A nested-PCR with an Internal Amplification Control for the detection and differentiation of Bartonella henselae and B. clarridgeiae: An examination of cats in Trinidad
© Rampersad et al; licensee BioMed Central Ltd. 2005
Received: 14 April 2005
Accepted: 12 August 2005
Published: 12 August 2005
Bartonella species are bacterial blood parasites of animals capable of causing disease in both animals and man. Cat-Scratch Disease (CSD) in humans is caused mainly by Bartonella henselae and is acquired from the cat, which serves as a reservoir for the bacteria. A second species, B. clarridgeiae is also implicated in the disease. Diagnosis of Bartonellosis by culture requires a week or more of incubation on enriched media containing blood, and recovery is often complicated by faster growing contaminating bacteria and fungi. PCR has been explored as an alternative to culture for both the detection and species identification of Bartonella, however sensitivity problems have been reported and false negative reactions due to blood inhibitors have not generally been addressed in test design.
A novel, nested-PCR was designed for the detection of Bartonella henselae and B. clarridgeiae based on the strategy of targeting species-specific size differences in the 16S-23S rDNA intergenic regions. An Internal Amplification Control was used for detecting PCR inhibition. The nested-PCR was utilized in a study on 103 blood samples from pet and stray cats in Trinidad.
None of the samples were positive by primary PCR, but the Nested-PCR detected Bartonella in 32/103 (31%) cats where 16 were infected with only B. henselae, 13 with only B. clarridgeiae and 3 with both species. Of 22 stray cats housed at an animal shelter, 13 (59%) were positive for either or both species, supporting the reported increased incidence of Bartonella among feral cats.
The usefulness of a single PCR for the detection of Bartonella henselae and B. clarridgeiae in the blood of cats is questionable. A nested-PCR offers increased sensitivity over a primary PCR and should be evaluated with currently used methods for the routine detection and speciation of Bartonella henselae and B. clarridgeiae. In Trinidad, B. henselae and B. clarridgeiae are the predominant species in cats and infection appears highest with stray cats, however B. clarridgeiae may be present at levels similar to that of B. henselae in the pet population.
Bartonella are fastidious, gram-negative, bacteria comprised of at least 19 species and 3 subspecies  that are obligate parasites of the blood in reservoir animals. Bartonella species are considered emerging zoonotic pathogens  and may be involved in a number of disease presentations including angiomatosis  and ocular manifestations . Similarly, Bartonella species are being associated with disease in their animal hosts (see reviews [2, 5]. The role of cats as a reservoir for human Bartonellosis is well documented however probably incomplete. Studies suggest that other Bartonella species, known to cause disease in humans, are found in the cat (see for example  and . Of these, Bartonella henselae and, to a lesser extent, Bartonella clarridgeiae are known to cause Cat-Scratch Disease (CSD) in humans ; see also  for review of CSD.
As a fastidious organism, Bartonella usually requires over a week of incubation for primary isolation. The slow growth of the organism complicates its isolation since faster growing bacteria and fungi can overrun the plate. Thus various types of tests using Polymerase Chain Reaction (PCR) have been explored as a diagnostic tool for the detection and identification of Bartonella species from blood [10–12]. Previously, Jensen et al.,  developed a PCR for the detection of Bartonella that targets species-specific size differences in the 16S-23S rDNA intergenic region. However, as a primary PCR, it was questionable if the sensitivity of the test was optimal for the detection of relatively low numbers of bacteria  and a control for the detection of false-negative reactions due to inhibition by blood components was not addressed. Herein we describe the development of a nested-PCR for the detection of B. henselae and B. clarridgeiae based on the strategy of species-specific size differences in the 16S-23S rDNA intergenic region that includes an Internal Amplification Control for PCR inhibitors. The test was evaluated on the blood of 103 apparently healthy cats in Trinidad to investigate the presence of these organisms in the local cat population and to verify the test's ability to detect these organisms in the blood of apparently healthy animals.
All samples were collected over an 11 month period in 2001. Blood samples were collected in commercial blood collection tubes containing EDTA and transported to the laboratory on ice, where possible the same day, or stored at 4°C until transported. Samples were collected from geographically distinct areas in Trinidad including an animal shelter, private veterinary clinics and the Veterinary Hospital located at the University of the West Indies' School of Veterinary Medicine by both Veterinarians and final year veterinary students.
