Skip to main content

Therapeutic effects of Lucilia sericata larval excretion/secretion products on Leishmania major under in vitro and in vivo conditions



Leishmaniasis is a neglected infectious disease caused by protozoa of the genus Leishmania. The disease generally manifests as characteristic skin lesions which require lengthy treatment with antimonial drugs that are often associated with adverse side effects. Therefore, a number of studies have focused on natural compounds as promising drugs for its treatment. This study aimed to evaluate the effects of larval excretion/secretion products (ES) of Lucilia sericata in crude and fractionated forms on Leishmania major, by using in vitro and in vivo models.


The in vitro experiments involved evaluation of ES on both promastigotes and macrophage-engulfed amastigotes, whereas the in vivo experiments included comparative treatments of skin lesions in L. major-infected mice with Eucerin-formulated ES and Glucantime.


The half maximal inhibitory concentrations of the crude ES, > 10-kDa ES fraction, < 10-kDa ES fraction, and Glucantime were 38.7 μg/ml, 47.6 μg/ml, 63.3 μg/ml, and 29.1 μg/ml, respectively. Significant differences were observed between percentage viabilities of promastigotes treated with the crude ES and its fractions compared with the negative control (P < 0.0001). The crude ES was more effective on amastigotes than the two ES fractions at 300 μg/ml. The macroscopic measurements revealed that the reduction of lesion size in mice treated with the crude ES followed quicker cascades of healing than that of mice treated with Glucantime and the ES fractions.


The present study showed that the larval ES of L. sericata in both crude and fractionated forms are effective for both intracellular and extracellular forms of L. major. Also, the ES exert both topical and systemic effects on mice experimentally infected with L. major.

Graphical abstract


Leishmaniasis is a neglected tropical disease caused by protozoa of the genus Leishmania (Trypanosomatida: Trypanosomatidae) [1, 2]. It is estimated that approximately 350 million people who live in areas endemic for leishmaniasis are at risk of various forms of this disease [3]. About 20 species of Leishmania are known to be capable of infecting humans and a range of other animals. In humans, the parasite causes one of three clinical forms: visceral leishmaniasis (VL), cutaneous leishmaniasis (CL), and mucosal CL (MCL) [4]. The disease is mainly transmitted by bites of infected female sand flies belonging to the genera Phlebotomus and Lutzomyia, which occur in the Old World and the New World, respectively [5].

CL is the most common form of the disease, and causes disfiguring skin lesions with lifelong scarring [6]. Globally, leishmaniasis is responsible for a great number of disability-adjusted life years and large economic losses each year [7]. In endemic areas, the abundance of sand fly vectors, the high cost of drugs, prolonged treatments, and drug resistance are among the most serious setbacks for the control of this disease [8, 9]. In addition to the side effects of medications, the post-treatment scars of CL may be stigmatizing, especially for children [10]. Since the 1940s, pentavalent antimonial compounds such as Glucantime and Pentostam have been used as first-line drugs for the treatment of leishmaniasis [11]. Pentamidine, amphotericin B and paromomycin constitute the next choice of drugs, though the first two are contraindicated in pregnancy [12]. In Iran, antileishmanial therapy is currently based on the use of Glucantime ampoules [13]. With prolonged use, antileishmanial drugs can lead to clinical complications such as cardiac arrhythmia and anemia, and even toxicity and renal failure [11, 14, 15]. Given these problematics, alternative therapies have recently been suggested for CL treatment. These include the use of insect-derived natural compounds such as maggot-derived products, which have shown to have wound-healing effects [16, 17].

Maggot debridement therapy (MDT) has been widely used in the treatment of chronic wounds. MDT has been successfully used to treat necrotizing fasciitis; perianal gangrene; surgical wounds; burns; and venous, arterial and diabetic foot ulcers [18, 19]. The maggots of Lucilia sericata (Diptera: Calliphoridae) are usually used for MDT [20, 21]. These maggots exert a combination of wound debridement and disinfection as well as accelerated wound healing by secreting various enzymes such as proteases and nucleases, antimicrobial peptides and small active molecules [17, 22, 23]. Since its emergence 20 years ago, MDT has been increasingly recognized as a promising alternative therapy for wound healing which not only results in efficient wound debridement but also reduces the risk of post-surgery infections [18, 24, 25]. MDT has received approval as a medical device in many countries, including the USA (US Food and Drug Administration, 2004, case number K033391) [26].

The larval excretion/secretion products (ES) of L. sericata exhibit antimicrobial activity against both gram-positive and gram-negative bacteria [25, 27], as well as against protozoan agents of CL [28, 29]. In the present study, the effects of the crude and fractionated ES of L. sericata were comparatively investigated against Leishmania major using both in vitro and in vivo models. Also, in an attempt to find an alternative treatment for CL ulcers, the ES was formulated and tested against skin lesions of L. major-infected mice.


Collection and rearing of L. sericata

Wild adults of L. sericata were collected using bottle traps baited with raw chicken wing and liver in suburban areas of Saqqez City, Kurdistan Province, Iran between May and July 2020. The adult flies were anaesthetized with cold shock and morphologically identified using morphological keys [30, 31]. The fly colony was reared in mesh cages (60 × 60 × 60 cm) at the insectarium of the Medical Entomology Department of Tarbiat Modares University under the following conditions: 25 ± 1 °C, 60 ± 5% relative humidity and 16:8 h light/dark cycles [29]. Milk powder and sugar water solution (1:1 ratio) were supplied to feed the adults. Egg harvesting was performed by placing 150- to 200-g pieces of fresh beef liver in the rearing cage for 24 h as the oviposition substrates [32].

Larval ES preparation and sterilization

About 100 stage II and III larvae of L. sericata were collected from established colonies. The larvae were starved for 6 h before being washed with 0.5% sodium hypochlorite followed by 5% formaldehyde and finally rinsed twice with sterile saline solution in a 50-ml Falcon tube for 5 min [33]. Subsequently, 1 ml of saline solution was added to the confined larvae and the tube was covered with aluminum foil and incubated at 37 °C for 1 h [33]. The larval ES were then collected by pipetting and centrifuged at 4000 g for 10 min [34].

