# Physiological Age Structure andLeishmania spp. Detection in Phlebotomus (Larroussius) orientalis (Parrot, 1936) (Diptera: Psychodidae) at an Endemic Focus of Visceral Leishmaniasis in Northern Ethiopia

Authors: Araya Gebresilassie; Ibrahim Abbasi; Oscar David Kirstein; Essayas Aklilu; Solomon Yared; Habte Tekie; Meshesha Balkew; Alon Warburg; Asrat Hailu; Teshome Gebre-Michael
Journal: Journal of Tropical Medicine
 (2015)

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## Abstract

Visceral leishmaniasis (VL) caused byLeishmania donovani is endemic in northern Ethiopia, where P. orientalis is the most important presumed vector. This study was designed to determine the physiological age structure and the occurrence of Leishmania infection in the vector of VL in Tahtay Adiyabo district, northern Ethiopia. Sand flies were collected using CDC light traps from peridomestic and agricultural fields between May 2011 and April 2012 and P. orientalis females were dissected for age determination and detection of Leishmania promastigotes. Sand flies were also analyzed for L. donovani detection using molecular methods. Of 1,282 P. orientalis examined for abdominal stages and age characterization, 66.2%, 28.2%, 4.1%, and 1.6% were unfed, freshly fed, half-gravid, and gravid. Parous rate in unfed females was 34.1% and 35.4% in peridomestic and agricultural fields, respectively. Out of 921 P. orientalis females dissected, one specimen (0.1%) was found naturally infected with promastigotes. Five pools (25 females) of unfed P. orientalis were also found with DNA of Leishmania spp. In particular, a single P. orientalis was positive for L. donovani (0.5%). Based on this and other evidences (abundance, human blood feeding, and xenodiagnostic studies), P. orientalis is the principal vector of VL in this endemic focus.


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## Body

## 1. Introduction

Visceral leishmaniasis, whose causative agent isL. donovani, is a common parasitic infection and a major public health concern in East African countries with approximately 29,400 to 56,700 new cases each year [1]. In Ethiopia, the first case of VL was identified in the 1940s in the lower Omo plains, the southwestern part of the country [2]. Subsequently, the disease has been known to be endemic in many parts of the country. The main endemic areas foci of VL in the country include the Humera and Metema plains in the northwest [3–5], Omo plains, Aba Roba focus, and Weyto River Valley in the southwest [5–7]. However, recently increasing VL cases have been reported from previously nonendemic regions such as Libo Kemkem district of Amhara and Tahtay Adiyabo district in Tigray, northern Ethiopia [8, 9], causing high mortality and morbidity among the local residents.The distribution of VL depends on the presence of competent vectors and reservoir hosts in a particular area. Detection of natural infection withLeishmania and determination of the physiological age structure of field caught sand fly vectors are of prime importance in vectorial and epidemiological studies of leishmaniasis [10]. The infection of competent vectors withLeishmania promastigotes has been determined by dissection of individual sand flies under a microscope. However, the use of this method to determine infection rate is difficult because promastigote infection in competent vectors is generally low and estimation of infection rate requires the examination of a large number of specimens. Previous microscopical surveys on different species of sand flies in different regions showed infection rates ranging from 1.7% to 10.7% [11–14]. Recently, polymerase chain reaction- (PCR-) based techniques have been employed to detectLeishmania spp. in sand flies [15–17].In different parts of Ethiopia,P. martini,P. celiae, andP. orientalis have been found infected withL. donovani and implicated as vectors of VL [13, 18]. In particular,P. orientalis has been suspected as the vector of VL in the north and northwest of Ethiopia [19, 20], but it has already been incriminated in the adjacent endemic regions of Sudan [14, 21, 22]. However, data on the determination of the physiological age structure and natural infection ofLeishmania parasites withinPhlebotomus spp., specifically from the VL endemic area of Tahtay Adiyabo, is lacking. Therefore, the current study was carried out with the aim of determining the physiological age structure and the occurrence ofLeishmania parasites in vector of VL in the study area.


## 2. Materials and Methods

### 2.1. Study Area and Sand Fly Collection

Field collection of sand flies was conducted in three villages (namely, Ademeyti, Lemlem, and Mentebteb) of Tahtay Adiyabo district (14°23′41′′N/37°46′15′′E) in the Tigray Regional State, northern Ethiopia. The ecology and physical environment of the study area have previously been described in detail in Gebresilassie et al. [23]. Sand flies used in the present study were originally sampled, collected, and identified as published in [23]. Briefly, female sand flies were collected from three different villages of the study area using CDC light traps between May 2011 and April 2012. Trapping of sand flies from peridomestic (places with human and animal shelters) and agricultural fields (on the periphery of settlements) was conducted for 12 nights per month. Five CDC light traps suspended with 40–50 cm above the ground level were randomly distributed to representative locations of peridomestic habitats and agricultural fields.


