIP 101260
Listeria monocytogenes (3)
CIP 103575, ATCC 895807, ATCC 19115
Listeria innocua (3)
CCUG 15531, ENVN-INRA
Salmonella enterica serovar enteridis
S. enterica serovar typhimurium
Enterococcus faecalis (2)
CIP 103013, CCUG 19916
Pseudomonas aeruginosa (2)
Enterobacter aerogenes (2)
Staphylococcus aureus (2)
Y. ruckeri fish isolates (5)
Precision of the C. jejuni and C. coli real-time PCR assays
Intra- and Inter-assay variabilities of C. coli and C. jejuni real-time PCR assays for the standard curves generated with purified genomic DNA of C. coli CIP 70.81 and C. jejuni NCTC 11168, ranging from 101 to 108 genome copies per PCR reaction (genome copy number) and with DNA extracted from Campylobacter-negative pig faecal samples spiked with different amounts of C. coli and C. jejuni ranging from 2 × 102 to 2 × 107 CFU/g of faeces including the DNA extraction procedure (CFU/g of faeces)
Genome copy number
CFU/g of faeces
CV c (%)
CV j (%)
CV c (%)
CV j (%)
2 × 10 8
2 × 10 7
2 × 10 6
2 × 10 5
2 × 10 4
2 × 10 3
2 × 10 2
Validation of the real time PCR assays for the analysis of faecal, feed, and environmental samples spiked with C. coli and C. jejuni
Samples were checked for PCR inhibition in a separate test using a bacterial internal amplification and extraction control . Inhibitors of real-time PCR were identified in 4% of the examined samples, which were consequently removed from the quantification study.
To obtain values for the intra- and inter-assay variation of each real-time PCR assay with field samples, DNA extracted from the Campylobacter-negative spiked faecal samples was subjected to each real-time PCR in ten duplicates, with 10 different mixes performed on different runs. The results are reported in Table 2. The CV of the Ct values for the ten different intra-assay experiments ranged from 1.15 to 4.40% for C. coli real-time PCR and from 0.91 to 2.53% for C. jejuni real-time PCR. The standard curves were y = -3.33x + 45.82 with R2 = 0.98 for C. coli and y = -3.24x + 46.00 with R2 = 0.98 for C. jejuni. The CV of the Ct values for the ten different inter-assay experiments, including the DNA extraction procedure, ranged from 0.57 to 2.58% and from 0.70 to 2.10% respectively for C. coli and C. jejuni real-time PCR assays. The mean standard curves were y = -3.36x + 43.70 and y = -3.25x + 46.20 respectively.
Analysis of faecal samples of experimentally infected pigs
Comparison of real-time PCR and microaerobic culture in faecal samples of experimentally infected pigs for the detection of (3.1) Campylobacter coli and (3.2) Campylobacter jejuni
3.1 Campylobacter coli detection
3.2 Campylobacter jejuni detection
Analysis of field samples of naturally contaminated pigs
No C. jejuni was identified among the faecal, feed, and environmental samples from the different pig herds by conventional PCR or by our C. jejuni real-time PCR assay. Conversely, all the Campylobacter tested were identified as C. coli by both methods.
Comparison of Campylobacter coli real-time PCR and microaerobic culture in (4.1) faecal, (4.2) feed, and (4.3) environmental samples of naturally contaminated pigs
4.1 Campylobacter coli detection in faecal samples
4.2 Campylobacter coli detection in feed samples
4.3 Campylobacter coli detection in environmental samples
For the different field samples tested, the quantification results obtained by C. coli real-time PCR matched equally the results obtained by bacterial culture: 58% of the samples had a difference in cell number of less than 1 log, 37% of less than 2 logs, and 5% of less than 3 logs.
The real-time PCR asays developed in this study provide an effective, rapide, and sensitive alternative method to culture-based methods for the detection and the quantification of C. coli and C. jejuni in pure cultures and in complex samples.
