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BMC Infectious Diseases

, 19:98 | Cite as

Leishmania cytochrome b gene sequence polymorphisms in southern Iran: relationships with different cutaneous clinical manifestations

  • Iraj MohammadpourEmail author
  • Gholam Reza Hatam
  • Farhad Handjani
  • Farzaneh Bozorg-Ghalati
  • Daniel PourKamal
  • Mohammad Hossein MotazedianEmail author
Open Access
Research article
  • 190 Downloads
Part of the following topical collections:
  1. Parasitological diseases

Abstract

Background

Cutaneous leishmaniasis (CL) caused by Leishmania species, is a geographically extensive disease that infects humans and animals. CL is endemic in half of the 31 provinces of Iran, with 29,201 incidence cases reported in Fars province from 2010 to 2015. CL is polymorphic and may result in lesions characterized by different clinical features. Parasite genetic diversity is proposed to be one of the factors affecting the clinical outcome and lesion characteristics in CL patients. However, there is still very limited data regarding the genetic variation of Leishmania spp. based on the sequencing of Cytochrome b (Cyt b) gene.

Methods

All patients originated from endemic regions in Fars province. The amplification of the Cyt b gene from isolates of 100 patients with disparate clinical forms of CL was accomplished using Nested-PCR. Sequence analysis of the amplified Cyt b was used to scrutinize the genetic variations among Leishmania isolates and connect the results with clinical pictures. The clinical demonstrations were basically of two types, typical and atypical lesions. Molecular phylogenetic tree was constructed using the Neighbor-Joining method, with species/strains from this study compared to species/strains from other geographical regions.

Results

Leishmania major was identified as the predominant infecting Leishmania spp. (86% of cases), with the remainder of cases being infected by Leishmania tropica. Clinical examination of patients revealed 12 different clinical CL forms. Among Leishmania samples analyzed, five distinct haplotypes were recognized: three in L. major and two in L. tropica. We found a correlation between clinical outcomes and Cyt b sequence variation of Leishmania spp. involved. Moreover, we observed a higher presence of polymorphisms in L. major compared with L. tropica. This difference may be due to the different eco-epidemiologies of both species, with L. tropica being an anthroponosis compared to L. major, which is a zoonosis.

Conclusions

The sequence analysis of Cyt b gene from 25 L. major and L. tropica strains demonstrated genetic variability of L. major and L. tropica causing CL in southern Iran, and a feasible connection amid the genetic heterogeneity of the parasite, geographical source and clinical appearance of the disease in human was detected.

Keywords

Leishmania Minicircle kDNA Cytochrome b (Cyt b) Sequencing Phylogenetic analysis Iran 

Abbreviations

7SL

7 Splicing Leader

A

Adenine

Arg

Arginine

C

Cytosine

CL

Cutaneous leishmaniasis

Cys

Cysteine

Cyt b

Cytochrome b

FCS

Fetal Calf Serum

G

Guanine

GP63

Glycoprotein 63

HSP

Heat Shock Protein

IFN-γ

Interferon γ

Ile

Isoleucine

ITS

Internal Transcribed Spacer

kDNA

kinetoplast DNA

Leu

Leucine

MLEE

Multi-locus enzyme electrophoresis

NJ

Neighbor-Joining

PBS

Phosphate Buffered Saline

Pfu

Pyrococcus furiosus

Phe

Phenylalanine

SNP

Single Nucleotide Polymorphism

T

Thymine

Thr

Threonine

TNF

Tumor Necrosis Factor

Trp

Tryptophan

Tyr

Tyrosine

Background

Cutaneous leishmaniasis (CL), is a vector-borne zoonotic infectious disease caused by protozoan parasites of the genus Leishmania (Kinetoplastida, Trypanosomatidae) [1, 2]. It is transferred to humans through the bite of infected female phlebotomine sand flies of the genera Phlebotomus and Lutzomyia [3]. CL can cause by 21 Leishmania spp. and result in a wide spectrum of clinical manifestations in humans, with the infecting species being a great determinant of clinical outcome [4]. Contingent upon the species of Leishmania involved, humans and a large spectrum of mammals operate as reservoirs [5]. The disease is endemic in the tropical and subtropical regions of 98 countries across four continents. More than two thirds of new cases of CL transpire in six countries: Afghanistan, Algeria, Brazil, Colombia, Iran and Syria. An estimated of 0.7–1.3 million new cases occur worldwide annually [4, 6]. In Iran CL is caused by Leishmania tropica, (the agent for anthroponotic CL), Leishmania major (the agent of zoonotic CL), and rarely by Leishmania infantum [7, 8, 9]. In addition, it is common for different species to coexist in the same endemic areas, as seen in Fars province [7, 8, 9]. Single or multiple CL lesions typically occur on exposed parts of the body, such as face, and upper and lower extremities. Lesions usually self-heal in a few months, but may persist for many years (e.g. when super-infected or when located on joints), causing considerable morbidity and large scars [10].

There have been several reports from studies in Iran of atypical manifestations of the disease due to either uncommon sites of lesions or their unusual morphology. Lesions on atypical sites result in a more complex differential diagnosis [7, 8]. Uncommon clinical presentations include lupoid, verrucous, sporotrichoid, erysipeloid, eczematous, psoriasiform, zosteriform, keloidal, whitlow, paronychia, carcinoma-like, and midfacial destructive lesions [7, 8, 10, 11, 12]. Occasionally CL may manifest as isolated lymphadenopathy, or proceed into disseminated CL [13, 14].

The genetic heterogeneity may cause various phenotypes that manifest themselves in the variability of clinical features observed. Therefore, bestowed genetic variations in Leishmania populations, disease control and treatment could be challenging [15]. Multi-locus enzyme electrophoresis (MLEE) has traditionally been the gold standard for strain and species characterization [16, 17]. However, this customary classification has been challenged using nuclear and mitochondrial molecular markers, as they inclined to be more specific and stable [18]. Generally, DNA analysis demands reiterated copying of the genome, and the levels of inter- and intra-species diversity has to be taken into account. In order to appraise genetic characterization, a number of nuclear and extra nuclear DNA markers have been employed, including kDNA [19], GP63 [20], ITS1 [21], ITS2 [22], the N-acetylglucosamine-1-phosphate transferase gene [23], Cytochrome Oxidase II [24], Cytochrome b (Cyt b) [25], Miniexon [26], 7SL RNA [27], HSP70 [28], and Cysteine Proteinase B [29].

The mitochondrial genome has been disclosed to be a splendid origin of accessible genetic variation. Analysis of mitochondrial DNA has been used to understand the evolutionary biology at the inter- and intra-species levels [30, 31]. Mitochondrial DNA’s rapid rate of evolution, clonal patrimony, and absence of recombination makes it an ideal target for phylogenetic studies and a source of genetic markers of species and geographically confined populations [30, 31]. Mitochondrial kinetoplastid DNA (kDNA), arranged as mini and maxicircles, encodes proteins involved in energy production and ribosomal RNAs. Minicircles are about 800-bp in size, closely 600-bp variable and 200-bp conserved region, and repeated 10,000 times. Maxicircles are around 20–35 kb in size, and have 20–50 repetitions in the genome [30, 31]. The mitochondrial genome can encode gene products such as Cyt b in the cellular respiration cycle [32]. Cyt b is the principal redox catalytic subunit of Quinol, which is engaged in the electron transport process of the mitochondrial respiratory chain, and is regarded one of the most functional genes for phylogenetic studies [32, 33, 34].

In the present study, the sequence analysis of the amplified Cyt b gene was applied to investigate the presence of genetic polymorphisms among Leishmania isolates and correlate the findings with the clinical features of CL lesions in Fars province, Iran, over a 2-year period. Moreover, molecular phylogenetic relationships were assessed using Cyt b gene sequences obtained by this study and download from the GenBank database.

Methods

Ethics statement

The research protocol was endorsed (approval no. 94–7548) by the Institutional Ethics Clearance Committee (IECC) of Shiraz University of Medical Sciences and performed in accordance with international policies established by the Declaration of Helsinki.

Written informed consent

Written informed consent (Code: IR.SUMS.REC.1394.S282) to participate in the study and use clinical images in publications was obtained from all adult patients and/or parents/legal guardians for children under the age of 16 years.