Bradford assay for protein measurement

A Bradford assay kit was used as a quick and ready-to-use colorimetric method for measuring the total protein content of the ES. The amount of protein in the solution was measured using a standard curve based on a serial dilution of known bovine serum albumin concentrations (0, 31.25, 62.5, 125, 250, 500, 1000 μg/ml). The protein samples were assayed using 8-well plates (SPL, Korea). The plates were incubated at 25 °C for 10 min in a dark place. Subsequently, optical absorption was read using an ELISA reader (model 680; Bio-Rad, Munich, Germany) at a wavelength of 595 nm [35].

Fractionation of larval ES

The separation of the > 10-kDa ES and < 10-kDa ES fractions was achieved by centrifugation at 7500 g for 40 min using an Amicon Ultra-4 Centrifugal Filter Unit. The isolated fractions and the crude ES were filtered through a 0.22-µm syringe filter for sterilization. The sterilized ES was tested on blood agar medium to ensure that it was free of bacterial contamination. The ES were kept at − 20 °C until use.

Larval ES protein profile determined by sodium dodecyl sulfate–polyacrylamide gel electrophoresis

The protein patterns of the ES samples of L. sericata were analyzed by electrophoresis on a 1-mm-thick 12.5% Tris–glycine sodium dodecyl sulfate–polyacrylamide gel. To this end, constant-current electrophoresis was performed at 110 V using Mini-PROTEAN 3 (Bio-Rad). After electrophoresis, the gels were stained with a solution containing Coomassie brilliant blue G250 and methanol. The mass-separated protein profiles were visualized against a pre-stained protein ladder (PAGEmark, 786-418) to estimate the molecular weights of the protein fractions.

Leishmania major culture conditions

Leishmania major strain MRHO/IR/75/ER was maintained by regular passage through BALB/c mice. The amastigotes were isolated from spleens of infected BALB/c mice and developed into promastigotes on Novy-MacNeal-Nicolle medium. The logarithmic phase promastigotes at 2 × 106 cells/ml were inoculated into Roswell Park Memorial Institute 1640 medium (Gibco, USA) supplemented with 10% heat-inactivated fetal bovine serum (FBS; Gibco) and 100 μg/ml penicillin–streptomycin (Thermo Fisher Scientific, USA). The promastigotes were grown in 25-ml cell culture flasks (Jet Biofil) and incubated at 26 °C until they reached the desired growth phase.

Cell line culture

The mouse macrophage cell line (J774A.1) was obtained from the Pasteur Institute of Iran (Tehran). The macrophages were cultured in Dulbecco’s modified Eagle medium (Gibco) supplemented with 10% heat-inactivated FBS (Gibco) and 100 μg/ml penicillin–streptomycin (Thermo Fisher Scientific) at 37 °C in a humidified 5% CO2 incubator. The macrophages were grown in cell culture flasks (Jet Biofil).

Promastigote survival assay

Logarithmic-phase promastigotes of L. major were cultured in Roswell Park Memorial Institute (RPMI) culture medium supplemented with 20% FBS in 96-well plates (SPL) at a concentration of 1 × 106 cells/ml. A serial dilution was prepared from the crude and fractionated ES at initial concentrations of 350 µg/ml using RPMI 1640 medium. The ES dilutions were used to treat promastigotes aliquoted into 96-well plates. The negative control consisted of promastigotes cultured in the same medium without any ES treatment. The test plates were incubated at 26 °C and done in triplicate. The effects of ES dilutions on the survival of promastigotes were assessed by determining the multiplication of the promastigotes after 24, 48 and 72 h of incubation using a hemocytometer (Neubauer chamber) [36].

ES cytotoxicity to macrophages determined by 3-(4.5-dimethylthiazol-2-yl)-2,5-diphenyltetrazolium bromide assay

The macrophages (J774A.1 cell line) were cultured in Dulbecco’s modified Eagle medium containing 10% FBS at 37 °C under a 5% CO2 atmosphere [37]. The macrophages at a concentration of 105 cells/ml were aliquoted into each well of a 96-well plate (SPL). The larval ES of L. sericata and Glucantime were then added to the plates at various concentrations [negative control (0), 25, 50, 100, 150, 200, 250, 300 and 350 μg/ml]. The loaded plates were incubated at 37 °C for 72 h before 20 μl 3-(4.5-dimethylthiazol-2-yl)-2,5-diphenyltetrazolium bromide was added to each well. The plates were again incubated at 37 °C for 5 h. Finally, the supernatant was drained and replaced by 100 μl of dimethyl sulfoxide per well. After 15 min, the absorbance was read at 570 nm using an ELISA reader (model 680; Bio-Rad). The selectivity was calculated using the following formula: selectivity index = 50% cell cytotoxicity/inhibitory concentration for 50% of the parasites (half maximal inhibitory concentration; IC50).

Amastigote susceptibility to larval ES

Twelve-well plates (SPL) were seeded with macrophages at a concentration of 2 × 10cells/ml after a sterile coverslip (cover glass) had been placed on the bottom of each well. The plates were incubated at 37 °C for 24 h to allow the cells to adhere to the coverslips. The macrophages were then infected with L. major promastigotes (stationary phase) at 10:1 parasite:macrophage ratio and further incubated at 37 °C for 24 h. Next, free promastigotes were washed out with phosphate buffered saline and the adhered infected macrophages were exposed to a series of concentrations of (i) crude ES (150–300 μg/ml), (ii) > 10-kDa ES (150–300 μg/ml), (iii) < 10-kDa ES (150–300 μg/ml), and (iv) Glucantime (50–100 μg/ml). The tested concentrations were determined based on IC50 values obtained in the earlier promastigote survival assay. The tests were performed in triplicate. The 5th group of plates, the negative control, received no treatment. After 72 h of incubation, the coverslips inside the wells were fixed with methanol, stained with 10% Giemsa and examined using light microscopy. The number of infected macrophages and the average number of parasites per macrophage were counted per 100 cells [36].