DNA was extracted from whole blood according to the method of Boom et al.,  with modifications as described by Rampersad et al., . One microlitre of blood-extracted DNA template was used in the primary PCR reaction and 1 μl of the primary reaction was used in the nested reaction. In order to minimize contamination, separate rooms were used for preparing the PCR reaction mix, template preparation, gel electrophoresis, and performing nested reactions. Nested reactions were performed in a biosafety hood where 1 μl of primary reaction was delivered to a nested tube with a 1 μl urine loop, the end of the loop was then washed briefly in a 10% bleach solution, rinsed in water then flamed before reusing.
Primary and nested-PCR reactions were optimized by testing 1.5, 2 and 3 mM MgCl2 in the reaction, each at 12 temperatures ranging from 45°C to 65°C using an Eppendorf Gradient Master Cycler. B. henselae and B. clarridgeiae strains used for template were a gift from Dr. Jill Clarridge. Optimized PCR cycle conditions were 94°C -15 s, 48.2°C -30 s and 72°C -30 s for 40 cycles for the primary-PCR and 94°C -15 s, 56°C -30 s and 72°C -30 s for 40 cycles for the nested-PCR. The PCR strategy was an adaptation of a primary PCR described by Jensen et al., . Primary PCR primers were P-bhenfa (5'-TCTTCGTTTCTCTTTCTTCA) and P-benr1 (5'-CAAGCGCGCGCTCTAACC) which gave an approximately 186 bp fragment for B. henselae and a 168 bp fragment for B. clarridgeiae, and nested primers N-bhenf1a (5'-GATGATCCCAAGCCTTCTGGC) and N-bhenr (5'-AACCAACTGAGCTACAAGCC) which gave an approximately 152 bp fragment for B. henselae and a 134 bp fragment for B. clarridgeiae. The Internal Amplification Control (IAC) consisted of a DNA amplicon, randomly amplified from the genome of a chicken with primer IAC (5'-TGTTTGACAGCTTATCAT). All reactions were performed in a 25 μl volume as follows: Primary reaction (0.2 mM each dNTP, 0.5 pmoles/μl each P-bhenfa and P-benr1, 3 mM MgCl2 reaction buffer, 0.4 pmoles/μl primer IAC, 1 μl of IAC template stock (concentration unknown), 0.5 units Taq polymerase (Promega) and Nested (0.2 mM each dNTP, 0.5 pmoles/μl each N-bhenf1a and N-bhenr, 1.5 mM MgCl2 reaction buffer, 0.4 pmoles/μl primer IAC, 0.5 units Taq polymerase).
The B. clarridgeiae-specific PCR was performed using 1 μl of a primary reaction in a PCR reaction with primers bclarF (5'- GCACAAGCCTCTGAGAGGGA) and N-bhenr. Reactions were performed in a 25 μl volume as follows: Primary reaction (0.2 mM each dNTP, 0.5 pmoles/μl each primer, 3 mM MgCl2 reaction buffer, 0.5 units Taq polymerase). PCR cycle conditions were 94°C -15s, 55°C -30 s and 72°C -30 s for 40 cycles.
PCR amplification products were separated on either a 2% or 3% agarose gel, stained with ethidium bromide and visualized under 302 nm ultra-violet light. DNA markers were created by PCR amplification of virulence genes from Escherichia coli generating calculated-sized fragments (bp) of 881, 520, 337, 275 171 and relative sizes confirmed using a commercial DNA size standard (100 bp ladder, Promega).
One hundred microliters of blood was spread on a Brain Heart Infusion Agar plate (Difco) supplemented with 10% whole sheep blood and incubated for 2–3 weeks at 37°C in 5% CO2. In some cases the blood was frozen at -70°C before being cultured.
Amplification products generated in the nested reaction for B. henselae and B. clarridgeiae were electrophoresed through a 1% agarose gel. The agarose containing the amplified DNA was cut from the gel, briefly frozen then thawed and spun at 12,000 rpm through a polypropylene fibre to remove the DNA-containing liquid. The DNA was concentrated by ethanol precipitation and used in the sequencing reaction. An ABI Big Dye sequencing kit was used according to manufacturer's instructions using the nested primers individually in two separate reactions, and the reactions resolved on an ABI 377 DNA sequencing machine.
Bartonella species associated with living environments of cats
Blood cultures were generally contaminated with both spreading bacteria and fungi, to such a degree that it was felt that little meaningful data could be gained through culture, and it was discontinued.
