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Journal of Clinical Microbiology, June 2000, p. 2389-2391, Vol. 38, No. 6
Department of Infectious
Diseases1 and Laboratory of
Parasitology,2 Hôpital Saint-Louis, Paris,
France
Received 30 December 1999/Returned for modification 26 February
2000/Accepted 25 March 2000
The ribosomal DNA internal transcribed spacer sequences of 13 unrelated Encephalitozoon intestinalis isolates obtained
from human immunodeficiency virus (HIV)-infected patients with
intestinal microsporidiosis were analyzed by gene amplification and DNA
sequencing. Among these isolates, we found only one genetic lineage
which suggests that E. intestinalis may have a clonal
distribution in HIV-infected patients.
In recent years, microsporidia have
emerged as important opportunistic parasites in human immunodeficiency
virus (HIV)-infected patients. Encephalitozoon intestinalis
is the second most prevalent microsporidian species infecting humans
(10, 21). This intestinal parasite is the cause of severe
diarrheal illness and disseminated infections in HIV-infected patients
(9, 16). Recent studies have also identified this pathogen
in immunocompetent individuals (8, 18, 20). Humans remained
the only recognized host of this agent until 1998, when Bornay-Llinares
and colleagues described E. intestinalis from a variety of
mammals (donkey, pig, dog, cow, and goat) in Mexico, suggesting the
possibility that E. intestinalis infection is zoonotic in
origin (1). In addition, this agent has recently been found
in water, indicating that this human-pathogenic microsporidian
may also be a waterborne pathogen (7). The epidemiology of
E. intestinalis remains, however, poorly understood. To help elucidate the epidemiology of E. intestinalis, we wished to
study the genetic diversity of E. intestinalis strains by
analyzing the internal transcribed spacer (ITS) sequences of their
ribosomal DNAs (rDNAs). This approach has proven successful in defining the genotype diversity within three microsporidian species in humans
(Encephalitozoon cuniculi, Enterocytozoon
bieneusi, and Encephalitozoon hellem) based on
variation in the ITS sequences of their rDNAs and has helped us to
study their zoonotic potential (4, 5, 11, 13, 14, 15, 19).
In this report, we used 13 stool specimens obtained over a 5-year
period (1994 to 1998) from 13 unrelated HIV-infected patients with
E. intestinalis seen in Paris, France (16, 17).
Species-level identification of E. intestinalis was made by
PCR with DNAs extracted from stools (n = 13) using a
specific primer set of E. intestinalis small-subunit rDNAs
as previously described (12). In this study, microsporidian
DNAs were extracted from stored stool samples in potassium dichromate
with a High Pure PCR Template Preparation kit (Boerhringer Mannheim,
Meylan, France) by following the manufacturer's protocol for isolation
of nucleic acids from yeast. Primers for PCR were chosen to amplify a
237-bp fragment that includes a portion of the small-subunit rDNA (107 bp), the entire ITS region (28 bp), and a segment of the large-subunit
rDNA (102 bp). These primers do not amplify rDNA from E. cuniculi, E. hellem, or E. bieneusi. The
forward primer EL1 (5'-CTA AGA TGA CGC AGT GGA CG-3'), complementary to
positions 1 to 20, was designed by using the GenBank sequence of
E. intestinalis (accession no. Y11611). The reverse primer EL2 (5'-CCC CAA GCG CTT CCG CTT CA-3') was designed to be complementary to positions 218 to 237 of the GenBank sequence of E. intestinalis (accession no. Y11611). Amplification was done in a
50-µl reaction mixture including 2.5 µg of each primer/ml, 200 µmol of each deoxynucleoside triphosphate/liter, 75 mmol of Tris-HCl
(pH 9.0)/liter, 20 mmol of
(NH4)2SO4/liter, 0.01% Tween 20, 2 mmol of MgCl2/liter, and 2 U of Taq DNA
polymerase (Goldstar; Eurogentec, Seraing, Belgium). After a
denaturation of the DNA at 94°C for 10 mn, 40 cycles were run with a
Hybaid (Teddington, Middlesex, United Kingdom) touchdown apparatus as
follows: denaturation at 94°C for 30 s, annealing at 55°C for
30 s, and elongation at 72°C for 30 s. A 10-min extension at 72°C was used after the 40 cycles. To detect inhibition of the
amplification reactions, two different volumes of each DNA preparation
were tested: 10 µl of the initial extract and a 10-fold dilution of
released DNA. All positive samples were independently examined twice
(DNA extraction and amplification). Each set of reaction mixtures
included a negative control to ensure the absence of contamination of
samples during analysis and a positive control represented by culture
spores of E. intestinalis. To assess genetic diversity, DNA
sequencing of amplified products was performed by automated means (ABI
PRISM 377 system; Perkin-Elmer, Courtaboeuf, France). Both strands were
sequenced with the primers used for the PCR. Sequences were edited with
the Sequence Navigator (Perkin-Elmer) program and aligned using the
Multalin program (2).