### 2.2. Determination of Abdominal Status, Parous Rates, and Infection Rates of Phlebotomus spp.

Sand flies caught in CDC light traps from various sampling habitats were transported to a laboratory and females were transferred to test tubes. They were then knocked down using chloroform and emptied on Petri dishes for sorting into different categories (genera, sex, and abdominal status) under a dissecting microscope.Phlebotomus females were categorized into unfed, semigravid, gravid, and freshly fed. The freshly fed females were preserved in ethanol for parasite detection by PCR. Unfed, gravid, and semigravid female sand flies were washed in 2% savlon/saline solution followed by sterile physiological saline and dissected in sterile physiological saline for the detection of promastigotes [24]. After dissection, the ovaries of unfedPhlebotomus females were drawn out together with the guts to determine their parous state (parous or nulliparous). Parity was determined based on the presence of granules in the accessory glands [25] and the states of the ovaries [24]. The gut contents of parous, gravid, and semigravid females were examined under a phase contrast microscope at 40 × 10 magnifications for the presence ofLeishmania promastigotes. When promastigotes were observed in dissected females, the gut with its content was kept in 70% ethanol and stored at −20°C for later PCR detection ofLeishmania. Unfortunately, the promastigote positive guts could not be cultured into NNN media due to the scarcity of these media during the time of dissection.UndissectedPhlebotomus females were also preserved in 70% ethanol and stored at −20°C for later PCR detection ofLeishmania. The head and abdominal tips from the above process were mounted on glass slides using Hoyer medium and identified using the identification keys of [26–28].


### 2.3. Detection ofLeishmania Parasites by PCR

#### 2.3.1. DNA Extraction

P. orientalis females with abdominal status of unfed, half-gravid, and gravid were first grouped into 115 pools according to sampling date, collection site, and abdominal conditions with up to five specimens in each pool. Following this, DNA was extracted in pools from these specimens using phenol and chloroform method [9]. At the same time, DNA was processed individually from blood-fed females. Briefly, ethanol-preserved sand flies were incubated in a microfuge tube with 200 μL of lysis buffer (50 mM NaCl, 10 mM EDTA, 50 mM Tris-HCl pH 7.4, 1% triton X-100, and 200 μg/mL of proteinase K) at 65°C for 2 hours. Equal volumes of TE-saturated phenol (pH 8) were added to the aqueous solution; the mixture was vortexed for few seconds and then centrifuged for 2 minutes at 14,000 rpm. The upper aqueous layer was transferred to a new microcentrifuge tube and the DNA was precipitated by adding NaCl to a concentration of 0.2 M (addition of 8 μL of 5 M NaCl to 200 μL aqueous solution) and 2.5 volumes of 100% cold ethanol. DNA was incubated at −20°C overnight and centrifuged at 14,000 rpm for 10 minutes. The supernatant was discarded and the DNA pellet was dried in speed-vac. The DNA pellet was suspended with double distilled water and stored at −20°C until use for PCR.


#### 2.3.2. ITS Polymerase Chain Reaction (PCR)

PCR reactions were carried out in a volume of 25μL using ready mix PCR tubes (Syntezza, Jerusalem, Israel). For each reaction, 20 pmoles of the two 320 bpLeishmania specific ribosomal internal transcribed spacer 1 (ITS1) regions using the primers LITSR (5′-CTG GAT CAT TTT CCG ATG-3′) and L5.8S (5′-TGA TAC CAC TTA TCG CACTT-3′) was added followed by 5 μL of the template DNA [29]. Double distilled water along with primers and DNA from promastigotes ofL. donovani,L. major,L. aethiopica, andL. tropica was used as negative and positive controls, respectively. The thermal profile comprised 5 min at 95°C, followed by 35 cycles starting at 95°C for 30 seconds, 56°C for 30 seconds, and 72°C for 1 min, with a final elongation step at 72°C for 10 min.


#### 2.3.3. Gel Electrophoresis

Amplified products (7μL) were run on 1.5% agarose gel containing ethidium bromide for 1 h at 80 V. The gel products were visualized under ultraviolet (UV) transilluminator and then digital photographs were prepared.Leishmania infections were identified by comparison of PCR products of specimens with the reference strains and molecular weight markers.DNA Sequencing. The amplified ITS1 PCR products that demonstrated a moderate to strong ITS1 bands were sequenced by automated fluorescent DNA sequencing using ABI PRISM 377 sequencer (PE Biosystems, Foster City, California). The sequences obtained were compared for their homology to known sequences in the GenBank database using BLAST online service provided through the PubMed/US National Institute of Health (http://www.ncbi.nlm.nih.gov/BLAST).