To use real-time PCR for quantitative measurements and to ensure a correct quantification, information on both linear range and amplification efficiency of the real-time PCR assay must be available. With a quantitative detection limit of 10 genome copies, an amplification efficiency of 99%, and a linear range of seven to eight orders of magnitude, the C. coli and C. jejuni real-time PCR assays allowed a precise quantification of C. coli or C. jejuni DNA amounts extracted from pure culture preparations. The specificity of the assays was assessed (i) by the species-specific amplification of DNA from different field strains/isolates of C. coli and C. jejuni, and (ii) by the absence of amplification from DNA isolated from 30 pig faecal, feed, and environmental samples previously determined to be Campylobacter-free by culture. The real-time PCR assays were also shown to be highly specific since no PCR amplicons were detected when the method was applied to DNA from different bacterial reference strains, including different Campylobacter species, Campylobacter-related bacteria, and other bacteria. Both intra- and inter-assay coefficients of variation of the Ct values for the purified genomic DNA were satisfactorily low and in concordance with those reported for other molecular assays based on PCR amplification . They confirmed the reliability and the accuracy of the technical setup over time and over the complete range of quantification.
The technique was developed to detect and quantify C. coli and/or C. jejuni directly in pig faecal, feed, and environmental samples. In order to determine the detection limits of C. coli and C. jejuni real-time PCR assays for field samples, Campylobacter-negative faecal samples were spiked with 10-fold dilutions of the Campylobacter suspensions of each reference strain (C. jejuni NCTC 11168 and C. coli CIP 70.81). Standard curves for environmental and feed samples were constructed in a similar way. The established C. coli and C. jejuni real-time PCR assays proved highly sensitive (with a quantitative detection limit of approximately 2.5 × 102 CFU/g of faeces, 1.3 × 102 CFU/g of feed, and 1.0 × 103 CFU/m2 for the environmental samples) and were linear over a range of six orders of magnitude (from 2.0 × 102 to 2.0 × 107 CFU/g of faeces). Both intra- and inter-assay coefficients of variation of the Ct values for the DNA extracted from Campylobacter-negative faecal samples did not differ significantly. This may indicate that the main reason for variation is not due to pipetting errors in setting up the PCR assay but may be caused by contaminants from the fecal samples. Nevertheless, we did not observe systematically lower CV values of intra- and inter-assay variations with purified genomic DNA. This does not support the hypothesis that inhibitors and contaminants may interfere with uniform and consistent dilution as well as the amplification of target DNA.
Samples tested in this study constitute complex biological substrates due to the presence of (i) numerous types of bacteria, (ii) different kinds of inhibitors, and (iii) food degradation products [36, 37]. Moreover, contrary to faecal and caecal chicken samples [35, 38], the consistency and the composition of pig faecal samples are highly variable and heterogeneous (i) between individuals, (ii) over time according to the age of the animals, and (iii) depending on the diet components in the same way as for cattle faeces [39, 40]. In this study, we sampled faeces of sows, piglets, weaners, and finishers, exhibiting considerable heterogeneity (water content, presence of mucus, and fiber content). All these variables may have an impact on the DNA extraction process and inhibitor removal, affecting the quality and the quantity of DNA obtained, thereby limiting the sensitivity of molecular studies. The modified sample preparation procedure, which included (i) a large volume of faeces (5 g fresh weight), (ii) a boiling step known to remove inhibitors of the Taq polymerase , and (iii) the use of a DNA extraction kit, allowed a better homogenization of the faeces and achieved partial removal of inhibitors. No difference was noticed between real-time PCR assays and culture at both qualitative and quantitative levels for faecal samples differing by the composition, the consistency, or the age of the sampled animal (data not shown). Nevertheless, in this study, the potential presence of PCR inhibitory compounds was in parallel assessed with the use of an internal bacterial control of extraction and amplification in a separate real-time PCR test . Inhibitors of real-time PCR were identified only in 4% of the examined samples, which were consequently removed from the quantification study. Moreover, the DNA extraction step reproducibility, an important parameter when evaluating the DNA purification , was satisfactory proved with the low CV values of the inter-assay variability including the DNA extraction procedure.