Development of ulcers

Thirty female BALB/c mice (4–6 weeks old) were obtained from Razi Vaccine and Serum Research Institute (Karaj, Iran). The mice were divided into six groups, each consisting of five animals. Each group was kept in a separate cage in the stress-free animal house of Tarbiat Modares University and fed ad libitum. The stationary-phase promastigotes are more resistant, active and efficient cells. They are obtained when the parasite population ceases growth. This is determined by daily sampling and counting of promastigotes. The inocula were injected subcutaneously into mice at the base of the tail. Injections were performed by insulin syringe under aseptic conditions under a laminar air flow cabinet. CL lesion development was monitored on a weekly basis until ulceration in the 5th week post-inoculation, after which the treatments were applied. Lesions were measured before and after treatments and their size used as an indication of wound-healing effect. The weekly measurements of the lesions were continued for a further 4 weeks.

ES preparations for the treatment of ulcers

To obtain formulated ointments to treat the lesions of the infected mice, Eucerin was added to each of the crude ES and their fractions at a ratio of 1:1. The concentration of the ES fractions used as treatments was 300 μg/ml. The ointments formulated with the crude ES, the ES fraction > 10 kDa and the ES fraction < 10 kDa were used to treat the 1st, 2nd and 3rd groups of infected mice, respectively. As a positive control, the 4th group was treated with subcutaneous injection of Glucantime around the lesion (60 mg/kg per day for 28 days) and the 5th group was left without treatment as a negative control. Finally, the 6th group was treated with pure Eucerin to evaluate its possible impact on lesion healing. All the materials were freshly prepared before application.

Parasite load evaluation

Eight weeks after treatment of the lesions, two mice from each of the six groups were sacrificed to determine the number of live L. major parasites in their infected spleens using the parasite-limiting dilution assay. For this purpose, 30 mg of spleen tissue was used to prepare a serial dilution of 1–10−15 of the parasite before being cultured in a 96-well plate containing complete medium enriched with 20% FBS, and streptomycin at 100 μg/ml [38]. The plates were then incubated at 26 °C for 10–14 days. Three replications were performed for each piece of mouse spleen, i.e. six replicates per group. Finally, the total number of positive wells (presence of motile promastigotes) and negative wells (absence of motile promastigotes) was identified under an inverted light microscope [39].

The following equation [40] was used to determine the parasite burden:

$${\text{parasite}}\,{\text{burden}} = - \log \,\left( {{\text{parasite}}\,{\text{dilution/spleen}}\,{\text{weight}}} \right)$$

Statistical analyses

The experimental results were analyzed by t-test and one-way ANOVA in GraphPad Prism version 6.07. To determine the independence of two categorical variables, χ2 and/or Fisher’s exact tests were also undertaken. The data are presented as means ± SD. Dose–response curves were drawn using non-linear regression. The area under the curve was used to estimate the larval ES effect against L. major promastigotes. The Bradford equation was applied through online software at ( and the graph was plotted using GraphPad Prism. Indices such as infection rate, decrease in infection rate, percentage viability, decrease in percentage viability, parasite load and survival index of amastigotes were determined using the equations presented in Rahimi et al. [41]. Differences were considered statistically significant at P < 0.05.


Bradford assay

A linear relationship was observed between protein concentration and absorbance at 595 nm (Fig. 1). This enabled the calculation of the corresponding linear equation and hence the protein concentrations of the ES samples. Given that the average net absorbance values at 595 nm for the crude ES, > 10-kDa ES and < 10-kDa ES were 1.69, 1.53 and 1.15, respectively, the average protein concentrations were 885.92, 731.80 and 366.71 μg/ml, respectively (Fig. 1). Therefore, the maximum protein concentration of ES samples used in this study was set at 350 μg/ml.

Fig. 1
figure 1

Bradford assay standard curve and the plotted excretion/secretion product (ES) sample concentrations. BSA Bovine serum albumin

Larval ES protein profiles

The electrophoretic protein patterns of larval ES of L. sericata are shown in Fig. 2. The protein bands indicate clear fractionation at a 10-kDa cut-off, with no or minimal loss of ingredients. The relatively high recovery of the ES samples, which only required mild processing, indicated that the methodology used was reliable for the production of ES fractions for use in bioassays against leishmanial cells. About 20–25 protein bands were observed for the crude ES, which matched bands in both the > 10-kDa and < 10-kDa fraction. This shows that the precision of the fractionation of the crude ES had an accuracy of almost 100% with no or only minor effects on the resulting protein profiles.

Fig. 2
figure 2

Sodium dodecyl sulfate–polyacrylamide gel electrophoresis patterns of ES protein profiles of Lucilia sericata larvae. L Pre-stained protein ladder (PAGEmark, 786–418), lane 1 crude ES, lane 2 > 10-kDa ES fraction, lane 3 < 10-kDa ES fraction

Sensitivity of promastigotes to ES

The IC50 values of the larval ES of L. sericata against promastigotes were evaluated at 24, 48 and 72 h. The lowest IC50 values for the crude ES, > 10-kDa ES and < 10-kDa ES were 38.70 μg/ml (log = 1.588), 47.61 μg/ml (log = 1.667) and 63.34 μg/ml (log = 1.802), respectively, at 72 h. The results were compared with those of Glucantime (Fig. 3). The area under each curve shows the corresponding number of parasites as a function of the drug concentration. These results support the data presented in Fig. 4. The percentage viabilities of the promastigotes exposed to different doses of the crude ES, > 10-kDa ES and < 10-kDa ES were significantly different than that of the negative control (P ≤ 0.001). While < 10-kDa ES was significantly less effective than Glucantime with respect to reducing promastigote viability (P = 0.001), no significant differences were observed between the percentage viabilities of promastigotes exposed to the crude ES and the > 10-kDa ES and those exposed to Glucantime at 72 h post-exposure (P = 0.841 and P = 0.860, respectively). It was obvious that higher concentrations of the ES fractions at longer exposure times were more toxic for promastigotes. Therefore, the toxic effect of ES was considered to be both dose and exposure time dependent (Fig. 4).