## 2.1. Study Area and Sand Fly Collection

Field collection of sand flies was conducted in three villages (namely, Ademeyti, Lemlem, and Mentebteb) of Tahtay Adiyabo district (14°23′41′′N/37°46′15′′E) in the Tigray Regional State, northern Ethiopia. The ecology and physical environment of the study area have previously been described in detail in Gebresilassie et al. [23]. Sand flies used in the present study were originally sampled, collected, and identified as published in [23]. Briefly, female sand flies were collected from three different villages of the study area using CDC light traps between May 2011 and April 2012. Trapping of sand flies from peridomestic (places with human and animal shelters) and agricultural fields (on the periphery of settlements) was conducted for 12 nights per month. Five CDC light traps suspended with 40–50 cm above the ground level were randomly distributed to representative locations of peridomestic habitats and agricultural fields.


## 2.2. Determination of Abdominal Status, Parous Rates, and Infection Rates of Phlebotomus spp.

Sand flies caught in CDC light traps from various sampling habitats were transported to a laboratory and females were transferred to test tubes. They were then knocked down using chloroform and emptied on Petri dishes for sorting into different categories (genera, sex, and abdominal status) under a dissecting microscope.Phlebotomus females were categorized into unfed, semigravid, gravid, and freshly fed. The freshly fed females were preserved in ethanol for parasite detection by PCR. Unfed, gravid, and semigravid female sand flies were washed in 2% savlon/saline solution followed by sterile physiological saline and dissected in sterile physiological saline for the detection of promastigotes [24]. After dissection, the ovaries of unfedPhlebotomus females were drawn out together with the guts to determine their parous state (parous or nulliparous). Parity was determined based on the presence of granules in the accessory glands [25] and the states of the ovaries [24]. The gut contents of parous, gravid, and semigravid females were examined under a phase contrast microscope at 40 × 10 magnifications for the presence ofLeishmania promastigotes. When promastigotes were observed in dissected females, the gut with its content was kept in 70% ethanol and stored at −20°C for later PCR detection ofLeishmania. Unfortunately, the promastigote positive guts could not be cultured into NNN media due to the scarcity of these media during the time of dissection.UndissectedPhlebotomus females were also preserved in 70% ethanol and stored at −20°C for later PCR detection ofLeishmania. The head and abdominal tips from the above process were mounted on glass slides using Hoyer medium and identified using the identification keys of [26–28].


## 2.3. Detection ofLeishmania Parasites by PCR

### 2.3.1. DNA Extraction

P. orientalis females with abdominal status of unfed, half-gravid, and gravid were first grouped into 115 pools according to sampling date, collection site, and abdominal conditions with up to five specimens in each pool. Following this, DNA was extracted in pools from these specimens using phenol and chloroform method [9]. At the same time, DNA was processed individually from blood-fed females. Briefly, ethanol-preserved sand flies were incubated in a microfuge tube with 200 μL of lysis buffer (50 mM NaCl, 10 mM EDTA, 50 mM Tris-HCl pH 7.4, 1% triton X-100, and 200 μg/mL of proteinase K) at 65°C for 2 hours. Equal volumes of TE-saturated phenol (pH 8) were added to the aqueous solution; the mixture was vortexed for few seconds and then centrifuged for 2 minutes at 14,000 rpm. The upper aqueous layer was transferred to a new microcentrifuge tube and the DNA was precipitated by adding NaCl to a concentration of 0.2 M (addition of 8 μL of 5 M NaCl to 200 μL aqueous solution) and 2.5 volumes of 100% cold ethanol. DNA was incubated at −20°C overnight and centrifuged at 14,000 rpm for 10 minutes. The supernatant was discarded and the DNA pellet was dried in speed-vac. The DNA pellet was suspended with double distilled water and stored at −20°C until use for PCR.