Patients

One hundred patients who showed different types of CL lesions participated in this study. The patients were referred to the Dermatology Clinic of Saadi Hospital and Fajr Health Center from January 2015 to the end of December 2016. Selected patient lesions (the most recent, in case of multiple lesions) were first photographed and standard clinical descriptions for these lesions were obtained from the attending dermatologist. All patients originated from different rural and urban regions of Fars province. We excluded patients with clinical evidence of intercurrent bacterial or fungal superinfection of the ulcer, and those undergoing active treatment for CL. For each patient a structured questionnaire was completed with all demographic information about the patient (including code, age, sex, address, and travel history), the lesion (including the number of lesions, localizations, onset of the disease, and clinical characteristics), and therapeutic data. The questionnaire used in our study, was designed and developed for this study.

Dermal scraping

For the margin dermal scraping, a deep disinfecting of the indurated active margin of the lesion with 70% ethanol was performed. Samples were taken by using a no. 15 disposable sterile surgical blade (Unicut, Chicago, IL, USA) to make an incision in the border of the lesion. Exudates and dermal tissues from the wall of the slit were scraped and smeared on two glass slides [7, 8]. The touch impression smears were air dried, methanol-fixed, stained with Giemsa (Merck, Darmstadt, Germany), and finally examined for amastigotes by microscopy.

In vitro culture

Moreover, the dermal syringe-sucked fluid was collected under sterile conditions from each patient as follows: 0.1 mL of sterile saline solution was injected using an insulin syringe (1-mL, 25-gauge needle) into the nodule and the needle was rotated gently several times. A small amount of saline solution was injected into the tissue, and then aspirated. The fluid was transferred to two tubes of modified NNN culture medium. Modified NNN medium was biphasic, comprise of horse blood agar base and an overlay Locke’s solution [7, 8]. The specimens were inoculated into the medium and incubated at 25 °C. Every 2 to 3 days, the liquid phases of cultures examined under invert microscope, in order to observe motile promastigotes. Positive cultures were mass cultivated in RPMI-1640 medium (Gibco, Frankfurt, Germany) supplemented with 15% heat-inactivated Fetal Calf Serum (Gibco, Frankfurt, Germany), 2 mM L-glutamine, 100 U/mL Penicillin, and 100 μg/mL Streptomycin (Gibco, Frankfurt, Germany) [7, 8]. Nearly 2 × 106 promastigotes were harvested by centrifugation (10,000 g for 10 min) and washed thrice in cold sterile PBS (pH 7.2). Parasites pellets were stored at − 20 °C until used.

DNA extraction

Total genomic DNA was extracted from each clinical sample using the QIAamp® DNA Mini Kit (QIAGEN, Hilden, Germany), according to manufacturer’s instructions. Following the centrifugation and washing steps, the DNA was eluted from the silica spin columns with 50-μL elution buffer to increase its concentration. The quantity and quality of the extracted DNA was determined by measuring optical absorbance at 260 nm using a Nano spectrophotometer (NanoDrop® 2000, Thermo Fisher Scientific, Wilmington, DE, USA). Each samples for PCR assays were prepared with aerosol-guard pipette tips to avoid contamination. All reactions were performed in appropriated places, following the good practice of laboratories to avoid sample contamination [7, 8]. The extracted DNA was stored at − 20 °C until used.

kDNA semi-nested PCR

All samples (cultures and impression smears) were identified to Leishmania species level using kDNA primers before they were subjected to Cyt b amplification.

The conserved area of the minicircle kDNA from the Leishmania species of all the samples was amplified by semi-nested PCR using primers LINR4 (forward) (5′-GGG GTT GGT GTA AAA TAG GG-3′), LIN17 (reverse) (5′-TTT GAA CGG GAT TTC TG-3′), and LIN19 (reverse) (5’-CAG AAC GCC CCT ACC CG-3′) for species identification [7, 8, 35].

PCR was performed in a Bio-Rad MyCycler Thermocycler (Hyland Scientific, Stanwood, WA, USA). The PCR conditions were composed of pre-denaturation at 94 °C for 5 min, then 40 cycles of denaturation at 94 °C for 30 s, annealing at 52 °C (LINR4 and LIN17) or 58 °C (LINR4 and LIN19) for 45 s, and extension at 72 °C for 1 min, followed by final extension at 72 °C for 10 min. Amplicons were analyzed on 1.5% agarose gels (AddGene, Watertown, MA, USA) by electrophoresis at 90 V in 1 × TAE buffer (40 mM Tris-acetate and 1 mM EDTA, pH 8.3) and visualized by UV light (Uvitec, Cambridge, UK) after being stained with GelRed® (Biotium, Hayward, CA, USA). Cross-contamination was monitored by negative controls for sample extraction and PCR solutions.

Cyt b nested-PCR

Maxicircle Cyt b gene was amplified using nested-PCR. Nest 1 primers corresponded to COIIIF (5′ - GTT TAT ATT GAC ATT TTG TAG ATT - 3′) and MURF4R (5′ - CGA CGA ATC TCT CTC TCC CTT - 3′). Nest 2 primers matched to LCBF1 (5′ - GGT GTA GGT TTT AGT TTA GG - 3′) and LCBR2 (5′ - CTA CAA TAA ACA AAT CAT AAT ATA CAA TT - 3′) [34].

The partial region of the Cyt b gene was amplified with Pfu DNA Polymerase (Agilent Technologies, Santa Clara, CA, USA) under the following conditions: initial denaturation at 94 °C for 5 min, followed by 40 cycles, each consisting of 30 s at 94 °C, 45 s at 58 °C (COIIIF and MURF4R) or 50 °C (LCBF1 and LCBR2), 1 min at 72 °C, and a final extension at 72 °C for 10 min. Electrophoresis and visualizing were performed under the same conditions as described above.

Roche Molecular Diagnostics Laboratories (Roche, Penzberg, Germany) synthesized all primers.

Reference strains of L. major (MHOM/IR/54/LV39) and L. tropica (MHOM/IR/89/ARD-L2) were used as positive controls.

Sequencing

The amplified DNA fragments of both kDNA and Cyt b genes were visualized on 1.5% agarose gels, parallel with standard DNA marker (Fermentas, Vilnius, Lithuania) to permit sizing. The PCR products were extracted from gel sections using the QIAquick® Gel Extraction Kit (QIAGEN, Hilden, Germany).

Sequencing of 200 ng of the amplified kDNA gene products were accomplished by using the LINR4 and LIN19 primers. Direct sequencing was performed to bridge gaps in nucleotide sequences.

Sequencing of the amplified Cyt b gene products were executed by using Nest 2 primers (LCBF1, LCBR2) and two specific internal primers LCBF4 (5′ – TGT TAT TGA ATA TGA GGT AGT G - 3′) and LCBR4 (5′ – GAA CTC ATA AAA TAA TGT AAA CAA AA - 3′). DNA sequencing was carried out on an ABI PRISM® 3730xl Genetic Analyzer (Applied Biosystems, Foster City, CA, USA) by the Sanger dideoxy chain termination method using the Big Dye Terminator Cycle Sequencing Ready Reaction Kit (Applied Biosystems, Foster City, CA, USA). Sequence accuracy was confirmed by sequencing both directions through the sequencing service of Roche Molecular Diagnostics (Roche, Mannheim, Germany). Special attention was paid to the double peaks and the accurate direction of the sequences was guaranteed. The variations between and within Leishmania species, and the number of different nucleotides in each sequence was determined.

Phylogenetic analysis

The raw nucleotide sequences and chromatograms of both forward and reverse directions were viewed and analyzed using the Chromas (2.6.6) program. The nucleotide sequences were aligned and analyzed using the MUSCLE multiple sequence alignment program [36]. Consensus sequences were compared with homologous sequences in the GenBank database using the BLAST algorithm [37]. The sequences were assembled and edited with the BioEdit (7.2.6) to identify single nucleotide polymorphisms (SNPs) [38]. Multiple alignments were performed with data related to Leishmania species from Iran and other countries deposited in GenBank. The parasite species were confirmed based on the homology with kDNA and Cyt b genes sequences from Leishmania reference strains. A molecular phylogenetic tree was constructed by the Neighbor-Joining (NJ) method and genetic distances were calculated with Maximum Composite Likelihood model using MEGA-X [39]. The reliability of the NJ tree was assessed by the bootstrap method with 1000 replications. Leishmania equatorensis was treated as out-group in Cyt b phylogenetic analysis.