Fig. 3
figure 3

ad Dose–response curves of tested ES of Lucilia sericata larvae and Glucantime against Leishmania major promastigotes (half maximal inhibitory concentration; IC50) at 24 h, 48 h and 72 h. Area under the curve indicates the relationship between the number of parasites and the tested doses compared with the negative control. a Crude ES, b > 10-kDa ES, c < 10-kDa ES, d Glucantime

Fig. 4
figure 4

Number of Leishmania major promastigotes per milliliter upon exposure to different concentrations of the crude and fractionated ES compared with Glucantime at three time points (24, 48 and 72 h). Data are presented as means ± SD; means are significantly different at P < 0.05

ES cytotoxicity to macrophages

Figure 5 shows the cytotoxicity of various concentrations of ES fractions and Glucantime to macrophage cell line J774A.1 after 72 h of exposure. The ES fractions exerted similar, non-significantly different, mild effects on the percentage viability of macrophages. However, the crude ES was as toxic as Glucantime to macrophages, and there was no significant difference between their cytotoxicity (P = 0.340). The selectivity indices for the crude ES, > 10-kDa ES and < 10-kDa ES were 3.87, 2.79 and 1.58, respectively.

Fig. 5
figure 5

The number of viable J774A.1 cells treated with increasing doses of ES of Lucilia sericata larvae and Glucantime at 72 h of exposure. There were no significant differences between the treatments (P = 0.343)

Amastigote susceptibility to larval ES fractions

Table 1 indicates that infection rates of macrophages and the percentages of viable amastigotes inside them were considerably reduced at 72 h of exposure to larval ES fractions when compared with the control group (P = 0.001 and P = 0.001, respectively). The macrophage infection rates were reduced to a similar level by > 10-kDa ES and < 10-kDa ES (P = 0.476), though these treatments were significantly less effective than Glucantime (P = 0.015 and P = 0.007, respectively). However, crude ES and Glucantime were similarly effective in reducing macrophage infection rates, with no significant difference between them (P = 0.749) (Fig. 6). In addition, no significant difference was observed between the effect of > 10-kDa ES and that of the < 10-kDa ES (P = 0.290) in reducing the mean number of amastigotes per infected macrophage. Also, both ES fractions were significantly less effective than Glucantime (P = 0.029 and P = 0.01, respectively) in reducing the number of amastigotes per macrophage. However, crude ES and Glucantime exerted similar effects (P = 0.789). Treatment with crude ES at higher concentrations reduced the infection rate of macrophages and the viability of amastigotes (P = 0.036). Treatment with crude ES at 300 μg/ml lead to a significant reduction in the parasite loads of macrophages, equal to 1.75 ± 0.05 per cell, compared with the negative control. Treatment with Glucantime at 50 μg/ml also reduced parasite loads, to 1.96 ± 0.07 amastigotes per macrophage. The survival index of amastigotes was lowest, i.e. 53.72 ± 2.44, upon treatment with crude ES at 300 μg/ml (Table 1).

Table 1 Parameters indicative of Leishmania major amastigote viability and infectivity to J774A.1 in the crude ES, fractionated larval ES and Glucantime treatments
Fig. 6
figure 6

Reduction in infection rate and viability of amastigotes upon treatment with the crude ES, fractionated ES and Glucantime

Effect of larval ES fractions on leishmanial lesions

The skin lesions of all of the infected mice began with redness and swelling at the site of injection in the 3rd week post-inoculation. The swelling increased gradually, and lead to crust formation and the development of gangrene in the 4th week. The mean lesion measurements are presented in Table 2. The lesions of control mice increased progressively in size until the 4th week post-inoculation, where they reached a mean size of 12.8 ± 2.86 mm2. Likewise, the lesions increased in size in Eucerin-treated mice, and reached a mean size of 12 ± 1.87‌ mm2 over the same period. There was no statistically significant difference between the lesion sizes of control and Eucerin-treated mice (P = 0.782). This indicates that Eucerin has no therapeutic effect when applied on its own. In contrast, the lesions started to decrease gradually in size in mice treated with the crude ES. The mean lesion sizes were 2.6 ± 1.19 mm2 in the crude ES-treated group, 5 ± 2.35 mm2 in the > 10-kDa ES-treated group, 5.2 + 2.280 mm2 in the < 10-kDa ES-treated group and 2.2 ± 1.327 mm2 in the Glucantime-treated group. Although the crude ES and Glucantime were similarly effective in reducing the lesion sizes, with no significant difference between these treatments (P = 0.489), when lesion sizes in these treatments were compared with those in the > 10-kDa ES and < 10-kDa ES treatments, the differences were statistically significant (P < 0.001). In fact, the > 10-kDa ES and < 10-kDa ES treatments were similarly less effective against lesion development, and there was no significant difference between them with respect to reducing lesion sizes (P = 0.747) (Table 2).

Table 2 The effects of the crude ES and fractionated ES at 300 μg/ml on lesion size (mean ± SD) of Leishmania-infected mice versus positive and negative controls at different time points post-infection

After the termination of the treatment period, the measurement of the lesions was continued for several weeks to assess the possibility of a recurrence of inflammation. A slight increase in lesion size was observed in the case of the crude ES-treated (3.0 ± 2.55 mm2) and Glucantime-treated (2.6 ± 1.96 mm2) groups. In contrast, the wounds erupted upon the cessation of treatment in mice treated with > 10-kDa ES (6.6 ± 3.78 mm2) and < 10-kDa ES (7 ± 3.39 mm2) (Fig. 7).

Fig. 7
figure 7

Progression of leishmanial lesion size in treated and control BALB/c mice from pre-intervention stages until the 8th week post-treatment (differences are considered statistically significant at P < 0.05; ****P < 0.001)

Parasite loads

The parasite loads of the spleens of mice infected with L. major were determined using a parasite-limiting dilution assay. The parasite load was significantly lower in treated groups compared with the negative control group (P < 0.001). There was no significant difference between the latter group and the Eucerin-treated groups in parasite loads (P > 0.05). The crude ES-treated group had the lowest parasite load when compared with all the treated groups (P < 0.001) with the exception of the Glucantime-treated group (P = 0.267). As seen in the other comparisons, there was no statistically significant difference between the parasite loads of the groups treated with > 10-kDa ES and < 10-kDa ES (P = 0.059) (Fig. 8).