### 2.3.2. ITS Polymerase Chain Reaction (PCR)

PCR reactions were carried out in a volume of 25μL using ready mix PCR tubes (Syntezza, Jerusalem, Israel). For each reaction, 20 pmoles of the two 320 bpLeishmania specific ribosomal internal transcribed spacer 1 (ITS1) regions using the primers LITSR (5′-CTG GAT CAT TTT CCG ATG-3′) and L5.8S (5′-TGA TAC CAC TTA TCG CACTT-3′) was added followed by 5 μL of the template DNA [29]. Double distilled water along with primers and DNA from promastigotes ofL. donovani,L. major,L. aethiopica, andL. tropica was used as negative and positive controls, respectively. The thermal profile comprised 5 min at 95°C, followed by 35 cycles starting at 95°C for 30 seconds, 56°C for 30 seconds, and 72°C for 1 min, with a final elongation step at 72°C for 10 min.


### 2.3.3. Gel Electrophoresis

Amplified products (7μL) were run on 1.5% agarose gel containing ethidium bromide for 1 h at 80 V. The gel products were visualized under ultraviolet (UV) transilluminator and then digital photographs were prepared.Leishmania infections were identified by comparison of PCR products of specimens with the reference strains and molecular weight markers.DNA Sequencing. The amplified ITS1 PCR products that demonstrated a moderate to strong ITS1 bands were sequenced by automated fluorescent DNA sequencing using ABI PRISM 377 sequencer (PE Biosystems, Foster City, California). The sequences obtained were compared for their homology to known sequences in the GenBank database using BLAST online service provided through the PubMed/US National Institute of Health (http://www.ncbi.nlm.nih.gov/BLAST).


## 2.3.1. DNA Extraction

P. orientalis females with abdominal status of unfed, half-gravid, and gravid were first grouped into 115 pools according to sampling date, collection site, and abdominal conditions with up to five specimens in each pool. Following this, DNA was extracted in pools from these specimens using phenol and chloroform method [9]. At the same time, DNA was processed individually from blood-fed females. Briefly, ethanol-preserved sand flies were incubated in a microfuge tube with 200 μL of lysis buffer (50 mM NaCl, 10 mM EDTA, 50 mM Tris-HCl pH 7.4, 1% triton X-100, and 200 μg/mL of proteinase K) at 65°C for 2 hours. Equal volumes of TE-saturated phenol (pH 8) were added to the aqueous solution; the mixture was vortexed for few seconds and then centrifuged for 2 minutes at 14,000 rpm. The upper aqueous layer was transferred to a new microcentrifuge tube and the DNA was precipitated by adding NaCl to a concentration of 0.2 M (addition of 8 μL of 5 M NaCl to 200 μL aqueous solution) and 2.5 volumes of 100% cold ethanol. DNA was incubated at −20°C overnight and centrifuged at 14,000 rpm for 10 minutes. The supernatant was discarded and the DNA pellet was dried in speed-vac. The DNA pellet was suspended with double distilled water and stored at −20°C until use for PCR.


## 2.3.2. ITS Polymerase Chain Reaction (PCR)

PCR reactions were carried out in a volume of 25μL using ready mix PCR tubes (Syntezza, Jerusalem, Israel). For each reaction, 20 pmoles of the two 320 bpLeishmania specific ribosomal internal transcribed spacer 1 (ITS1) regions using the primers LITSR (5′-CTG GAT CAT TTT CCG ATG-3′) and L5.8S (5′-TGA TAC CAC TTA TCG CACTT-3′) was added followed by 5 μL of the template DNA [29]. Double distilled water along with primers and DNA from promastigotes ofL. donovani,L. major,L. aethiopica, andL. tropica was used as negative and positive controls, respectively. The thermal profile comprised 5 min at 95°C, followed by 35 cycles starting at 95°C for 30 seconds, 56°C for 30 seconds, and 72°C for 1 min, with a final elongation step at 72°C for 10 min.


## 2.3.3. Gel Electrophoresis

Amplified products (7μL) were run on 1.5% agarose gel containing ethidium bromide for 1 h at 80 V. The gel products were visualized under ultraviolet (UV) transilluminator and then digital photographs were prepared.Leishmania infections were identified by comparison of PCR products of specimens with the reference strains and molecular weight markers.DNA Sequencing. The amplified ITS1 PCR products that demonstrated a moderate to strong ITS1 bands were sequenced by automated fluorescent DNA sequencing using ABI PRISM 377 sequencer (PE Biosystems, Foster City, California). The sequences obtained were compared for their homology to known sequences in the GenBank database using BLAST online service provided through the PubMed/US National Institute of Health (http://www.ncbi.nlm.nih.gov/BLAST).