Statistical analysis

The Fisher’s Exact Test was used for analyzing the relation between clinical features and Leishmania species involved. All statistical analyses were performed using SPSS (SPSS 24.0, Chicago, IL, USA). A P-value < 0.05 was considered statistically significant.

Nucleotide sequence accession numbers

The partial sequences of the Cyt b gene obtained in this study were deposited in the GenBank database under accession numbers KX176846, KY290231, KY360312-KY360314.

Results

Clinical results

From clinical standpoint, 58 out of 100 patients surmised to have CL were male. The patients were part of an incongruous population in Fars province, Iran. Their ages sorted from 0.7 to 89 years. The period of the cutaneous lesion fluctuated between 2 weeks to 2 years.

The relative distribution of Leishmania species in Fars province was shown to be heterogeneous. The majority of CL was due to L. major (86% of all cases), with the remainder due to L. tropica. While L. major was isolated from patients originating throughout Fars province, L. tropica was exclusively isolated from patients originating from the city of Shiraz (14% of L. tropica isolates reported).

Lesions were categorized into three main typical and nine atypical forms according to the clinical features. Three main types categorized as follows: 1- Elevated erythematous lesions smaller than 0.5 cm in diameter were defined as papular. 2- Elevated deeply seated erythematous lesions larger than 0.5 cm were elucidated as nodular. 3- Erythematous elevated lesions larger than 1 cm in diameter with ulcer were illustrated as ulcerative plaque. The majority of the patients had lesions over exposed parts of the body, most commonly hands and arms, followed by legs, face, and trunk. Sixty-six patients had one lesion, 19 patients had two lesions, and 15 patients had three or more lesions. The clinical features of the patients are summarized in Table 1.
Table 1

Clinical presentations in patients with cutaneous leishmaniasis

Clinical Patterns

No.

Location

Sex

Duration

Nodular

21

upper and lower extremities, Lip, Trunk, Neck

M and F

2 weeks-7 months

Ulcerative Plaque

19

upper and lower extremities, Face

M and F

3 weeks-2 years

Hyperkeratotic

19

upper and lower extremities, Face, Neck, Nose

M and F

3 weeks-10 months

Erythematous

9

upper and lower extremities, Face

M and F

3 weeks-5 months

Eczematous

9

upper and lower extremities, Face, Neck

M and F

5 weeks-8 months

Volcanic

8

upper and lower extremities

M and F

5 weeks-7 months

Multi-Lesional

5

upper and lower extremities, Trunk

M and F

3–6 months

Verrucous

4

Foot, Forehead

F

2–6 months

Papular

2

Hand, Finger

M and F

4 months

Psoriasiform

2

Hand, Ear

M and F

3–5 months

Carcinoma-Like

1

Eyelid

F

5 months

Recidivans Type (Lupoid)

1

Wrist

F

15 months

The most common clinical presentation was nodular CL with 21 patients, followed by ulcerative plaque 19, hyperkeratotic 19, erythematous 9, eczematous 9, volcanic 8, multi-lesional 5, verrucous 4, psoriasiform 2, papular 2, carcinoma-like 1 [7, 8], and 1 recidivans-type (lupoid) (Fig. 1a-j). Numerous intracellular and scattered extracellular amastigotes were observed microscopically. Employing Giemsa, amastigotes are seen within the cytoplasm of macrophages as pale blue oval bodies with a dark blue nucleus and a small rod-shaped kinetoplast with a specified mitochondrial frame that contains extra-nuclear DNA (Fig. 2). CL was confirmed by microscopic examination of smears in 80% of 100 patients.
Fig. 1

Clinical presentations of CL lesions caused by L. tropica and L. major: (a) Hyperkeratotic; (b) Multi-Lesional; (c) Erythematous; (d) Eczematous; (e) Psoriasiform; (f) Verrucous; (g) Discoid Lupus-Like; (h) Paronychia, Eczematous, and Hyperkeratotic; (i) Erythemato-Ulcerative; and (j) Wet Ulcerative Plaque

Fig. 2

Touch impression smear. Numerous intracellular and scattered extracellular amastigotes are present (Giemsa stain; original magnification, × 1000). Kinetoplasts are visible in many amastigotes

Molecular, sequencing, and phylogenetic analysis findings

Semi-nested PCR was accomplished for amplification of the conserved area of the minicircle kDNA from the Leishmania spp. A 650-bp fragment was amplified for L. major, while a 760-bp fragment was amplified for L. tropica (Fig. 3). All 100 samples were sequenced for kDNA gene. The kDNA sequence analysis showed 14 cases of L. tropica and 86 cases of L. major.
Fig. 3

Electrophoresis of PCR products of DNA extracted from positive smears and cultures. The 8 lanes contained the products from positive controls of L. tropica (lane 6) and L. major (lane 7), negative control (lane 5), cutaneous lesions due to L. major and L. tropica (lanes 1–4), and a molecular marker (MM)

Nested-PCR was executed for amplification of estimated size of 866-bp fragment of the internal Cyt b region in the second PCR reaction (Fig. 4). In this study, many of the 100 patients had similar skin lesions in size and clinical picture. Thus, 25 CL patients with various size lesions and different clinical outcomes were randomly selected and fully characterized for Cyt b gene sequencing. The resulting sequences of Cyt b gene were aligned and compared with those of existing sequences related to Leishmania in GenBank. The achieved sequences confirmed the presence of L. major and L. tropica that were recognized by the kDNA sequence analysis.
Fig. 4

PCR result of Leishmania spp. isolated from CL lesions. The PCR product size is approximately 866 bp. The 8 lanes contained the products from positive controls of L. tropica (lane 4) and L. major (lane 5), negative control (lane 6), cutaneous lesions due to L. major and L. tropica (lanes 1–3), and molecular marker (MM)

In this study, two different strains of L. major (MRHO/IR/75/ER and MHOM/SU/73/5ASKH) and one strain of L. tropica (MHOM/SU/74/K27) were detected in Fars province, Iran. The Cyt b sequence analysis of 25 CL patients showed a 99–100% similarity to the previously published strains of Leishmania spp. The sequences of L. major patients with accession number KX176846 showed 99% identity to the published strains MRHO/IR/75/ER, and HU64, Abrkouh/Iran (KU680828 and KU680829). The sequences of L. major patients with accession number KY360312 showed 100% identity to the published strain MHOM/SU/73/5ASKH (EU140338, EF579898, and AB095961). Also, these isolates showed 99% identity to the published KU680827. The sequences of L. major patients with accession number KY360313 showed 100% identity to the published strain MRHO/IR/75/ER (KU680828). Also, these isolates showed 99% identity to the published strain HU64, Abrkouh/Iran (KU680829). The sequences of L. tropica with accession number KY360314 showed 100% identity to the published strain MHOM/SU/74/K27 (KU680831, HQ908270, and EF579904). Furthermore, the sequences of L. tropica with accession number KY290231 showed 99% identity to the published strain MHOM/SU/74/K27 (EF579904, HQ908270, and KU680831) (Fig. 5).
Fig. 5

Molecular phylogenetic relationship among various Leishmania isolates to each other as inferred by Neighbor-Joining tree based on Cyt b gene. Numbers on branches are percentage bootstrap values of 1000 replicates. The evolutionary distances between sequences were computed using the Maximum Composite Likelihood method. The scale bar indicates an evolutionary distance of 0.01 nucleotides per position in the sequence. The reference sequences accession numbers are inserted. Evolutionary analyses were conducted in MEGA-X

The common term of haplotype is a specific group of mutations or a collection of SNPs in the orthologous gene of the parasite. In this study, the haplotype diversity of Cyt b gene was observed to be higher in L. major population. Three haplotypes of Cyt b polymorphism of L. major were identified. In the sequencing result of L. major haplotype II (KX176846), thymine (T) is replaced by cytosine (C) at nucleotide position 258, C is replaced by T at nucleotide positions 394 and 801, and T is replaced by adenine (A) at nucleotide position 813. Alignment of the amino acid sequence corresponding to the non-edited region of haplotype II revealed Phe → Tyr substitution. Haplotype II was observed in the psoriasiform, and eczematous lesions.

In L. major haplotype III (KY360313), T is replaced by C at nucleotide position 280, C is replaced by T at nucleotide position 416, and T is replaced by A at nucleotide position 839. Alignment of the amino acid sequence corresponding to the non-edited region of haplotype III revealed two amino acid substitutions: One Trp → Arg substitution, and one Thr → Ile substitution. Haplotype III was principally observed in the carcinoma-like lesions.