Fig. 8
figure 8

Parasitic loads of the spleens of mice infected with Leishmania major at 8th week post-treatment. Data are presented as means ± SD of triplicates (***P = 0.001, ns not significant)

Mice mortality during the study phases

The mortality of the experimental mice was monitored from the beginning of the treatments until 20 weeks post-treatment. Mortality in the negative control and Eucerin-treated mice occurred after the 7th week post-treatment and increased rapidly, so that all of the mice were dead by week 13 post-treatment. In contrast, mortality in the ES-treated mice did not change after week 14 post-treatment, so that more than 60% of these mice were still alive by the end of week 20. Mortality in the negative control and Eucerin-treated groups was similarly high, with no significant difference between them (P = 0.813). However, both of these groups differed significantly from the other treatment groups in their mortality rates (P < 0.001). The lowest mortality rates were observed in the crude ES-treated group and the Glucantime-treated group, with no significant difference between them (P = 0.239). By the end of week 20 post-inoculation, the survival rates of mice treated with > 10-kD ES and < 10-kDa ES were similar at 20%; although there was no significant difference between them (P = 0.346), they were significantly different from the survival rates of the crude ES and Glucantime-treated groups (P < 0.001) (Fig. 9).

Fig. 9
figure 9

Survival of treated and untreated mice over a period of 20 weeks post-infection with Leishmania major promastigotes (differences are significant at P < 0.05)


Leishmaniasis is a major health problem in tropical and subtropical regions of the world [29, 42]. Pentavalent antimonial compounds remain the first-line therapies for leishmaniasis, but entail painful injections and a long course of administration, have side effects, and are costly [43, 44]. Therefore, research has been devoted to finding cheaper and more effective drugs for leishmaniasis, especially among natural products, with minimum or no side effects [43]. Many studies have examined the cytotoxic effects of larval ES of various species of flies, including Lucilia sericata, against different Leishmania species, both under in vitro and in vivo conditions [29, 45, 46]. In the present study we evaluated the anti-leishmanial activity of the crude and fractionated ES of Lucilia sericata against promastigotes and amastigotes of Leishmania major, both under in vitro and in vivo conditions, using BALB/c mice as an animal model. In this study we also examined the cytotoxic effects of the ES against L. major promastigotes and macrophage cell line J774A.1. To the best of the our knowledge, this is the first comparative study of the effects of Lucilia sericata crude ES and its fractions on Leishmania major and macrophages.

In this study, the highest rates of cytotoxicity of the highly concentrated ES on the macrophages were 15%, 13% and 12% for > 10-kDa ES, < 10-kDa ES and the crude ES, respectively (Fig. 4). These results contrast with those of a study by Sanei-Dehkordi et al. [29] in which the cytotoxicity of L. sericata larval ES to the same macrophage cell line was reported to be 40%, although ambiguity regarding the exact concentration of their applied ES makes comparison difficult. However, testing L. sericata hemolymph and saliva on the same cell line, Rahimi et al. [41] reported lower toxicity to macrophages at a level comparable to that recorded in our study. Evaluating the effect of the ES derived from L. sericata and Sarconesiopsis magellanica on a human lung cell line (MRC5), Laverde-Paz et al. [47] showed that it had no effect on cell survival rates at a low concentration (10 μg/ml), but was effective in reducing cell survival rates at a higher concentration (20 μg/ml). The toxicity of an ES seems to be a function of various factors including insect species, rearing methods, ES concentration and storage conditions, as well as the types of exposed cells.

In our study, all larval ES of L. sericata were effective against promastigotes, but to various degrees. The crude ES was more lethal than the > 10-kDa ES and < 10-kDa ES fractions. These findings are consistent with those of other studies in which the effects of ES, hemolymph, and saliva of Lucilia sericata larvae were evaluated against Leishmania tropica both under in vivo and in vitro conditions [28, 41]. Similar results have been reported by other authors examining promastigote susceptibility to larval ES [48, 49].

The antibiotic properties of L. sericata-derived ES have been shown against fungi as well as gram-positive and gram-negative bacteria [50, 51]. ES fractions of L. sericata with molecular weights of < 1 kDa and 3–10 kDa have been shown to exert antibacterial activity against gram-positive and gram-negative bacteria including Pseudomonas aeruginosa, Klebsiella pneumoniae and Staphylococcus aureus [52]. The results of the present study showed that the ES fraction with a molecular weight of < 10 kDa had slightly lower anti-leishmanial activity than the ES fraction of higher molecular weight (> 10 kDa). However, the crude ES showed the highest toxicity to L. major, both under in vitro and in vivo conditions. Therefore, for an effective and strong anti-leishmanial activity, apparently all ES constituents, of different molecular weights, are required. This argument is supported by the results of the sodium dodecyl sulfate–polyacrylamide gel electrophoresis, which showed that the fractionation process caused no loss of proteins according to the protein profiles of the resulting ES fractions (Fig. 2).

An analysis of the susceptibility of intracellular amastigotes of Leishmania major to the ES of Lucilia sericata showed that the parasites are more vulnerable to the ES at high concentrations than at low concentrations. The ES significantly reduced the parasite’s survival rate. This finding contrasts with data reported in two studies [29, 48] which used Leishmania major and Leishmania panamensis amastigotes to infect the macrophage cell line J774 and U937 cell line, respectively. The authors postulated that the applied ES were more toxic at low concentrations than at high concentrations. In the present study, the lowest percentage viabilities of amastigotes were 20.6 ± 2.7 and 15.5 ± 1.1, following application of the crude ES (300 μg/ml) and Glucantime (100 μg/ml), respectively (Table 1; Fig. 5). The survival index values upon treatment with the crude ES were lower than those obtained with > 10-kDa ES and < 10-kDa ES in amastigote-infected macrophages (J774A.1). Also, a considerable reduction in the survival index was seen in the ES-treated cells compared with the control cells (Table 1). It is noteworthy that the anti-leishmanial effects of the crude ES and its fractions may be controlled by adjusting their concentrations [41, 53]. In the present study, the parasite load and survival index were both determined under in vitro and in vivo conditions. In both cases, the crude ES and Glucantime induced the lowest parasite loads. Also, significant decreases in parasite load and survival index were observed in groups treated with ES compared with the negative control groups (Table 1; Fig. 8).