## 3. Results

### 3.1. Abdominal Status and Parous Rates

Tables1 and 2 show the abdominal categories of differentPhlebotomus spp. collected from the study villages. In Ademeyti, the number of unfed, freshly fed, half-gravid, and gravidP. orientalis females from peridomestic habitat was 180, 163, 17, and 2, respectively (Table 1). Similarly, more numbers of unfed (n=197) and engorged (n=133)P. orientalis were found in peridomestic biotopes of Lemlem village. Of the 60 females ofP. orientalis obtained from Mentebteb, 40 were unfed, 17 freshly fed, and 3 gravid and half-gravid.Table 1
Abdominal status of femalePhlebotomus spp. captured from peridomestic sites in three different villages, May 2011 to April 2012.
Species
Number of dissected
Number of  unfed
Number of freshly fed
Number of half-gravid
Number of gravid
Total
Adm.
Lem.
Men.
Adm.
Lem.
Men.
Adm.
Lem.
Men.
Adm.
Lem.
Men.
Adm.
Lem.
Men.
P. orientalis
362
334
60
180
197
40
163
133
17
17
2
1
2
2
2
756
P. bergeroti
3
10
1
1
3
0
2
0
0
1
2
0
1
3
1
14
P. martini
0
0
2
0
0
0
0
0
0
0
0
0
2
0
0
2
P. papatasi
2
3
0
2
3
0
0
0
0
0
0
0
0
0
0
5
P. duboscqi
2
1
0
2
1
0
0
0
0
0
0
0
0
0
0
3
P. lesleyae
1
0
0
1
0
0
0
0
0
0
0
0
0
0
0
1
Total
370
348
63
186
204
40
165
133
17
18
4
1
5
5
3
781
Adm: Ademeyti; Lem: Lemlem; Men: Mentebteb.Table 2
Abdominal status of femalePhlebotomus spp. collected from agricultural fields in three different villages, May 2011 to April 2012.
Species
Number of dissected
Number of  unfed
Number of freshly fed
Number of half-gravid
Number of gravid
Total
Adm.
Lem.
Men.
Adm.
Lem.
Men.
Adm.
Lem.
Men.
Adm.
Lem.
Men.
Adm.
Lem.
Men.
P. orientalis
173
264
87
144
200
86
24
24
0
0
31
1
5
9
0
524
P. bergeroti
0
2
2
0
1
1
0
0
0
0
0
0
0
1
1
4
P. martini
2
1
0
1
0
0
0
0
0
1
1
0
0
0
0
3
P. rodhaini
1
3
0
1
3
0
0
0
0
0
0
0
0
0
0
4
P. papatasi
0
1
0
0
1
0
0
0
0
0
0
0
0
0
0
1
P. duboscqi
0
0
0
0
0
0
0
0
0
0
0
0
0
0
0
0
P. lesleyae
2
31
0
2
31
0
0
0
0
0
0
0
0
0
0
33
P. heischi
0
2
0
0
2
0
0
0
0
0
0
0
0
0
0
2
Total
178
304
89
148
238
87
24
24
0
1
32
1
5
10
1
571
Adm: Ademeyti; Lem: Lemlem; Men: Mentebteb.Of the total 524 females ofP. orientalis dissected from agricultural fields, 430, 48, 32, and 14 were unfed, freshly fed, half-gravid, and gravid females, respectively (Table 2). Less numbers of blood-fed females were caught in agricultural fields of Ademeyti and Lemlem villages. Likewise, no blood-fed females were detected in agricultural fields of Mentebteb. However, more numbers of (n=32) half-gravid females were recorded in Lemlem than the two villages.In total, 847 unfedP. orientalis were dissected and examined for parous state based on the appearance of accessory glands and condition of ovaries (Table 3). Of 417P. orientalis dissected in peridomestic biotopes, 142 (34.1%) were parous: 33.3%, 30.9%, and 52.5% in Ademeyti, Lemlem, and Mentebteb villages, respectively, while the parous rate in agricultural fields in Ademeyti, Lemlem, and Mentebteb was 43.8%, 31.0%, and 31.4%, respectively (Table 3).Table 3
Parous rates ofP. orientalis females trapped using CDC light traps, May 2011 to April 2012.
Villages
Habitat type
Number of dissected
Peridomestic
Number of dissected
Agricultural field
Number of parous (%)
Number of parous (%)
Ademeyti
180
60 (33.3)
144
63 (43.8)
Lemlem
197
61 (30.9)
200
62 (31.0)
Mentebteb
40
21 (52.5)
86
27 (31.4)
Total
417
142 (34.1)
430
153 (35.6)


### 3.2. Natural Infection Rates with Promastigotes

Among the 921P. orientalis females dissected for parasite detection, one female (0.11%) was found infected withLeishmania promastigotes. The infected specimen was collected from agricultural field in Lemlem village during July. However, none of the other seven species ofPhlebotomus was found infected withLeishmania promastigote. The number of dissected female sand flies includes 34P. lesleyae (1 from peridomestic and 33 from agricultural fields), 16P. bergeroti (12 from peridomestic and 4 from agricultural field), 6P. papatasi (5 from peridomestic and 1 from agricultural field), 4P. rodhaini (all from agriculture field), 3P. duboscqi (all from peridomestic), 5P. martini (2 from the peridomestic and 3 from agricultural field), and 2P. heischi (all from agricultural field).