Moreover, in L. tropica (KY290231), T is replaced by G at nucleotide position 810, and conversely at nucleotide position 811. Alignment of the amino acid sequence corresponding to the non-edited region of L. tropica (KY290231) revealed Leu → Cys substitution. This haplotype was essentially observed in the LR (lupoid) lesions. All variations occurred in microsatellite regions and were due to SNPs. In Fig. 5, the partial sequences of five haplotypes obtained in this study and deposited in the GenBank database, were analyzed.

The tree based on the classification of lesions grouped the 25 genotypes into 7 clusters (Fig. 6). Cluster I contained isolated strains from the verrucous, volcanic, and psoriasiform variants of CL patients who came from the same geographical region (isolates 27, 34, 50, 52, and 87). Cluster II included isolated strains from the erysipeloid and eczematous variants of CL patients who came from the same geographical origin (isolates 29, 37, 54, and 91). Cluster III comprised isolated strain from the ulcerative plaque of CL patients who came from the same geographical source (isolates 64, 71, and 75). Cluster IV embraced isolated strains from the hyperkeratotic variants of CL patients who came from the same geographical region (isolates 28, 30, and 59). Cluster V combined isolated strains from the erythematous variant of CL patients who came from the same geographical zone (isolates 9, 10, and 31). Cluster VI incorporated isolated strain from the carcinoma-like of CL (isolate 24). Withal, Cluster VII hugged isolated strains from the LR, papular, nodular, and multi-lesional variants of CL patients who came from the same geographical area (isolates 15, 20, 26, 49, 60, and 96). In Fig. 6, raw sequencing data of 25 Cyt b sequenced CL patients with different clinical pictures and sizes were used for phylogenetic consensus tree. The data shown in this phylogenetic consensus tree disclosed that those patients, who had the same clinical outcomes and came from the same geographical source, were infected with closely related strains of L. major in the phylogeny.
Fig. 6

A phylogenetic consensus tree between all Leishmania isolates using MEGA-X and clustering algorithms. L. infantum (AB095958), two L. major (AB095961, KU680828), and two L. tropica (EF579904, KU680831) were used as out-group and standard isolates, respectively

The analysis of the phylogenetic tree revealed two distinct clades: L. major and L. tropica. Within the clades intra-species divergence was more pronounced in L. major than in L. tropica. The Iranian strains of L. major and L. tropica found in this study were more similar to strains from the eastern and northern neighbor countries of Iran (Fig. 5).

Discussion

Cutaneous leishmaniasis is a polymorphic disease that can divulge distinctive clinical outcomes, and is characterized by skin lesions and ulcers on exposed parts of the body, departing perpetual scars. CL is allotted in greater than half of the 31 provinces of Iran, with 29,201 incidence cases reported in Fars province from 2010 to 2015 [40]. Fars province in southern Iran is a hyper-endemic region of CL [41]. Early identification and genetic characterization of causative agents of CL using Cyt b gene or other genetic markers has been avail for appraisal of Leishmania polymorphisms, since infected Leishmania species are confederated with the clinical presentation and drug susceptibility.

In this study, we used Cyt b gene sequencing to study genetic diversity among 100 Leishmania isolates from the different parts of Fars province, Iran and to correlate the genetic polymorphism of the parasite with the clinical manifestations of the disease in humans. One of the advantages about using gene sequencing is the understanding of the inter- and intra-species genetic diversity of Leishmania. Cyt b is situated in the maxicircle part of the kinetoplast that is about 50 copies. There is sufficient degree of nucleotide sequence change amid Leishmania spp. genomes for characterization and heterogeneity aims [34]. Recently sequencing of the Cyt b gene has been employed with prosperity for Leishmania sp. identification [33, 42, 43, 44, 45, 46, 47] and polymorphism [25, 34, 42, 43, 48, 49, 50]. Despite the low inter-species heterogeneity of the Cyt b gene, the key nucleotide positions depicted previously corroborate the potential of this gene as a molecular marker for Leishmania species characterization, not only in geographically related isolates, but also in widely separated regions [45].

The data from this study revealed genetic diversity of the Cyt b gene of Leishmania spp. isolated from a wide spectrum of clinical forms of CL in Fars province, Iran. This is in accordance with prior studies. Myint et al. [49] found three types of Cyt b polymorphism of L. major and no connection between clinical presentation and causal Leishmania parasites. Ramirez et al. [51] reported a high genetic diversity displayed by L. panamensis and L. braziliensis using Cyt b barcoding.

The genetic diversity of Leishmania spp. seen in academic research studies is dependent on a number of factors ranging from the parasite’s different eco-epidemiologies (e.g. are parasites isolated from humans, reservoir hosts or vectors; are they transmitted anthroponotically or zoonotically) to laboratory tools and molecular tools used (e.g. nuclear in contrast with mitochondrial DNA) [43]. Additionally, the occurrence of clonal reproduction and hybridization causes intrinsic genetic diversity in Leishmania [52, 53]. Of all these factors, sexual reproduction is the basic biological process that influences the population’s genetic structure. Many authors have reported evidence of hybrid formation and fortuitous bouts of genetic exchange or hybridization in Leishmania [54, 55, 56, 57]. Clearly, infrequent or rare sessions of sexual recombination in normally asexual parasites can have a deep effect on the range of genetic diversity. It has been informed that increased transmission potential and a new form of CL is the result of hybrid formation between L. major and L. infantum [56, 57].

A high degree of genetic polymorphisms in Leishmania parasites based on ITS1 and kDNA genes has been reported previously in Iran [58, 59, 60, 61, 62], and in the neighboring country of Afghanistan [63, 64]. In a preceding study by Baghaei, mutual connection between the genetic heterogeneity of L. major and clinical presentations of ZCL in Isfahan, Iran based on PCR-RFLP of ITS gene in the ribosomal operon, has been investigated [58]. His study revealed that L. major is genetically highly polymorphic and a correlation may exist between genetic heterogeneity of the parasite and the clinical picture of the disease in human. The PCR-RFLP of the RNA polymerase II largest subunit (RPOIILS) gene of L. major has divulged genetic diversity in Iran [65]. The genetic variability of L. major from Iranian isolates have been disclosed antecedently by Single-Strand Conformation Polymorphism PCR (SSCP-PCR) and sequence analysis of the ITS gene [60]. The Permissively Primed Intergenic Polymorphic-PCR (PPIP-PCR) displayed further genetic heterogeneity amid the clinical isolates of L. major causing CL in Isfahan, Iran [66]. Supplementally, the genetic polymorphism of the rDNA gene of L. major has been informed in Fars province, Iran [67].

In addition, substantial heterogeneity has been studied and reported within the ITS gene of strains of L. tropica [59, 64, 68, 69]. Oryan et al. [61] and Shirian et al. [62] assessed the heterogeneity of L. major causing CL based on sequencing of kDNA and showed a high genetic diversity of the parasite and correlations among the geographical origin and the clinical outcomes of the disease. Moreover, conspicuous genetic variability has been exhibited within the Nagt gene amidst L. tropica, L. major, and L. infantum strains [70, 71], and by RAPD-PCR among L. major and L. infantum strains [72, 73, 74]. Considerable genetic diversity was detected among L. major strains from different endemic areas and even between some isolates of the same endemic area in Iran using the RAPD technique [73]. The latter result might be elucidated by substantial “Gene Flow” among isolates belonging to the same area [75].

The findings of higher molecular diversity in L. major isolated from tropical and subtropical regions of the Fars province in this study rather than L. tropica from the Shiraz region could be related to the greater number of animal reservoirs and diversity of sand fly fauna encountered in these regions [3, 5, 41].

In this study, an intelligible correlation was discerned between the Cyt b gene sequence polymorphism of isolates and clinical pictures of skin lesions. This is in conformity with previous studies [42, 49, 50]. Our results disclosed noteworthy variations in the clinical features of the CL caused by L. major secluded from different geographical regions of Fars province, Iran. The CL typically demonstrates as papules, scaled-crusted nodules, and ulcerative plaques. However, it may sometimes pose in various atypical clinical outcomes such as sporotrichoid, erysipeloid, lupoid, keloidal, eczematous, erythematous, psoriasiform, zosteriform, chancriform, hyperkeratotic, verrucous, whitlow, paronychia, carcinoma-like and other atypical exhibitions [7, 8, 10, 11]. Coherent with these data, in a prior study, assessment of four L. major isolates collected from four different endemic areas in Iran displayed diverse clinical and immunological patterns in BALB/c mice [76]. The different clinical expressions of CL depend on both intra-species genetic diversity of Leishmania and host immune status. Compound lesions have been portrayed in connection to L. mexicana, L. braziliensis, L. tropica and L. major, the mentioned last leading to primarily dermotropic types. In similar circumstances, the disease disseminates from the initial lesion by way of the lymphatic vessels, presenting subcutaneous nodules or localized adenopathy that have a similar appearance to lymphocutaneous sporotrichosis [10, 11].