In this study, lesions of BALB/c mice infected with L. major showed a significant reduction in size upon treatment with the crude ES and Glucantime, averaging 5 mm2 and 4.6 mm2, respectively (Table 2). The lesions treated with the crude ES, > 10-kDa ES and < 10-kDa ES were significantly smaller than those left untreated or treated with Eucerin (Fig. 7). Using Lucilia sericata maggots to directly treat the lesions of BALB/c mice infected with Leishmania major, Kabiri et al. [46] did not find any significant difference between the treated and untreated lesions. This indicates that the extracted ES of L. sericata larvae is more effective than the debridement activity of the larvae in healing leishmanial wounds. A study by Sanei-Dehkordi et al. [29] confirmed that ES extracts of Lucilia sericata and Calliphora vicina larvae were highly effective in reducing the size of lesions of BALB/c mice infected with Leishmania major when compared with the negative control. A similar result [28] also confirmed the effectiveness of larval ES of Lucilia sericata in healing the leishmanial ulcers of BALB/c mice infected with Leishmania tropica compared with the control group (P < 0.001). However, another study [33] showed that maggot therapy and the ES derived from Lucilia sericata and S. magellanica larvae were similarly effective in treating lesions caused by Leishmania panamensis in hamsters. The efficacy of L. sericata larval ES in reducing the development of the leishmanial lesions was attributed to its potency in skewing the monocyte-macrophage differentiation from pre-inflammatory to pro-angiogenic pathways [54].

Various studies have shown the potential therapeutic effects, under both in vitro and in vivo conditions, of the larval ES of different fly species on different species of Leishmania, including Leishmania amazonensis [55], Leishmania tropica [28], Leishmania major [29, 46], and Leishmania panamensis [33]. Here, we also clearly showed the anti-leishmanial activity of the larval ES of Lucilia sericata on the intracellular and extracellular forms of the parasite Leishmania major both under in vitro and in vivo conditions. We also provide evidence that the ES of larval L. sericata has both topical and systemic therapeutic effects on leishmanial lesions of the model animal used here.


To the best of our knowledge, this is the first report of the fractionation of the ES of larval L. sericata into two fractions of different molecular weight, > 10 kDa and < 10 kDa. Microscopic and macroscopic evaluation showed that both fractions are effective in the treatment of both intracellular and extracellular forms of the parasite L. major, although the > 10-kDa fraction was slightly more effective than the < 10-kDa fraction. However, the crude ES showed a higher antileishmanial activity than the fractionated ES. This study revealed that Lucilia sericata crude ES and its fractions are effective candidates for the treatment and cure of lesions induced by Leishmania major. However, the addition of suitable adjuvants may reinforce their effectiveness, and this deserves further study.

Availability of data and materials

The data supporting the conclusions of the present study are available from the corresponding author on reasonable request.



Cutaneous leishmaniasis


Excretion and secretion products


Fetal bovine serum

IC50 :

Half maximal inhibitory concentration


Maggot debridement therapy


Roswell Park Memorial Institute


  1. Akhoundi M, Kuhls K, Cannet A, Votýpka J, Marty P, Delaunay P, et al. A historical overview of the classification, evolution, and dispersion of Leishmania parasites and sand flies. PLoS Negl Trop Dis. 2016;10:e0004349.

    Article  PubMed  PubMed Central  CAS  Google Scholar 

  2. Barbosa JF, de Figueiredo SM, Monteiro FM, Rocha-Silva F, Gaciele-Melo C, Coelho SSC, et al. New approaches on leishmaniasis treatment and prevention: a review of recent patents. Recent Pat Endocr Metab Immune Drug Discov. 2015;9:90–102.

    Article  CAS  PubMed  Google Scholar 

  3. Desjeux P. The increase in risk factors for leishmaniasis worldwide. Trans R Soc Trop Med Hyg. 2001;95:239–43.

    Article  CAS  PubMed  Google Scholar 

  4. Herrera G, Hernández C, Ayala MS, Flórez C, Teherán AA, Ramírez JD. Evaluation of a multilocus sequence typing (MLST) scheme for Leishmania (Viannia) braziliensis and Leishmania (Viannia) panamensis in Colombia. Parasit Vectors. 2017;10:236.

    Article  PubMed  PubMed Central  CAS  Google Scholar 

  5. Monge-Maillo B, López-Vélez R. Therapeutic options for Old World cutaneous leishmaniasis and New World cutaneous and mucocutaneous leishmaniasis. Drugs. 2013;73:1889–920.

    Article  CAS  PubMed  Google Scholar 

  6. Khademvatan S, Salmanzadeh S, Foroutan-Rad M, Bigdeli S, Hedayati-Rad F, Saki J, et al. Spatial distribution and epidemiological features of cutaneous leishmaniasis in southwest of Iran. Alex J Med. 2017;53:93–8.

    Google Scholar 

  7. WHO. Control of the leishmaniases: key facts. 2020. Accessed 17 June 2020.

  8. Fazaeli A, Fouladi B, Sharifi I. Emergence of cutaneous leishmaniasis in a border area at south-east of Iran: an epidemiological survey. J Vector Borne Dis. 2009;46:36–42.

    CAS  PubMed  Google Scholar 

  9. Khajedaluee M, Yazdanpanah MJ, Seyed Nozadi S, Fata A, Juya MR, Masoudi MH, et al. Epidemiology of cutaneous leishmaniasis in population covered by Mashhad University of Medical Sciences in 2011. Med J Mashhad Univ Med Sci. 2014;57:647–54.

    Google Scholar 

  10. Al-Kamel MA. Impact of leishmaniasis in women: a practical review with an update on my ISD-supported initiative to combat leishmaniasis in Yemen (ELYP). Int J Women Dermatol. 2016;2:93–101.

    Article  Google Scholar 

  11. Singh N, Kumar M, Singh RK. Leishmaniasis: current status of available drugs and new potential drug targets. Asian Pac J Trop Med. 2012;5:485–97.

    Article  CAS  PubMed  Google Scholar 

  12. Tiuman TS, Santos AO, Ueda-Nakamura T, Dias Filho BP, Nakamura CV. Recent advances in leishmaniasis treatment. Int J Infect Dis. 2011;15:e525–32.

    Article  CAS  PubMed  Google Scholar 

  13. Bamorovat M, Sharifi I, Tavakoli Oliaee R, Jafarzadeh A, Khosravi A. Determinants of unresponsiveness to treatment in cutaneous leishmaniasis: a focus on anthroponotic form due to Leishmania tropica. Front Microbiol. 2021;12:638957.