Three faecal samples of experimentally infected pigs, detected as negative by PCR and direct streaking, were positive by culture after an enrichment step (one out of 41 and two out of 26 for C. coli and C. jejuni real-time PCR assays respectively) leading to a sensitivity of 97.6% and 92.3%. Although the internal control was positive, we cannot exclude the hypothesis of inhibition of C. coli and C. jejuni amplification. Indeed, it was previously reported that some PCR primers are more markedly affected than others by impurities present in DNA preparations [43, 44]. Moreover, it could be false negative PCR samples, which have been below the detection limit of the two real-time PCR assays. Genetic variability among the isolates of Campylobacter spp., which has been demonstrated previously [45–47], can also affect the efficacy of a PCR if changes occur within one or both of the binding sites [17, 46]. The enrichment step enhanced the sensitivity of the bacteriological method by lowering the detection limit. Nevertheless, even if it is helpful for poorly contaminated samples, researchers have reported several cases in which C. jejuni signals detected by direct PCR disappeared after enrichment. Conversely C. coli signals were maintained when present before enrichment, or else became detectable when undetectable before enrichment [24, 48]. This suggests that the enrichment media may favour the growth of one Campylobacter species comparatively to the other .
Furthermore, for the experimentally infected pigs, only one culture-negative faecal sample was positive by real-time PCR for each target leading to a specificity of 96.2% for both C. coli and C. jejuni real-time PCR assays. These results may be due to the presence of viable but nonculturable (VBNC) forms or dead bacteria cells, since DNA-based tests detect all DNA of the extract from live as well as dead bacteria [27, 29, 50]. If this is the case, it is another advantage of these real-time PCR assays as Campylobacter cells in a VBNC state may potentially be still infectious [18, 51]. The bacteriological method may also explain these results given that the sensitivity of culture may vary depending on the Campylobacter spp. due to differences in susceptibility to antibiotics present in selective agar . Moreover, in pig faceal and environmental samples, the enrichment of C. jejuni could be difficult due to the presence of a high background flora and due to the more numerous C. coli quantity .
Finally, for the faecal samples of experimentally infected pigs, we observed a good correlation at the quantitative level between culture enumeration and quantitative PCR for both C. coli and C. jejuni real-time PCR assays (R2 = 0.90 and R2 = 0.93 respectively). Among the PCR-culture positive samples, the real-time PCR quantification seems to be accurate compared to the culture enumeration used as a gold standard. Indeed, more than 95% of the samples with a difference in cell number of less than 2 logs, of these 72.5% and 67% less than 1 log respectively for C. coli and C. jejuni real-time PCR assays. The observed discrepancy might be due to the possible presence of VBNC forms, dead cells and antagonistic bacterial species. Another possibility could be the impact of dilution factors used for quantitative culture or an insufficient homogenization of the samples. This method provides a mean to identify and quantify at the species level C. coli and C. jejuni directly from faecal, feed, and environmental samples without requiring an enrichment step. For the different field samples tested, the qualitative data (specificity and sensitivity) as well as the quantification results obtained by C. coli real-time PCR matched equally the results obtained by bacterial culture. In this study, no C. jejuni was identified among the faecal, feed, and environmental samples from the different pig herds by conventional PCR or by our C. jejuni real-time PCR assay. Conversely, all the Campylobacter tested were identified as C. coli by both methods. In France, pigs were found to be almost always contaminated by C. coli, these first results confirmed this predominance. Nevertheless, given that we can find both species in pigs [10, 12–14], these real-time PCR assays allow a direct and rapid investigation of the carriage and the excretion of C. coli and C. jejuni in conventional pigs.
The real-time PCR assays for C. coli and C. jejuni described in this study have several advantages over culture-based techniques. These include allowing a large increase in throughput, enabling simultaneous processing of several samples (the real-time PCR can be run in a 96-well format and many steps in the assay can be automated), and reducing the total time required for analysis. The identification at the species level and the quantification on the entire DNA extracted from faecal, feed, and environmental samples is a new tool to enhance our understanding of the epidemiology of Campylobacter. In terms of risk assessment, this ability to differentiate and quantify these two species permits a more precise description of the carriage and excretion of C. coli and C. jejuni by livestock animals.