In addition to the intra-species genetic variability of the Leishmania, host immune reaction performs a significant function in the clinical presentation of CL. For example, patients with defect of the T cell reply frequently improve an anergic condition named diffuse CL characterized by multiple nodular lesions full of amastigotes. Moreover, host genetic inheritance and bacterial habitat are contributed to the outcome of CL [77, 78, 79, 80]. It has turned into limpid that the outcome of CL arises from an equilibrium between pro- and anti-inflammatory agents [81]. In CL patients, pathophysiology of disease is allied with a strong Th1 immune response to Leishmania antigens. Lesion dimension clearly connects with the immensity of Leishmania antigen- aroused TNF yield by peripheral blood mononuclear cells, and with the amount of flow TNF and IFN-γ producing CD4+ lymphocytes [82, 83]. Furthermore, there is an alliance between the strength of the inflammation and the frequency of CD8+ T cells exuding granzyme A [84].

Extra agents that have been asserted to affect the clinical outcome of CL comprise the place of inoculation, the total amount of the inoculated promastigotes, hormonal secretion quality, the quantity, quality and variety of food intake of the host, and the temperament of the final non-blood repast of the vector. Besides, agents like a non-native person, aged people communally, utilize of oral steroid drugs, immunodeficiency illnesses, and still lesion pollution with inorganic particles are able to modify the signs and symptoms of CL [85].

With relation to the effective causes of CL in Iran, the high usually recognized parasites were L. major and L. tropica, respectively. Dependent upon the results of this study, L. major is the supreme species liable for CL in this district. Three Leishmania spp. comprise of L. major, L. tropica, and sometimes L. infantum had been recognized as the causative agents of CL and ML collaborated with disparate clinical pictures in this territory [7, 8, 9]. The data procured in this study disclosed that those patients who had the similar clinical outcomes and came from the same geographical source were affected with almost linked strains of L. major in the phylogeny. Certain patients with various clinical configurations were situated in the equal bunch.

The established data from this study revealed that a correlation might be exist between the genetic variability of the parasite, clinical manifestation, and geographical source of the disease in humans. This is in agreement with previous studies [48, 49, 50].

Conclusions

The sequence analysis of the Leishmania Cyt b gene showed genetic polymorphisms in L. major and L. tropica and a feasible correlation among the genetic heterogeneity of the parasite, geographical source and clinical outcome of the disease in human was found. Furthermore, these data confirm and emphasize the usefulness of Cyt b gene sequencing on Leishmania spp. genetic polymorphism and phylogenetic relationship analysis. Based on our findings, we believe that different clones of parasites or mixed populations are circulating in endemic regions of Fars province, Iran. It is significant to contemplate that the clinical configuration of CL does not solely be contingent upon the Leishmania species involved. Meanwhile, even though certain lesion characteristics maybe more commonly associated with a particular species, one should not rely on clinical patterns to anticipate any species involvement.

Notes

Acknowledgements

The results described in this paper were a part of Ph.D. thesis of Iraj Mohammadpour.

Funding

This article was extracted in part from the thesis written by Iraj Mohammadpour as partial fulfillment of the requirements for obtaining his Ph.D. degree in the field of Medical Parasitology, which was funded supported by the office of Vice-Chancellor for Research of Shiraz University of Medical Sciences, Shiraz, Iran (Grant No. 94–7548). The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.

Availability of data and materials

The datasets generated and analyzed during the current study are not publicly available, because the personal information of the patients is confidential, but are available from the corresponding author on reasonable request.

Authors’ contributions

IM collected data, performed the molecular and phylogenetic analyses, and drafted the manuscript. FH typed the CL lesions, treated, and managed the patients at the clinical site and gave advice in drafting. IM, MHM, GRH, FBG, and DPK participated in interpretation and discussion. IM, MHM, GRH, and FBG finally approved the article. All authors read and approved the final manuscript.

Ethics approval and consent to participate

The research protocol was endorsed (approval no. 94–7548) by the Institutional Ethics Clearance Committee (IECC) of Shiraz University of Medical Sciences and performed in accordance with international policies established by the Declaration of Helsinki.

Consent for publication

Written informed consent (Code: IR.SUMS.REC.1394.S282) for use of clinical images in publications was obtained from all adult patients and/or parents/legal guardians for children under the age of 16 years. A copy of the written consent is available for review by the Editor of this journal.

Competing interests

The authors declare that they have no competing interests.