    Article  PubMed  PubMed Central  Google Scholar 

  14. Ouellette M, Drummelsmith J, Papadopoulou B. Leishmaniasis: drugs in the clinic, resistance and new developments. Drug Resist Updat. 2004;7:257–66.

    Article  CAS  PubMed  Google Scholar 

  15. Omidian M, Jadbabaei M, Omidian E, Omidian Z. The effect of Nd:YAG laser therapy on cutaneous leishmaniasis compared to intralesional meglumine antimoniate. Postepy Dermatol Alergol. 2019;36:227–31.

    Article  PubMed  PubMed Central  Google Scholar 

  16. Macêdo CG, Fonseca MYN, Caldeira AD, Castro SP, Pacienza-Lima W, Borsodi MPG, et al. Leishmanicidal activity of Piper marginatum Jacq. from Santarém-PA against Leishmania amazonensis. Exp Parasitol. 2020;210:107847.

    Article  PubMed  CAS  Google Scholar 

  17. Sherman RA. Mechanisms of maggot-induced wound healing: what do we know, and where do we go from here? Evid Based Complement Alternat Med. 2014.

    Article  PubMed  PubMed Central  Google Scholar 

  18. Sherman RA. Maggot therapy for treating diabetic foot ulcers unresponsive to conventional therapy. Diabetes Care. 2003;26:446–51.

    Article  PubMed  Google Scholar 

  19. Zarchi K, Jemec GB. The efficacy of maggot debridement therapy–a review of comparative clinical trials. Int Wound J. 2012;9:469–77.

    Article  PubMed  PubMed Central  Google Scholar 

  20. Courtenay M, Church J, Ryan T. Larva therapy in wound management. J R Soc Med. 2000;93:72–4.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  21. Namias N, Varela EJ, Varas RP, Quintana O, Ward GC. Biodebridement: a case report of maggot therapy for limb salvage after fourth-degree burns. J Burn Care Res. 2000;21:254–7.

    Article  CAS  Google Scholar 

  22. Chambers L, Woodrow S, Brown A, Harris P, Phillips D, Hall M, et al. Degradation of extracellular matrix components by defined proteinases from the greenbottle larva Lucilia sericata used for the clinical debridement of non-healing wounds. Br J Dermatol Suppl. 2003;148:14–23.

    Article  CAS  Google Scholar 

  23. Valachova I, Majtan T, Takac P, Majtan J. Identification and characterisation of different proteases in Lucilia sericata medicinal maggots involved in maggot debridement therapy. J Appl Biomed. 2014;12:171–7.

    Article  Google Scholar 

  24. Sherman RA. Maggot versus conservative debridement therapy for the treatment of pressure ulcers. Wound Repair Regen. 2002;10:208–14.

    Article  PubMed  Google Scholar 

  25. Sherman RA, Sherman J, Gilead L, Lipo M, Mumcuoglu KY. Maggot debridement therapy in outpatients. Arch Phys Med Rehabil. 2001;82:1226–9.

    Article  CAS  PubMed  Google Scholar 

  26. Baumann A, Lehmann R, Beckert A, Vilcinskas A, Franta Z. Selection and evaluation of tissue specific reference genes in Lucilia sericata during an immune challenge. PLoS ONE. 2015;10:e0135093.

    Article  PubMed  PubMed Central  CAS  Google Scholar 

  27. Bexfield A, Bond AE, Roberts EC, Dudley E, Nigam Y, Thomas S, et al. The antibacterial activity against MRSA strains and other bacteria of a < 500 Da fraction from maggot excretions/secretions of Lucilia sericata (Diptera: Calliphoridae). Microbes Infect. 2008;10:325–33.

    Article  PubMed  Google Scholar 

  28. Polat E, Cakan H, Aslan M, Sirekbasan S, Kutlubay Z, Ipek T, et al. Detection of anti-leishmanial effect of the Lucilia sericata larval secretions in vitro and in vivo on Leishmania tropica: first work. Exp Parasitol. 2012;132:129–34.

    Article  PubMed  Google Scholar 

  29. Sanei-Dehkordi A, Khamesipour A, Akbarzadeh K, Akhavan AA, Mohammadi AMA, Mohammadi Y, et al. Anti Leishmania activity of Lucilia sericata and Calliphora vicina maggots in laboratory models. Exp Parasitol. 2016;170:59–65.

    Article  PubMed  Google Scholar 

  30. Crosskey R, Lane R. House-flies, blow-flies and their allies (Calyptratae: Diptera). Medical insects and arachnids: Springer; 1993. p. 403–28.

    Google Scholar 

  31. Williams KA, Villet MH. Morphological identification of Lucilia sericata, Lucilia cuprina and their hybrids (Diptera: Calliphoridae). ZooKeys. 2014;420:69–85.

    Article  Google Scholar 

  32. Gasz N, Harvey M. A new method for the production of sterile colonies of Lucilia sericata. Med Vet Entomol. 2017;31:299–305.

    Article  CAS  PubMed  Google Scholar 

  33. Cruz-Saavedra L, Díaz-Roa A, Gaona MA, Cruz ML, Ayala M, Cortés-Vecino JA, et al. The effect of Lucilia sericata- and Sarconesiopsis magellanica-derived larval therapy on Leishmania panamensis. Acta Trop. 2016;164:280–9.

    Article  PubMed  Google Scholar 

  34. Alnaimat SM, Wainwright M, Aladaileh SH. An initial in vitro investigation into the potential therapeutic use of Lucilia sericata maggot to control superficial fungal infections. Jordan J Biol Sci. 2013;6:137–42.

    Article  Google Scholar 

  35. Mehata AK, Dehari D. Bradford assay as a high-throughput bioanalytical screening method for conforming pathophysiological state of the animal. J Drug Deliv Ther. 2020;10:105–10.

    Article  CAS  Google Scholar 

  36. Varshosaz J, Arbabi B, Pestehchian N, Saberi S, Delavari M. Chitosan-titanium dioxide-Glucantime nanoassemblies effects on promastigote and amastigote of Leishmania major. Int J Biol Macromol. 2018;107:212–21.

    Article  CAS  PubMed  Google Scholar 

  37. Garcia AR, Amaral ACF, Azevedo MM, Corte-Real S, Lopes RC, Alviano CS, et al. Cytotoxicity and anti-Leishmania amazonensis activity of Citrus sinensis leaf extracts. Pharm Biol. 2017;55:1780–6.