As an emerging pathogen known for causing disease in both humans and animals, a simple test for the routine identification of Bartonella species is desirable. Because multiple Bartonella species are associated with disease in both humans and animals, it would be advantageous to have a test capable of both detecting different species and differentiating between them. The strategy first presented by Jensen et al.,  generally fits these requirements by targeting DNA-length heterogeneity in the 16S rDNA-23S rDNA intergenic region. As such, this test is well suited for the detection of B. henselae and B. clarridgeiae, the causative agents of CSD in humans. However, as a single PCR reaction, this test has questionable sensitivity and has in fact been reported to show less sensitivity than culture for the detection of B. henselae and B. clarridgeiae in blood, ; see also . Similarly, the primary reaction used in this study was unable to detect Bartonella DNA in any of the samples although we were able to show the presence of Bartonella DNA in 32 samples with a nested reaction. These results question the usefulness of a single PCR reaction for the detection of Bartonella in blood without further enhancing the overall sensitivity of the test, such as with the addition of a nested-PCR reaction. However, many laboratories are reluctant to use a nested reaction for fear that its high sensitivity will detect contaminating DNAs (mainly amplicons) and deliver a false-positive result. In this work, none of our negative controls were positive. To help control cross contamination, template preparation, assembly of the PCR reaction, nested reactions and gel electrophoresis were performed in different rooms. Especially useful was the use of a UV hood and a 1 μl urine loop instead of barrier tips to transfer an aliquot of the primary reaction to the nested reaction. By immersing the end of the loop, after each transfer, in a 10% bleach solution to chemically degrade any amplicons, and then rinsing with water before flaming, any chance splattering or aerosolization of DNAs from the loop during flaming was reduced.
The test of Jensen et al.,  also lacked an Internal Amplification Control (IAC) to detect PCR inhibition. In fact, arguments have been made for Internal Amplification Controls to be mandatory when describing diagnostic tests based on PCR . Since blood, which is a known source of PCR inhibitors, is a commonly used sample for Bartonella detection, it is important that PCR-based tests for Bartonella include an IAC. Individuals interested in evaluating this method may write the authors for an aliquot of the IAC template.
Because of the slow growth and long culture time for Bartonella, faster growing contaminating bacteria and fungi can overrun a culture plate and make the detection of Bartonella difficult or even impossible. Early in this study we found that the contamination problem was so severe that culture was discontinued. The unexpectedly high level of contamination may have originated from the blood collection process where blood was collected by both private veterinary clinics and veterinary students as part of their studies, and thus was not strictly controlled. Although perhaps undesirable for the purposes of this study, the uncontrolled nature of its collection perhaps more accurately represented blood as it would arrive to the laboratory for diagnosis, and underscores one advantage of PCR over culture for the detection of Bartonella.
Prevalence studies reported for Bartonella infection in cats are generally characterized by a relatively high prevalence of B. henselae compared to B. clarridgeiae [19–22]. In this study, our results were mostly consistent with other studies where B. henselae was detected in slightly more samples than B. clarridgeiae. However approximately 40% of the infected cats originated from an animal shelter, which were not necessarily representative of the cat population as a whole in Trinidad. For example, discounting the animals from the shelter, 7 (8.6%) animals were positive for B. henselae, 10 (12.3%) for B. clarridgeiae and 2 (2.5%) for both bacteria, suggesting that B. clarridgeiae may be found among pet cats at levels similar to, or even higher than that for B. henselae. As has been reported in other studies [21, 22], cases of mixed infections with both species were found. In addition, there was a clear relationship between cats expected to be exposed to fleas (e.g. stray cats at an animal shelter), and the prevalence of infection.
The usefulness of a single PCR for the detection of B. henselae and B. clarridgeiae in the blood of cats is questionable and enhancement methods, such as a nested-PCR, should be utilized. In Trinidad, B. henselae and B. clarridgeiae are found in cats and infection appears highest among stray cats, however B. clarridgeiae may be present at levels similar to, or higher than, that of B. henselae in pet cats.
We thank Dr. Jill Clarridge for providing us with strains of B. henselae and B. clarridgeiae and her helpful suggestions on the culture of these organisms from blood, and the DNA Unit at Mt. Hope Trinidad for assistance with DNA sequencing. We also acknowledge the financial support provided to DRA by a grant from the University of the West Indies' Research and Publication Committee (Grant# CRP.4Z).
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