Bacterial strains and culture conditions
Different Campylobacter spp., Helicobacter, Wolinella, and Arcobacter reference strains were used to test the specificity of primers and probes for real-time PCR identification and differentiation of C. coli and C. jejuni (Table 1). In addition, we have tested 50 C. jejuni and 75 C. coli isolates (from human, poultry, and pig origin) as well as other enteric bacteria (clinical isolates and reference strains) selected from our in-house collection, the collection of the French Agency for Food, Environmental and occupational Health and Safety (Anses, Ploufragan), and the collection of the French National Reference Center for Campylobacter and Helicobacter (CNR-CH, Bordeaux). Strains were stored at -80°C in brain heart infusion broth (Difco, Detroit, Michigan) containing 20% (v/v) glycerol. Moreover, for the real-time PCR reactions, we used the two reference strains C. jejuni NCTC 11168 and C. coli CIP 70.81 as positive controls as well as Listeria monocytogenes ATCC 19115 and Escherichia coli CIP V517 as negative controls. Campylobacter strains were grown at 25, 37 or 41.5°C for 48 h in a microaerobic atmosphere (5% O2, 10% CO2, 85% N2) on Karmali agar plates (Oxoid, Dardilly, France). Arcobacter, Helicobacter, and Wolinella were grown at 37°C for 48 h on Columbia Blood agar plates (Oxoid, Dardilly, France) with 5% of defibrinated sheep blood (AES Chemunex, Combourg, France) and Enterobacter aerogenes on Purple Lactose agar plates (BCP, AES Chemunex, Combourg, France) for 24 h. All the other bacteria listed in Table 1 were grown under appropriate culture conditions at 30 or 37°C for 24 h on Tryptone soja agar yeast extract plates (TSAYE Oxoid, Dardilly, France).
DNA extraction from bacterial cultures
Genomic DNA from each bacterial culture was extracted using the Nucleospin® Tissue mini-kit (Macherey Nagel, Hoerdt, France) and according to the manufacturer's instructions. The concentration of isolated double stranded DNA was determined by measuring the optical density at 260 nm with the Spectronic® Genesys™ 5 (Spectronic Instruments Inc., New York, USA). The purity was assessed by the examination of 260/280 nm optical density ratios . All DNA samples classified as pure (i.e. having a 260/280 nm optical density ratio between 1.8 and 2.0) were adjusted to 20 ng μL-1 in TE buffer (10 mmol Tris-HCl, 1 mmol EDTA, pH 7.6) and stored at -20°C until required for analysis.
Construction of the standard curves with purified genomic DNA
Total genomic DNA of C. jejuni NCTC 11168 and C. coli CIP 70.81 cultures were extracted as described above. The genome copy numbers of C. jejuni and C. coli in 100 ng of DNA (for one PCR reaction) was calculated on the basis of the genome size (1 640 Kbp for C. jejuni, 1 860 Kbp for C. coli) [54–56] and was equal to 5.2 × 107 and 4.6 × 107 copies respectively. After DNA quantitation by spectrofotometrical analysis with the Spectronic® Genesys™ 5, 10-fold dilutions of each extract were produced in TE buffer, representing 101 to 108 genome copies of C. jejuni per 5 μL of template (PCR reaction) and 0.3 × 101 to 3.0 × 108 genome copies of C. coli per 5 μL of template (PCR reaction). Moreover, a standard curve with roughly equal genome copies of C. jejuni and C. coli together was produced for each PCR assay. Serial DNA dilutions were aliquoted: some were stocked at 4°C to be use directly, others were stored frozen at -20°C and thawed once for use.
Fifteen Campylobacter-negative faecal samples were obtained from specific pathogen-free (SPF) sows and piglets from the high-security barn at the Anses centre (Ploufragan, France). Moreover, five Campylobacter-negative feed samples and 10 Campylobacter-negative environmental samples were collected from the same high-security barns. These samples were used to test the specificity and/or the analytical sensitivity of the real-time PCR assays. For the environmental samples, each pen of pigs was sampled on the bottom of the wall and pen partitions using swabs (sterile square pieces of cotton cloth (32 . 32 cm) moistened with isotonic saline solution) (Sodibox, La Forêt-Fouesnant, France). The swabs were placed in a sterile bag before to be analyzed.