### 3.3.Leishmania DNA Detection in Sand Flies

In total, 575P. orientalis females, which were divided into 115 pools, were submitted to ITS1-PCR testing forLeishmania. Five pools were observed to possess the characteristic DNA band ofLeishmania spp. However, acceptable sequence could not be obtained during DNA sequencing due to the weak amplification of theLeishmania DNA. Moreover, 200 blood-engorged sand flies (198P. orientalis, 1P. bergeroti, and 1Sergentomyia africana) were analyzed.Leishmania DNA was detected by PCR in 22 female specimens (11.0%). In the direct sequencing of the 22 PCR products, only three specimens produced a complete genomic sequence ofL. donovani inP. orientalis,P. bergeroti, andS. africana females, respectively (Figure 1). Engorged specimen ofS. africana was accidentally included in the analysis.Figure 1
PCR ofLeishmania internal transcribed spacer 1 (ITS1) region amplified from female sand flies. M: 100 bp size marker; −ve: negative control; +ve: referenceLeishmania spp.; Lanes 1 and 2:L. donovani DNAs inP. orientalis andP. bergeroti females, respectively; Lane 3:L. donovani inS. africana; Lane 4:Leishmania DNA inP. orientalis, but failed to be sequenced.


## 3.1. Abdominal Status and Parous Rates

Tables1 and 2 show the abdominal categories of differentPhlebotomus spp. collected from the study villages. In Ademeyti, the number of unfed, freshly fed, half-gravid, and gravidP. orientalis females from peridomestic habitat was 180, 163, 17, and 2, respectively (Table 1). Similarly, more numbers of unfed (n=197) and engorged (n=133)P. orientalis were found in peridomestic biotopes of Lemlem village. Of the 60 females ofP. orientalis obtained from Mentebteb, 40 were unfed, 17 freshly fed, and 3 gravid and half-gravid.Table 1
Abdominal status of femalePhlebotomus spp. captured from peridomestic sites in three different villages, May 2011 to April 2012.
Species
Number of dissected
Number of  unfed
Number of freshly fed
Number of half-gravid
Number of gravid
Total
Adm.
Lem.
Men.
Adm.
Lem.
Men.
Adm.
Lem.
Men.
Adm.
Lem.
Men.
Adm.
Lem.
Men.
P. orientalis
362
334
60
180
197
40
163
133
17
17
2
1
2
2
2
756
P. bergeroti
3
10
1
1
3
0
2
0
0
1
2
0
1
3
1
14
P. martini
0
0
2
0
0
0
0
0
0
0
0
0
2
0
0
2
P. papatasi
2
3
0
2
3
0
0
0
0
0
0
0
0
0
0
5
P. duboscqi
2
1
0
2
1
0
0
0
0
0
0
0
0
0
0
3
P. lesleyae
1
0
0
1
0
0
0
0
0
0
0
0
0
0
0
1
Total
370
348
63
186
204
40
165
133
17
18
4
1
5
5
3
781
Adm: Ademeyti; Lem: Lemlem; Men: Mentebteb.Table 2
Abdominal status of femalePhlebotomus spp. collected from agricultural fields in three different villages, May 2011 to April 2012.
Species
Number of dissected
Number of  unfed
Number of freshly fed
Number of half-gravid
Number of gravid
Total
Adm.
Lem.
Men.
Adm.
Lem.
Men.
Adm.
Lem.
Men.
Adm.
Lem.
Men.
Adm.
Lem.
Men.
P. orientalis
173
264
87
144
200
86
24
24
0
0
31
1
5
9
0
524
P. bergeroti
0
2
2
0
1
1
0
0
0
0
0
0
0
1
1
4
P. martini
2
1
0
1
0
0
0
0
0
1
1
0
0
0
0
3
P. rodhaini
1
3
0
1
3
0
0
0
0
0
0
0
0
0
0
4
P. papatasi
0
1
0
0
1
0
0
0
0
0
0
0
0
0
0
1
P. duboscqi
0
0
0
0
0
0
0
0
0
0
0
0
0
0
0
0
P. lesleyae
2
31
0
2
31
0
0
0
0
0
0
0
0
0
0
33
P. heischi
0
2
0
0
2
0
0
0
0
0
0
0
0
0
0
2
Total
178
304
89
148
238
87
24
24
0
1
32
1
5
10
1
571
Adm: Ademeyti; Lem: Lemlem; Men: Mentebteb.Of the total 524 females ofP. orientalis dissected from agricultural fields, 430, 48, 32, and 14 were unfed, freshly fed, half-gravid, and gravid females, respectively (Table 2). Less numbers of blood-fed females were caught in agricultural fields of Ademeyti and Lemlem villages. Likewise, no blood-fed females were detected in agricultural fields of Mentebteb. However, more numbers of (n=32) half-gravid females were recorded in Lemlem than the two villages.In total, 847 unfedP. orientalis were dissected and examined for parous state based on the appearance of accessory glands and condition of ovaries (Table 3). Of 417P. orientalis dissected in peridomestic biotopes, 142 (34.1%) were parous: 33.3%, 30.9%, and 52.5% in Ademeyti, Lemlem, and Mentebteb villages, respectively, while the parous rate in agricultural fields in Ademeyti, Lemlem, and Mentebteb was 43.8%, 31.0%, and 31.4%, respectively (Table 3).Table 3
Parous rates ofP. orientalis females trapped using CDC light traps, May 2011 to April 2012.
Villages
Habitat type
Number of dissected
Peridomestic
Number of dissected
Agricultural field
Number of parous (%)
Number of parous (%)
Ademeyti
180
60 (33.3)
144
63 (43.8)
Lemlem
197
61 (30.9)
200
62 (31.0)
Mentebteb
40
21 (52.5)
86
27 (31.4)
Total
417
142 (34.1)
430
153 (35.6)