Using the DNA isolates as templates, amplified bands with primer set
EL1-EL2 were of the expected size (237 bp) (Fig.
1). For five (38%) stool specimens,
however, a 10-fold dilution of released DNA was necessary to remove PCR
inhibitors (data not shown). The sequences of all PCR products were
100% identical with the corresponding published sequence of an
E. intestinalis isolate (GenBank accession no. Y11611)
(Table 1). This result suggests that all
13 isolates belong to the same genetic lineage.
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Copyright © 2000, American Society for Microbiology. All rights reserved.
Genetic Homology among Thirteen
Encephalitozoon intestinalis Isolates Obtained from Human
Immunodeficiency Virus-Infected Patients with Intestinal
Microsporidiosis
ABSTRACT
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TABLE 1.
Alignment of the rDNA ITS sequences of
Encephalitozoon species
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FIG. 1.
Agarose gel analysis of PCR-amplified products using
species-specific primers (EL1 and EL2) for E. intestinalis.
Lanes: M, 100-bp DNA size marker; 1 and 17, positive controls; 2 and
16, negative controls; 3 to 15, stool specimens infected with E. intestinalis.
Previous studies showed that the ITS sequence was a main target for identifying gene polymorphism of microsporidia. For the two species E. cuniculi and E. hellem, a set of tetranucleotide repeats (5'-GTTT-3') in the ITS has been found to vary among isolates from different hosts, resulting in the definition of three different genotypes for these parasites (Table 1) (5, 15). Also, heterogeneity in the ITS region has been described for E. bieneusi isolates. The heterogeneity is due to nucleotide substitutions in the ITS sequence, generating four distinct ITS types (11).
Although genetic homology between E. intestinalis isolates suggests that there is a possibility that all 13 patients contracted their infections from a common source, this possibility seems unlikely since the material was collected from the patients over a 5-year period and since the patients lived in different geographic areas. Our results are in agreement with those of two previous studies which examined the potential diversity of E. intestinalis isolates. In the first study, Del Aguila and colleagues showed at the antigenic level that eight isolates from five unrelated HIV-infected patients had very similar antigenic profiles by Western blotting (3). In the second study, three E. intestinalis isolates from two HIV-infected patients were analyzed (6). We determined that the ITS sequences of these isolates shared identical DNA sequences with our 13 isolates. This result reinforces the hypothesis of a clonal distribution of E. intestinalis in HIV-infected patients. However, this hypothesis needs to be extended to a larger number of E. intestinalis isolates, including those from other human, animal, and environmental sources, in order to better understand the epidemiology of E. intestinalis infection.
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ACKNOWLEDGMENTS |
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We acknowledge SIDACTION (Fondation pour la Recherche Médicale) and the Centre d'Etudes et de Recherche en Infectiologie for their financial support.
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FOOTNOTES |
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* Corresponding author. Mailing address: Clinique des Maladies Infectieuses, Hôpital Saint-Louis, 1 avenue C. Vellefaux, 75475 Paris Cedex 10, France. Phone: (33) 1 42 49 90 66. Fax: (33) 1 42 49 90 67. E-mail: molina{at}chu-stlouis.fr.
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Journal of Clinical Microbiology, June 2000, p. 2389-2391, Vol. 38, No. 6
0095-1137/00/$04.00+0
Copyright © 2000, American Society for Microbiology. All rights reserved.
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