Publisher’s Note

Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

References

  1. 1.
    Steverding D. The history of leishmaniasis. Parasit Vectors. 2017;10:82.CrossRefGoogle Scholar
  2. 2.
    Akhoundi M, Kuhls K, Cannet A, Votypka J, Marty P, Delaunay P, Sereno D. A historical overview of the classification, evolution, and dispersion of Leishmania parasites and sandflies. PLoS Negl Trop Dis. 2016;10:e0004349.CrossRefGoogle Scholar
  3. 3.
    Davami MH, Motazedian MH, Kalantari M, Asgari Q, Badzohre A, Mohammadpour I. First microscopical and molecular-based characterization of Leishmania major within naturally infected Phlebotomus salehi (Diptera; Psychodidae) in Fars province, southern Iran. Ann Trop Med Parasitol. 2011;105:485–91.PubMedPubMedCentralGoogle Scholar
  4. 4.
    Alvar J, Velez ID, Bern C, Herrero M, Desjeux P, Cano J, Jannin J, den Boer M. Leishmaniasis worldwide and global estimates of its incidence. PLoS One. 2012;7:e35671.CrossRefGoogle Scholar
  5. 5.
    Davami MH, Motazedian MH, Kalantari M, Asgari Q, Mohammadpour I, Sotoodeh-Jahromi AR, Solhjoo K, Pourahmad M. Molecular survey on detection of leishmanial infection in rodent reservoirs in Jahrom district, southern Iran. J Arthropod Borne Dis. 2014;8:139–46.PubMedPubMedCentralGoogle Scholar
  6. 6.
    Palatnik-de-Sousa CB, Day MJ. One health: the global challenge of epidemic and endemic leishmaniasis. Parasit Vectors. 2011;4:197.CrossRefGoogle Scholar
  7. 7.
    Mohammadpour I, Motazedian MH, Handjani F, Hatam GR. Cutaneous leishmaniasis of the eyelids: a case series with molecular identification and literature review. Korean J Parasitol. 2016;54:787–92.CrossRefGoogle Scholar
  8. 8.
    Mohammadpour I, Motazedian MH, Handjani F, Hatam GR. Lip leishmaniasis: a case series with molecular identification and literature review. BMC Infect Dis. 2017;17:96.CrossRefGoogle Scholar
  9. 9.
    Shirian S, Oryan A, Hatam GR, Daneshbod Y. Three Leishmania/L. species–L. infantum, L. major, L. tropica–as causative agents of mucosal leishmaniasis in Iran. Pathog Glob Health. 2013;107:267–72.CrossRefGoogle Scholar
  10. 10.
    Banuls AL, Bastien P, Pomares S, Arevalo J, Fisa R, Hide M. Clinical pleiomorphism in human leishmaniases, with special mention of asymptomatic infection. Clin Microbiol Infect. 2011;17:1451–61.CrossRefGoogle Scholar
  11. 11.
    Remadi L, Haouas N, Chaara D, Slama D, Chargui N, Dabghi R, Jbeniani H, Mezhoud H, Babba H. Clinical presentation of cutaneous leishmaniasis caused by Leishmania major. Dermatology. 2016;232:752–9.CrossRefGoogle Scholar
  12. 12.
    Alam E, Abbas O, Moukarbel R, Khalifeh I. Cutaneous leishmaniasis: an overlooked etiology of midfacial destructive lesions. PLoS Negl Trop Dis. 2016;10:e0004426.CrossRefGoogle Scholar
  13. 13.
    Hurlot Q, Fillaux J, Laurent C, Berry A, Hofman P, Marchou B, Delobel P, Brousset P, Martin-Blondel G. A case report of isolated lymphadenopathy revealing localized leishmanial lymphadenopathy in an asthenic 25-year-old man. Medicine. 2016;95:e3932.CrossRefGoogle Scholar
  14. 14.
    Hashiguchi Y, Gomez EL, Kato H, Martini LR, Velez LN, Uezato H. Diffuse and disseminated cutaneous leishmaniasis: clinical cases experienced in Ecuador and a brief review. Trop Med Health. 2016;44:2.CrossRefGoogle Scholar
  15. 15.
    Rogers MB, Hilley JD, Dickens NJ, Wilkes J, Bates PA, Depledge DP, Harris D, Her Y, Herzyk P, Imamura H, Otto TD, Sanders M, Seeger K, Dujardin JC, Berriman M, Smith DF, Hertz-Fowler C, Mottram JC. Chromosome and gene copy number variation allow major structural change between species and strains of Leishmania. Genome Res. 2011;21:2129–42.CrossRefGoogle Scholar
  16. 16.
    Calvopina M, Armijos RX, Marco JD, Uezato H, Kato H, Gomez EA, Korenaga M, Barroso PA, Mimori T, Cooper PJ, Nonaka S, Hashiguchi Y. Leishmania isoenzyme polymorphisms in Ecuador: relationships with geographic distribution and clinical presentation. BMC Infect Dis. 2006;6:139.CrossRefGoogle Scholar
  17. 17.
    Pratlong F, Dereure J, Ravel C, Lami P, Balard Y, Serres G, Lanotte G, Rioux JA, Dedet JP. Geographical distribution and epidemiological features of Old World cutaneous leishmaniasis foci, based on the isoenzyme analysis of 1048 strains. Trop Med Int Health. 2009;14:1071–85.Google Scholar
  18. 18.
    Azmi K, Nasereddin A, Ereqat S, Schnur L, Schonian G, Abdeen Z. Methods incorporating a polymerase chain reaction and restriction fragment length polymorphism and their use as a ‘gold standard’ in diagnosing Old World cutaneous leishmaniasis. Diagn Microbiol Infect Dis. 2011;71:151–5.CrossRefGoogle Scholar
  19. 19.
    Anders G, Eisenberger CL, Jonas F, Greenblatt CL. Distinguishing Leishmania tropica and Leishmania major in the Middle East using polymerase chain reaction with kinetoplast DNA-specific primers. Trans R Soc Trop Med Hyg. 2002;96:S87–92.CrossRefGoogle Scholar
  20. 20.
    Mauricio IL, Gaunt MW, Stothard JR, Miles MA. Genetic typing and phylogeny of the Leishmania donovani complex by restriction analysis of PCR amplified gp63 intergenic regions. Parasitology. 2001;122:393–403.CrossRefGoogle Scholar
  21. 21.
    Mouttaki T, Morales-Yuste M, Merino-Espinosa G, Chiheb S, Fellah H, Martin-Sanchez J, Riyad M. Molecular diagnosis of cutaneous leishmaniasis and identification of the causative Leishmania species in Morocco by using three PCR-based assays. Parasit Vectors. 2014;7:420.CrossRefGoogle Scholar
  22. 22.
    Khan NH, Messenger LA, Wahid S, Sutherland CJ. Phylogenetic position of Leishmania isolates from Khyber Pakhtunkhwa province of Pakistan. Exp Parasitol. 2016;167:61–6.CrossRefGoogle Scholar
  23. 23.
    Waki K, Dutta S, Ray D, Kolli BK, Akman L, Kawazu SI, Lin CP, Chang KP. Transmembrane molecules for phylogenetic analyses of pathogenic protists: Leishmania-specific informative sites in hydrophilic loops of trans- endoplasmic reticulum N-acetylglucosamine-1-phosphate transferase. Eukaryot Cell. 2007;6:198–210.CrossRefGoogle Scholar
  24. 24.
    Cao DP, Guo XG, Chen DL, Chen JP. Species delimitation and phylogenetic relationships of Chinese Leishmania isolates reexamined using kinetoplast cytochrome oxidase II gene sequences. Parasitol Res. 2011;109:163–73.CrossRefGoogle Scholar
  25. 25.
    Kato H, Gomez EAL, Martini-Robles L, Muzzio J, Velez LN, Calvopina M, Romero-Alvarez D, Mimori T, Uezato H, Hashiguchi Y. Geographic distribution of Leishmania species in Ecuador based on the cytochrome B gene sequence analysis. PLoS Negl Trop Dis. 2016;10:e0004844.CrossRefGoogle Scholar
  26. 26.
    Serin MS, Daglioglu K, Bagirova M, Allahverdiyev A, Uzun S, Vural Z, Kayar B, Tezcan S, Yetkin M, Aslan G, Emekdas G, Koksal F. Rapid diagnosis and genotyping of Leishmania isolates from cutaneous and visceral leishmaniasis by microcapillary cultivation and polymerase chain reaction-restriction fragment length polymorphism of miniexon region. Diagn Microbiol Infect Dis. 2005;53:209–14.CrossRefGoogle Scholar
  27. 27.
    Sun K, Guan W, Zhang JG, Wang YJ, Tian Y, Liao L, Yang BB, Chen DL, Chen JP. Prevalence of canine leishmaniasis in Beichuan County, Sichuan, China and phylogenetic evidence for an undescribed Leishmania sp. in China based on 7SL RNA. Parasit Vectors. 2012;5:75.CrossRefGoogle Scholar
  28. 28.
    Montalvo AM, Fraga J, El Safi S, Gramiccia M, Jaffe CL, Dujardin JC, Van der Auwera G. Direct Leishmania species typing in Old World clinical samples: evaluation of 3 sensitive methods based on the heat-shock protein 70 gene. Diagn Microbiol Infect Dis. 2014;80:35–9.CrossRefGoogle Scholar
  29. 29.
    Chaouch M, Fathallah-Milli A, Driss M, Lahmadi R, Ayari C, Guizani I, Ben Said M, BenAbderrazak S. Identification of Tunisian Leishmania spp. by amplification of cysteine proteinase B (cpb) genes and phylogenetic analysis. Acta Trop. 2013;125:357–65.CrossRefGoogle Scholar