Additional faecal, feed, and environmental samples
Faecal samples were obtained from both pigs experimentally inoculated with 5 × 107 CFU of Campylobacter (n = 119, respectively 67 C. coli and 52 C. jejuni faecal samples)  and naturally contaminated pigs in five conventional herds (n = 146). Given that pig faeces can be highly heterogeneous, rectal faecal samples were collected individually from naturally contaminated (i) sows, (ii) pigs aged three to 16 weeks, and (iii) piglets aged one to three weeks. Additionally, in the five conventional herds, 86 environmental swabs of pig pens (either empty or with animals) and 50 feed samples were collected. The swabbed surface area was measured each time.
Sample processing and experimental conditions
All samples were examined within four hours after sampling for Campylobacter spp. quantification by conventional culture and for species-identification by the PCR described by Denis et al. (1999)  as well as for species-specific quantification by real-time PCR assays. All animals of this study were housed and treated in accordance with the regulations of the local veterinary office (Direction des Services Vétérinaires des Côtes d'Armor, France). The animal experimention was carried out following the international recognized guidelines. All the animals were reared in isolation rooms with controlled air flow .
DNA preparation for real-time PCR-based quantification
DNA isolation from the faecal, feed, and environmental samples was performed using a modified extraction protocol of the Nucleospin® Tissue mini-kit (Macherey Nagel, Hoerdt, France) with a preliminary step of boiling to remove inhibitors of the Taq polymerase . Five grams of sample (faeces or feed) were diluted in 5 mL of sterile water (for smaller amounts, an equivalent quantity of sterile water (w/w) was added). The environmental swabs, placed into sterile bags, were stomached for 2 min with 10 mL of sterile water. The sample solutions of faeces, feed, and swabs were boiled for 10 min, chilled on ice, and centrifuged (8000 g, 5 min). For each sample, 250 μL of supernatant was extracted using the Nucleospin® Tissue mini-kit according to the manufacturer's instructions. Finally, DNA preparations, eluted in 100 μL of elution buffer purchased in the kit, were stored at +4°C prior to use.
Control of PCR inhibition
To test the presence of PCR inhibitors in the DNA isolated from the samples, a fixed amount of the bacterium Yersinia ruckeri was added to each sample before the DNA extraction. This internal bacterial amplification and extraction control was quantified in a separate well using a real-time PCR test described in a previous work . Samples with PCR inhibition were then removed for the rest of the study.
Enumeration of Campylobacter spp. and species identification
Ten grams of fresh faeces, ten grams of feed, and the environmental swabs were vortexed in 90 mL of Preston broth (Oxoid, Dardilly, France) with a Preston antibiotic supplement (Oxoid, Dardilly, France) (for rectal swabs, 9 mL of Preston broth was added to one gram of faeces). For Campylobacter numeration, 100 μL of a ten-fold dilution serie (10-1 to 10-5) were plated both on Karmali agar (Oxoid, Dardilly, France) and on Butzler agar (Oxoid, Dardilly, France) and incubated for 24 to 72 h at 41.5°C in microaerobic conditions. To promote the detection of Campylobacter in samples harbouring less than 100 Colony Forming Unit of Campylobacter per gram of faeces (CFU/g of faeces), a second plating was carried out 24 h after broth enrichment and incubated 48 h. Thermophilic Campylobacter were cultured at 41.5°C in microaerobic conditions. For direct streaking and selective enrichment, the Campylobacter suspect colonies on Karmali or Butzler plates were confirmed by microscopy (cell morphology) and conventional PCR ). The number of CFU/g of faeces or feed as well as the number of CFU/m2 for the environmental samples were thus calculated. Finally, material from Campylobacter suspect colonies was suspended in TE buffer and subdued to DNA extraction and the species-specific PCR described by Denis et al. (1999)  for differentiation between C. coli and C. jejuni.