## 3.2. Natural Infection Rates with Promastigotes

Among the 921P. orientalis females dissected for parasite detection, one female (0.11%) was found infected withLeishmania promastigotes. The infected specimen was collected from agricultural field in Lemlem village during July. However, none of the other seven species ofPhlebotomus was found infected withLeishmania promastigote. The number of dissected female sand flies includes 34P. lesleyae (1 from peridomestic and 33 from agricultural fields), 16P. bergeroti (12 from peridomestic and 4 from agricultural field), 6P. papatasi (5 from peridomestic and 1 from agricultural field), 4P. rodhaini (all from agriculture field), 3P. duboscqi (all from peridomestic), 5P. martini (2 from the peridomestic and 3 from agricultural field), and 2P. heischi (all from agricultural field).


## 3.3.Leishmania DNA Detection in Sand Flies

In total, 575P. orientalis females, which were divided into 115 pools, were submitted to ITS1-PCR testing forLeishmania. Five pools were observed to possess the characteristic DNA band ofLeishmania spp. However, acceptable sequence could not be obtained during DNA sequencing due to the weak amplification of theLeishmania DNA. Moreover, 200 blood-engorged sand flies (198P. orientalis, 1P. bergeroti, and 1Sergentomyia africana) were analyzed.Leishmania DNA was detected by PCR in 22 female specimens (11.0%). In the direct sequencing of the 22 PCR products, only three specimens produced a complete genomic sequence ofL. donovani inP. orientalis,P. bergeroti, andS. africana females, respectively (Figure 1). Engorged specimen ofS. africana was accidentally included in the analysis.Figure 1
PCR ofLeishmania internal transcribed spacer 1 (ITS1) region amplified from female sand flies. M: 100 bp size marker; −ve: negative control; +ve: referenceLeishmania spp.; Lanes 1 and 2:L. donovani DNAs inP. orientalis andP. bergeroti females, respectively; Lane 3:L. donovani inS. africana; Lane 4:Leishmania DNA inP. orientalis, but failed to be sequenced.