  30. 30.
    Banuls AL, Hide M, Prugnolle F. Leishmania and the Leishmaniases: a parasite genetic update and advances in taxonomy, epidemiology and pathogenicity in humans. Adv Parasitol. 2007;64:1–109.CrossRefGoogle Scholar
  31. 31.
    Yatawara L, Le TH, Wickramasinghe S, Agatsuma T. Maxicircle (mitochondrial) genome sequence (partial) of Leishmania major: gene content, arrangement and composition compared with Leishmania tarentolae. Gene. 2008;424:80–6.CrossRefGoogle Scholar
  32. 32.
    Yang BB, Chen DL, Chen JP, Liao L, Hu XS, Xu JN. Analysis of kinetoplast cytochrome b gene of 16 Leishmania isolates from different foci of China: different species of Leishmania in China and their phylogenetic inference. Parasit Vectors. 2013;6:32.CrossRefGoogle Scholar
  33. 33.
    Asato Y, Oshiro M, Myint CK, Yamamoto Y, Kato H, Marco JD, Mimori T, Gomez EAL, Hashiguchi Y, Uezato H. Phylogenic analysis of the genus Leishmania by cytochrome b gene sequencing. Exp Parasitol. 2009;121:352–61.CrossRefGoogle Scholar
  34. 34.
    Luyo-Acero GE, Uezato H, Oshiro M, Takei K, Kariya K, Katakura K, Gomez-Landires E, Hashiguchi Y, Nonaka S. Sequence variation of the cytochrome b gene of various human infecting members of the genus Leishmania and their phylogeny. Parasitology. 2004;128:483–91.CrossRefGoogle Scholar
  35. 35.
    Aransay AM, Scoulica E, Tselentis Y. Detection and identification of Leishmania DNA within naturally infected sand flies by semi-nested PCR on minicircle kinetoplastic DNA. Appl Environ Microbiol. 2000;66:1933–8.CrossRefGoogle Scholar
  36. 36.
    Edgar RC. MUSCLE: multiple sequence alignment with high accuracy and high throughput. Nucleic Acids Res. 2004;32:1792–7.CrossRefGoogle Scholar
  37. 37.
    Camacho C, Coulouris G, Avagyan V, Ma N, Papadopoulos J, Bealer K, Madden TL. BLAST+: architecture and applications. BMC Bioinf. 2009;10:421.CrossRefGoogle Scholar
  38. 38.
    Hall TA. BioEdit: a user-friendly biological sequence alignment editor and analysis program for windows 95/98/NT. Nucleic Acids Symp Ser. 1999;41:95–8.Google Scholar
  39. 39.
    Kumar S, Stecher G, Li M, Knyaz C, Tamura K. MEGA X: Molecular evolutionary genetics analysis across computing platforms. Mol Biol Evol. 2018;35:1547–9.CrossRefGoogle Scholar
  40. 40.
    Zare M, Rezaianzadeh A, Tabatabaee H, Aliakbarpoor M, Faramarzi H, Ebrahimi M. Spatiotemporal clustering of cutaneous leishmaniasis in Fars province, Iran. Asian Pac J Trop Biomed. 2017;7:862–9.CrossRefGoogle Scholar
  41. 41.
    Razmjou S, Hejazy H, Motazedian MH, Baghaei M, Emamy M, Kalantary M. A new focus of zoonotic cutaneous leishmaniasis in shiraz, Iran. Trans R Soc Trop Med Hyg. 2009;103:727–30.CrossRefGoogle Scholar
  42. 42.
    Spotin A, Rouhani S, Parvizi P. The associations of Leishmania major and Leishmania tropica aspects by focusing their morphological and molecular features on clinical appearances in Khuzestan province, Iran. BioMed Res Int. 2014:1–13. Article ID 913510.  https://doi.org/10.1155/2014/913510.
  43. 43.
    Fotouhi-Ardakani R, Dabiri S, Ajdari S, Alimohammadian MH, AlaeeNovin E, Taleshi N, Parvizi P. Assessment of nuclear and mitochondrial genes in precise identification and analysis of genetic polymorphisms for the evaluation of Leishmania parasites. Infect Genet Evol. 2016;46:33–41.CrossRefGoogle Scholar
  44. 44.
    Foulet F, Botterel F, Buffet P, Morizot G, Rivollet D, Deniau M, Pratlong F, Costa JM, Bretagne S. Detection and identification of Leishmania species from clinical specimens by using a real time PCR assay and sequencing of the cytochrome B gene. J Clin Microbiol. 2007;45:2110–5.CrossRefGoogle Scholar
  45. 45.
    Martinez LP, Rebollo JA, Luna AL, Cochero S, Bejarano EE. Molecular identification of the parasites causing cutaneous leishmaniasis on the Caribbean coast of Colombia. Parasitol Res. 2010;106:647–52.CrossRefGoogle Scholar
  46. 46.
    Kato H, Watanabe J, Nieto IM, Korenaga M, Hashiguchi Y. Leishmania species identification using FTA card sampling directly from patients’ cutaneous lesions in the state of Lara, Venezuela. Trans R Soc Trop Med Hyg. 2011;105:561–7.CrossRefGoogle Scholar
  47. 47.
    Marco JD, Bhutto AM, Soomro FR, Baloch JH, Barroso PA, Kato H, Uezato H, Katakura K, Korenaga M, Nonaka S, Hashiguchi Y. Multilocus enzyme electrophoresis and cytochrome b gene sequencing–based identification of Leishmania isolates from different foci of cutaneous leishmaniasis in Pakistan. Am J Trop Med Hyg. 2006;75:261–6.CrossRefGoogle Scholar
  48. 48.
    Marco JD, Uezato H, Mimori T, Barroso PA, Korenaga M, Nonaka S, Basombrio MA, Taranto NJ, Hashiguchi Y. Are cytochrome b gene sequencing and polymorphism-specific polymerase chain reaction as reliable as multilocus enzyme electrophoresis for identifying Leishmania spp. from Argentina? Am J Trop Med Hyg. 2006;75:256–60.Google Scholar
  49. 49.
    Myint CK, Asato Y, Yamamoto Y, Kato H, Bhutto AM, Soomro FR, Memon MZ, Matsumoto J, Marco JD, Oshiro M, Katakura K, Hashiguchi Y, Uezato H. Polymorphisms of cytochrome b gene in Leishmania parasites and their relation to types of cutaneous leishmaniasis lesions in Pakistan. J Dermatol. 2008;35:76–85.CrossRefGoogle Scholar
  50. 50.
    Khan NH, Bari AU, Hashim R, Khan I, Muneer A, Shah A, Wahid S, Yardley V, O’Neil B, Sutherland CJ. Cutaneous leishmaniasis in Khyber Pakhtunkhwa province of Pakistan: clinical diversity and species-level diagnosis. Am J Trop Med Hyg. 2016;95:1106–14.CrossRefGoogle Scholar
  51. 51.
    Ramirez JD, Hernandez C, Leon CM, Ayala MS, Florez C, Gonzalez C. Taxonomy, diversity, temporal and geographical distribution of cutaneous leishmaniasis in Colombia: a retrospective study. Sci Rep. 2016;6:28266.CrossRefGoogle Scholar
  52. 52.
    Rogers MB, Downing T, Smith BA, Imamura H, Sanders M, Svobodova M, Volf P, Berriman M, Cotton JA, Smith DF. Genomic confirmation of hybridization and recent inbreeding in a vector-isolated Leishmania population. PLoS Genet. 2014;10:e1004092.CrossRefGoogle Scholar
  53. 53.
    Ramirez JD, Llewellyn M. Reproductive clonality in protozoan pathogens – truth or artefact? Mol Ecol. 2014;23:4195–202.CrossRefGoogle Scholar
  54. 54.
    Kato H, Caceres AG, Hashiguchi Y. First evidence of a hybrid of Leishmania (Viannia) braziliensis/L.: (V.) peruviana DNA detected from the phlebotomine sand fly Lutzomyia tejadai in Peru. PLoS Negl Trop Dis. 2016;10:e0004336.CrossRefGoogle Scholar
  55. 55.
    Odiwuor S, De Doncker S, Maes I, Dujardin JC, Van der Auwera G. Natural Leishmania donovani/Leishmania aethiopica hybrids identified from Ethiopia. Infect Genet Evol. 2011;11:2113–8.CrossRefGoogle Scholar
  56. 56.
    Ravel C, Cortes S, Pratlong F, Morio F, Dedet JP, Campino L. First report of genetic hybrids between two very divergent Leishmania species: Leishmania infantum and Leishmania major. Int J Parasitol. 2006;36:1383–8.CrossRefGoogle Scholar
  57. 57.
    Volf P, Benková I, Myšková J, Sádlová J, Campino L, Ravel C. Increased transmission potential of Leishmania major/Leishmania infantum hybrids. Int J Parasitol. 2007;37:589–93.CrossRefGoogle Scholar
  58. 58.
    Baghaei M. Intraspecific variation in Leishmania major isolated from different forms of zoonotic cutaneous leishmaniasis. Iran J Med Sci. 2005;30:51–4.Google Scholar
  59. 59.
    Ghatee MA, Sharifi I, Kuhls K, Kanannejad Z, Fasihi Harandi M, de Almeida ME, Hatam GR, Mirhendi H. Heterogeneity of the internal transcribed spacer region in Leishmania tropica isolates from southern Iran. Exp Parasitol. 2014;144:44–51.CrossRefGoogle Scholar
  60. 60.