Real-time PCR primers and probes
PCR primers and probes used in the species-specific real-time PCR assays
Primer or Probea
Nucleotide sequence 5'-3'
Location within target
Target Gene detectedb
Lagier et al. (2004)
Campylobacter coli glyA gene (125 bp)
glyA-P MGB Probe
Campylobacter jejuni hipO gene (124 bp)
hipO-P MGB Probe
To optimize the real-time PCR reaction and to improve the specificity and the mismatch discrimination, shorter Minor Groove Binder (MgB) probes have been designed [59–62]. At the 5'end, the C. coli probe was linked to the fluorophore FAM and the C. jejuni probe to the fluorophore VIC. The C. jejuni and C. coli species-specific primers and TaqMan® MgB probe sets were thus designed with Primer Express software version 2.0 (Applied Biosystems, Foster city, CA, USA) according to the recommendations of the manufacturer (Table 5). This software was used to choose the best combinations of each primers-probe set values. Finally, the selected primers and probes were checked for homology to non-target sequences by a search with the BLAST program of the National Center for Biotechnology Information (NCBI). Primers and MgB probes were synthesized by Applied Biosystems and stored at -20°C prior to use.
Real-time PCR amplification
Reactions were done in 20 μL PCR mixtures containing 10 μL of 1X Taqman Universal PCR Mastermix (AmpliTaq Gold™ DNA polymerase, dNTPs, Passive reference (ROX), and optimised buffer components including 5 mM MgCl2), 400 nM of each primer (glyA-R and glyA-F for C. coli real-time PCR assay, hipO-R and hipO-F for C. jejuni real-time PCR assay), 200 nM of the probe (glyA-P and hipO-P respectively), and 5 μL of template DNA. The thermal cycle protocol used was the following: activation of the Taq DNA polymerase at 95°C for 10 min, then 45 or 48 cycles of 15 s at 95°C and 60 s at 60°C. Thermal cycling, fluorescent data collection, and data analysis were carried out with the ABI PRISM® 7300 Sequence Detection System (Applied Biosystems) according to the manufacturer's instructions. Fluorescence of FAM and VIC was measured at their respective wavelengths during the annealing/elongation step of each cycle. After real-time data acquisition, the baseline cycles for the FAM and VIC signals were set from cycle three to three cycles below the cycle at which the first signal appeared and the threshold value at the point at which the fluorescence exceeded 10 times the standard deviation of the mean baseline emission. The threshold cycle (Ct) is the first PCR cycle at which a statistically significant increase in fluorescent signal is detected. All reactions were carried out alongside a non template control containing all reagents except DNA, positive controls containing DNA from reference strains (C. jejuni NCTC 11168 and/or C. coli CIP 70.81), and negative controls containing DNA from Listeria monocytogenes ATCC 19115 and from Escherichia coli CIP V517. All the DNA extractions were done as described before. Each control was run in triplicate and each sample in duplicate.
Evaluation of performance of the real-time PCR assays
Specificity and sensitivity
The specificity of each real-time PCR assay was first assessed with purified genomic DNA preparations (about 106 genome copies per PCR reaction) of different bacterial strains (Table 1) and then with DNA extracted from 30 Campylobacter-negative faecal, feed, and environmental samples as defined above. This screening strategy, described previously by Lagier et al. (2004) , ensure the specificity of the primers and probes for C. jejuni and C. coli only in field samples. Double-stranded DNA extracted from the 30 Campylobacter-negative faecal, feed, and environmental samples was examined in duplicate with each real-time PCR assay.
The sensitivity for each PCR assay was determined using the standard curves prepared with purified genomic DNA of cultures of C. jejuni NCTC 11168 and C. coli CIP 70.81, ranging from 101 to 108 genome copies per 5 μL of template (PCR reaction). In order to mimic realistic conditions and to determine the detection limits of C. coli and C. jejuni real-time PCR assays for field samples, different standard curves were prepared to quantify C. coli or C. jejuni in faecal, feed, and environmental samples. Campylobacter-negative faecal samples were spiked with 10-fold dilutions series of viable suspensions of each reference strain (C. jejuni NCTC 11168 and C. coli CIP 70.81), ranging from 101 to 108 Colony Forming Units per gram of faeces (CFU/g). Standard curves for environmental and feed samples were constructed in a similar way. DNA was extracted from each of the spiked samples and tested in real-time PCR, where the standard curves were created automatically by the ABI PRISM® 7300 Sequence Detection System Software by plotting the Ct values against each standard dilution of known concentration.