## 4. Discussion

Visceral leishmaniasis is affecting several people in various endemic areas of north and northwest Ethiopia. In particular, in this study area, 14.3% (680/4,757) of individuals were found positive forLeishmania k-DNA by real-time- (RT-) PCR [9]. In addition, 209 VL and 3 post-kala-azar dermal leishmaniasis (PKDL) cases were identified in the district in five years (2006–2011) [30].Parous rates ofP. orientalisdissected from peridomestic (34.1%) and agricultural field habitats (35.4%) were relatively low, which is comparable with those observed for the same species in Addis Zemen [31] and the Humera-Metema low lands [20], northern Ethiopia, and forP. martini in Aba Roba, southern Ethiopia [13]. The relatively small percentage of parous flies caught during the study period could indicate that females are short-lived and that few survive long enough to obtain more than one blood meal during their lives. This could also partly explain why low infection rate was detected inP. orientalis. Regarding the abdominal status ofP. orientalis, large numbers of blood-fed females were sampled in peridomestic habitats of the study villages compared with agricultural fields. This higher proportion of engorged females in this habitat is largely associated with the accessibility of large numbers of blood meal sources to questing females ofP. orientalis [32, 33]. On the other hand, relatively moderate numbers of half-gravid and gravid females were collected in agricultural fields, suggesting that older populations of the fly tend to remain in their breeding/resting sites until full development of ovules [34].Incrimination of a certain type of sand fly vector ofLeishmania species involves a number of criteria that include abundance in a leishmaniasis focus, high feeding habits on human, or reservoir host if the disease is zoonotic, demonstration of natural infections, and the ability to harbor, develop, and transmit theLeishmania parasite to a susceptible host [22, 35, 36]. Quite often, however, fulfilling all these criteria is exceedingly difficult [22, 36, 37].Usually, a sand fly species is suspected as a vector when it is predominant and proved to have anthropophilic behavior. In this area,P. orientalis was found to be the preponderant (98%) and human bitingPhlebotomus species [23]. Importantly, this sand fly species has already been incriminated as a vector ofL. donovani in the adjacent endemic regions of Sudan [14, 21, 38] and in the Lower Omo plains of south Ethiopia [18]. The present study also detectedLeishmania DNA by PCR in 20 blood-fed and 5 pools of unfedP.orientalis females. Specifically, one specimen ofP. orientalis was positive forL. donovani after sequencing, although it was in a recently engorged female. In addition, PCR detection ofLeishmania DNA inP. orientalis without blood meal (i.e., parous) is also suggestive, though sequencing of the PCR product failed to determine the exact identity of the parasites. Likewise,Leishmania promastigotes were detected in one specimen (1/921) ofP. orientalis female dissected, resulting in 0.11% natural infection. The promastigotes were observed in the abdominal and thoracic midgut of the fly but with low density. Despite the positive sample yielding a characteristic DNA band ofLeishmania in the PCR test, direct sequencing of this PCR product failed to give complete genomic sequence.A definitive substantiation can also be drawn from the results of earlier xenodiagnosis experiment, which was carried out to demonstrate the role of asymptomatic VL persons infectious toP. orientalis sand flies in the area (Gebre-Michael and Hailu, unpublished). In that xenodiagnosis study, laboratory bred females ofP. orientalis from the study area were allowed to feed on a VL-HIV coinfected patient and females were positive for promastigotes after 6-7 days of feeding. As well, the promastigotes were observed flourishing in the midgut with anterior migration to the foregut.In addition, engorged females ofP. bergeroti andS. africana, collected from Lemlem village in peridomestic habitat during January, were positive forL. donovani DNA.P. bergeroti bites human readily and has been suspected as a vector ofL. major in the Sahara [39] and around Mecca in Saudi Arabia [40]. DifferentSergentomyia spp. were found to be PCR positive for DNA of human pathogenicLeishmania species:L. major DNA was found inS. darling in Mali [17] andS. sintoni in Iran [41] whileL. donovani DNA was detected inS. babu in the Indian VL foci [42]. However, these infections were observed by PCR methods that have no ability of discerning mature from nonmature infection. Therefore, the observations might not necessarily reflect their involvement in the transmission of the parasites to humans sinceSergentomyia spp. do not support successful development of mammalianLeishmania in their guts, albeit they can be found to be PCR positive for DNA of human pathogenicLeishmania species [43, 44].


## 5. Conclusions

In conclusion, the predominant abundance ofP.orientalis and its attraction and blood feeding habits on humans and the detection ofL. donovani andLeishmania spp. in wild-caught females ofP.orientalis coupled with earlier results of xenodiagnosis on a patient strongly suggest thatP.orientalis is responsible for the maintenance ofL. donovani in Tahtay Adiyabo district. Other species (e.g.,P. martini andP. rodhaini) are probably involved as secondary vectors, although they are scarce in abundance. The former is the proven vector of VL in southern Ethiopia [13] while the latter was implied as possible vector in Sudan [45]. The results presented in this paper provided baseline information on primary and suspected vectors of VL in an active focus of this disease in northern Ethiopia. These findings could be used in epidemiologic studies and strategic planning for the control of VL in the region. Further studies should be conducted to reveal the exact infection rates ofP. orientalis in the current study area and other VL endemic foci in north Ethiopia.



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*Source: 710528-2015-07-29.xml*