    Tashakori M, Kuhls K, Al-Jawabreh A, Mauricio I, Schonian G, Farajnia S, Alimohammadian MH. Leishmania major: genetic heterogeneity of Iranian isolates by single-strand conformation polymorphism and sequence analysis of ribosomal DNA internal transcribed spacer. Acta Trop. 2006;98:52–8.CrossRefGoogle Scholar
  61. 61.
    Oryan A, Shirian S, Tabandeh MR, Hatam GR, Randau G, Daneshbod Y. Genetic diversity of Leishmania major strains isolated from different clinical forms of cutaneous leishmaniasis in southern Iran based on minicircle kDNA. Infect Genet Evol. 2013;19:226–31.CrossRefGoogle Scholar
  62. 62.
    Shirian S, Oryan A, Hatam GR, Tabandeh MR, Daneshmand E, Hashemi Orimi M, Saberi H, Daneshbod Y. Correlation of genetic heterogeneity with cytopathological and epidemiological findings of Leishmania major isolated from cutaneous leishmaniasis in southern Iran. Acta Cytol. 2016;60:97–106.CrossRefGoogle Scholar
  63. 63.
    van Thiel PPAM, van Gool T, Faber WR, Leenstra T, Kager PA, Bart A. Variation in clinical presentation and genotype of causative Leishmania major strain in cutaneous leishmaniasis in north and south Afghanistan. Am J Trop Med Hyg. 2011;85:60–3.Google Scholar
  64. 64.
    Fakhar M, Pazoki Ghohe H, Rasooli SA, Karamian M, Mohib AS, Ziaei Hezarjaribi H, Pagheh AS, Ghatee MA. Genetic diversity of Leishmania tropica strains isolated from clinical forms of cutaneous leishmaniasis in rural districts of Herat province, western Afghanistan, based on ITS1-rDNA. Infect Genet Evol. 2016;41:120–7.Google Scholar
  65. 65.
    Eslami G, Salehi R, Khosravi S, Doudi M. Genetic analysis of clinical isolates of Leishmania major from Isfahan, Iran. J Vector Borne Dis. 2012;49:168–74.PubMedGoogle Scholar
  66. 66.
    Dabirzadeh M, Mirmohammad Sadeghi H, Baghaie M, Hejazi H. Genetic polymorphism of Leishmania major in two hyper endemic regions of Iran revealed by PPIP-PCR and ITS-RFLP. Arch Iran Med. 2012;15:151–6.PubMedGoogle Scholar
  67. 67.
    Akhoundi M, Hajjaran H, Baghaei A, Mohebali M. Geographical distribution of Leishmania species of human cutaneous leishmaniasis in Fars province, southern Iran. Iran J Parasitol. 2013;8:85–91.Google Scholar
  68. 68.
    Ajaoud M, Es-Sette N, Hamdi S, El-Idrissi AL, Riyad M, Lemrani M. Detection and molecular typing of Leishmania tropica from Phlebotomus sergenti and lesions of cutaneous leishmaniasis in an emerging focus of Morocco. Parasit Vectors. 2013;6:217.CrossRefGoogle Scholar
  69. 69.
    Schonian G, Schnur L, El Fari M, Oskam L, Kolesnikov AA, Sokolowska-Kohler W, Presber W. Genetic heterogeneity in the species Leishmania tropica revealed by different PCR-based methods. Trans R Soc Trop Med Hyg. 2001;95:217–24.CrossRefGoogle Scholar
  70. 70.
    Sarkari B, Bavarsad Ahmadpour N, Motazedian MH, Mirjalali H, Akhoundi M, Mohebali M, Hajjaran H. Inter- and intra-specific variations of Leishmania strains isolated from patients with cutaneous and visceral leishmaniases in Fars province, south of Iran. Iran J Med Sci. 2016;41:209–16.PubMedGoogle Scholar
  71. 71.
    Hajjaran H, Mohebali M, Teimouri A, Oshaghi MA, Mirjalali H, Kazemi-Rad E, Shiee MR, Naddaf SR. Identification and phylogenetic relationship of Iranian strains of various Leishmania species isolated from cutaneous and visceral cases of leishmaniasis based on N-acetylglucosamine-1-phosphate transferase gene. Infect Genet Evol. 2014;26:203–12.CrossRefGoogle Scholar
  72. 72.
    Yazidi R, Bettaieb J, Ghawar W, Jaouadi K, Châabane S, Zaatour A, Salah AB. RAPD-PCR reveals genetic polymorphism among Leishmania major strains from Tunisian patients. BMC Infect Dis. 2015;15:269.CrossRefGoogle Scholar
  73. 73.
    Mahmoudzadeh-Niknam H, Ajdary S, Riazi-Rad F, Mirzadegan E, Rezaeian A, Khaze V, Djadid ND, Alimohammadian MH. Molecular epidemiology of cutaneous leishmaniasis and heterogeneity of Leishmania major strains in Iran. Trop Med Int Health. 2012;11:1335–44.Google Scholar
  74. 74.
    Toledo A, Martin-Sanchez J, Pesson B, Sanchiz-Martin C, Morillas-Marquez F. Genetic variability within the species Leishmania infantum by RAPD. A lack of correlation with zymodeme structure. Mol Biochem Parasitol. 2002;119:257–64.CrossRefGoogle Scholar
  75. 75.
    Al-Jawabreh A, Diezmann S, Müller M, Wirth T, Schnur LF, Strelkova MV, Kovalenko DA, Razakov SA, Schwenkenbecher JM, Kuhls K, Schonian G. Identification of geographically distributed sub-populations of Leishmania (Leishmania) major by microsatellite analysis. BMC Evol Biol. 2008;8:183.CrossRefGoogle Scholar
  76. 76.
    Alimohammadian MH, Darabi H, Ajdary S, Khaze V, Torkabadi E. Genotypically distinct strains of Leishmania major display diverse clinical and immunological patterns in BALB/c mice. Infect Genet Evol. 2010;10:969–75.CrossRefGoogle Scholar
  77. 77.
    Ribas-Silva RC, Ribas AD, Dos Santos MC, da Silva WV, Lonardoni MV, Borelli SD, Silveira TG. Association between HLA genes and American cutaneous leishmaniasis in endemic regions of southern Brazil. BMC Infect Dis. 2013;13:198.CrossRefGoogle Scholar
  78. 78.
    Samaranayake N, Fernando SD, Neththikumara NF, Rodrigo C, Karunaweera ND, Dissanayake VH. Association of HLA class I and II genes with cutaneous leishmaniasis: a case control study from Sri Lanka and a systematic review. BMC Infect Dis. 2016;16:292.CrossRefGoogle Scholar
  79. 79.
    Lopes ME, Carneiro MB, Dos Santos LM, Vieira LQ. Indigenous microbiota and leishmaniasis. Parasite Immunol. 2016;38:37–44.CrossRefGoogle Scholar
  80. 80.
    Sakthianandeswaren A, Foote SJ, Handman E. The role of host genetics in leishmaniasis. Trends Parasitol. 2009;25:383–91.CrossRefGoogle Scholar
  81. 81.
    Oliveira WN, Ribeiro LE, Schrieffer A, Machado P, Carvalho EM, Bacellar O. The role of inflammatory and anti-inflammatory cytokines in the pathogenesis of human tegumentary leishmaniasis. Cytokine. 2014;66:127–32.CrossRefGoogle Scholar
  82. 82.
    Antonelli LRV, Dutra WO, Almeida RP, Bacellar O, Carvalho EM, Gollob KJ. Activated inflammatory T cells correlate with lesion size in human cutaneous leishmaniasis. Immunol Lett. 2005;101:226–30.CrossRefGoogle Scholar
  83. 83.
    Oliveira F, Bafica A, Rosato AB, Favali CB, Costa JM, Cafe V, Barral-Netto M, Barral A. Lesion size correlates with Leishmania antigen-stimulated TNF-levels in human cutaneous leishmaniasis. Am J Trop Med Hyg. 2011;85:70–3.CrossRefGoogle Scholar
  84. 84.
    Faria DR, Souza PE, Duraes FV, Carvalho EM, Gollob KJ, Machado PR, Dutra WO. Recruitment of CD8+ T cells expressing granzyme A is associated with lesion progression in human cutaneous leishmaniasis. Parasite Immunol. 2009;31:432–9.Google Scholar
  85. 85.
    Convit J, Ulrich M, Perez M, Hung J, Castillo J, Rojas H, Viquez A, Araya LN, Lima HD. Atypical cutaneous leishmaniasis in central America: possible interaction between infectious and environmental elements. Trans R Soc Trop Med Hyg. 2005;99:13–7.Google Scholar

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© The Author(s). 2019

Open AccessThis article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated.

Authors and Affiliations

  1. 1.Department of Medical Parasitology and Mycology, School of MedicineShiraz University of Medical SciencesShirazIran
  2. 2.Molecular Dermatology Research Center, Department of Dermatology, School of MedicineShiraz University of Medical SciencesShirazIran
  3. 3.Department of Molecular Pathology, School of MedicineShiraz University of Medical SciencesShirazIran
  4. 4.Fajr Health CenterShiraz University of Medical SciencesShirazIran
  5. 5.Basic Sciences in Infectious Diseases Research Center, School of MedicineShiraz University of Medical SciencesShirazIran

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