Intra- and inter- assay variabilities
The assay variability was established by repeatedly testing samples containing several concentrations of C. coli and C. jejuni spanning the whole range covered by each real-time PCR in different assays (10 consecutive runs) and within an assay (10 duplicates in the same assay), in order to calculate the inter- and intra-assay coefficients of variation (CV) for the Ct values experimentally determined, as previously described .
To assess the intra-assay variation, each dilution of purified genomic DNA of cultures from C. jejuni NCTC 11168 and C. coli CIP 70.81 from approximately 101 to 108 CFU were measured 10 times each within one PCR run. The inter-assay variation was evaluated with the same different dilutions of purified genomic DNA in 10 independent PCR experiments on different days (10 different runs). For each PCR run, each dilution point was tested in duplicate and the mean standard curve was used for quantity estimation.
To assess the method with field samples, the values for the intra- and inter-assay variations of the real-time PCR assays were obtained with the DNA extracted from the Campylobacter-negative spiked samples. To assess the intra-assay variation, DNA extracted from the Campylobacter-negative faecal samples spiked with 10-fold dilutions of the Campylobacter suspensions, ranging from 2.5 × 107 to 2.5 × 102 CFU of C. coli/g of faeces and from 2.0 × 107 to 2.0 × 102 CFU of C. jejuni/g of faeces, were measured 10 times each within one real-time PCR run. The inter-assay variation was evaluated with different dilutions of DNA extracted each time with a specific extraction from the Campylobacter-negative spiked faecal samples in 10 independent real-time PCR experiments on different days. For each real-time PCR run (C. coli and C. jejuni real-time PCR assays), each dilution point was tested in duplicate and the mean standard curves were used for quantity estimation. The CV of the Ct values were calculated for the ten different inter-assay experiments. They illustrate the variability of the Ct values obtained between experiments including the specific DNA extraction procedure and the amplification step.
Use of the standard curves
The standard curves were thus used (i) to evaluate the sensitivity of the real-time PCR assays, (ii) to assess the intra- and inter-assay variabilities, and (iii) to allow a reliable quantification of C. jejuni and C. coli in pure cultures or in the field samples.
PCR amplification efficiency (E) was estimated using the slope of the standard curve and the formula E = 10(-1/slope)-1. A reaction with 100% efficiency will generate a slope of -3.32. Data analysis was performed using the SDS software (Applied Biosystems).
The 119 field samples from the experimental infection were evaluated in parallel with the real-time PCR assays and the bacterial culture described in this study. All data analyses were performed with Microsoft excel and SAS Systems version 8 (SAS, Cary, N.C.). Specificity and sensitivity were assessed using the bacterial culture as a gold standard. The sensitivity was calculated as a/(a+c), where a is the number of samples found positive by both real-time PCR and bacterial culture (direct inoculation or after selective enrichment) and c is the number of samples positive by bacterial culture but negative by real-time PCR. The specificity was calculated as d/(b+d), where d is the number of samples negative by both methods and b is the number of samples positive by real-time PCR but negative by bacterial culture. Kappa-statistic was used to measure the agreement between the microaerobic cultivation and each species-specific real-time PCR assay .
The authors thank Sebastien Tessier for technical assistance during his practice training period and the staff of the BioEpAR and MAE units at the Veterinary School of Nantes, notably Jean-Yves Audiart, Françoise Armand, Emmanuelle Blandin, and Françoise Leray.
We thank especially Francis Mégraud and Philippe Lehours of the French National Reference Center for Campylobacter and Helicobacter (Bordeaux, France) for providing us reference strains from their collection and field strains from clinical cases.
This work was supported by grants from INRA, Anses, and the Region Pays de La Loire.
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