    Article  PubMed  PubMed Central  Google Scholar 

  38. Abazari R, Mahjoub AR, Molaie S, Ghaffarifar F, Ghasemi E, Slawin AM, et al. The effect of different parameters under ultrasound irradiation for synthesis of new nanostructured Fe3O4@ bio-MOF as an efficient anti-leishmanial in vitro and in vivo conditions. Ultrason Sonochem. 2018;43:248–61.

    Article  CAS  PubMed  Google Scholar 

  39. Haghdoust S, Azizi M, Hoseini MHM, Bandehpour M, Masooleh MM, Yeganeh F. Parasite burden measurement in the Leishmania major infected mice by using the direct fluorescent microscopy, limiting dilution assay, and real-time PCR analysis. Iran J Parasitol. 2020;15:576–86.

    PubMed  PubMed Central  Google Scholar 

  40. Ghasemi E, Ghaffarifar F, Dalimi A, Sadraei J. In-vitro and in-vivo antileishmanial activity of a compound derived of platinum, oxaliplatin, against Leishmania major. Iran J Pharm Res. 2019;18:2028–41.

    CAS  PubMed  PubMed Central  Google Scholar 

  41. Rahimi S, Akhavan AA, Rafinejad J, Ahmadkhaniaha R, Bakhtiyari M, Veysi A, et al. The leishmanicidal effect of Lucilia sericata larval saliva and hemolymph on in vitro Leishmania tropica. Parasit Vectors. 2021;14:155.

    Article  PubMed  PubMed Central  Google Scholar 

  42. Postigo JAR. Leishmaniasis in the World Health Organization Eastern Mediterranean region. Int J Antimicrob Agents. 2010;36:S62–5.

    Article  CAS  PubMed  Google Scholar 

  43. Croft SL, Seifert K, Yardley V. Current scenario of drug development for leishmaniasis. Indian J Med Res. 2006;123:399–410.

    CAS  PubMed  Google Scholar 

  44. Karimipoursaryazdi A, Ghaffarifar F, Dalimi A, Dayer MS. In-vitro and in-vivo comparative effects of the spring- and autumn-harvested Artemisia aucheri Bioss extracts on Leishmania major. J Ethnopharmacol. 2020;257:112910.

    Article  CAS  PubMed  Google Scholar 

  45. Polat E, Kutlubay Z. Four cutaneous leishmaniosis case resistant to meglumine antimoniate treatment. Turk Parazitolojii Derg. 2014;38:177–80.

    Article  Google Scholar 

  46. Kabiri M, Dayer MS, Ghaffarifar F. Therapeutic effects of Lucilia sericata larvae on cutaneous leishmaniasis wounds caused by Leishmania major using BALB/c mice as animal model. J Kerman Univ Med Sci. 2017;24:389–96.

    Google Scholar 

  47. Pinilla YT, Patarroyo MA, Velandia ML, Segura NA, Bello FJ. The effects of Sarconesiopsis magellanica larvae (Diptera: Calliphoridae) excretions and secretions on fibroblasts. Acta Trop. 2015;142:26–33.

    Article  CAS  PubMed  Google Scholar 

  48. Laverde-Paz MJ, Echeverry MC, Patarroyo MA, Bello FJ. Evaluating the anti-Leishmania activity of Lucilia sericata and Sarconesiopsis magellanica blowfly larval excretions/secretions in an in vitro model. Acta Trop. 2018;177:44–50.

    Article  PubMed  Google Scholar 

  49. de Mello TF, Bitencourt HR, Pedroso RB, Aristides SM, Lonardoni MV, Silveira TG. Leishmanicidal activity of synthetic chalcones in Leishmania (Viannia) braziliensis. Exp Parasitol. 2014;136:27–34.

    Article  PubMed  CAS  Google Scholar 

  50. Barnes KM, Gennard DE, Dixon RA. An assessment of the antibacterial activity in larval excretion/secretion of four species of insects recorded in association with corpses, using Lucilia sericata Meigen as the marker species. Bull Entomol Res. 2010;100:635–40.

    Article  CAS  PubMed  Google Scholar 

  51. Hassan MI, Amer MS, Hammad KM, Zidan MM. Antimicrobial activity for excretion and secretion of the greenbottle fly larvae Lucilia Sericata (Meigen) (Diptera: Calliphoridae). J Egypt Soc Parasitol. 2016;46:179–84.

    PubMed  Google Scholar 

  52. Huberman L, Gollop N, Mumcuoglu K, Block C, Galun R. Antibacterial properties of whole body extracts and haemolymph of Lucilia sericata maggots. J Wound Care. 2007;16:123–7.

    Article  CAS  PubMed  Google Scholar 

  53. Tempone AG, de Oliveira CM, Berlinck RG. Current approaches to discover marine antileishmanial natural products. Planta Med. 2011;77:572–85.

    Article  CAS  PubMed  Google Scholar 

  54. van der Plas MJ, van Dissel JT, Nibbering PH. Maggot secretions skew monocyte-macrophage differentiation away from a pro-inflammatory to a pro-angiogenic type. PLoS ONE. 2009;4:e8071.

    Article  PubMed  PubMed Central  CAS  Google Scholar 

  55. Arrivillaga J, Rodríguez J, Oviedo M. Evaluación preliminar en un modelo animal de la terapia con larvas de Lucilia sericata para el tratamiento de la leishmaniasis cutánea. Biomedica. 2008;28:305–10.

    Article  PubMed  Google Scholar 

Download references


The authors would like to thank all the staff of the Department of Parasitology and Medical Entomology at Tarbiat Modares University.


This study was financially supported by Tarbiat Modares University (grant no. Med/8288).

Author information

Authors and Affiliations



All the authors were involved in all stages of the research—conceptualization, data analysis, investigation, and methodology—and also in the writing of the manuscript. All the authors read and approved the final manuscript.

Corresponding author

Correspondence to Mohammad Saaid Dayer.

Ethics declarations

Ethics approval and consent to participate

The experimental animal protocols were conducted according to the guidelines of the Experimental Animal Center of Tarbiat Modares University. The study was approved by the Ethics Committee of Tarbiat Modares University (approval no. IR.MODARES.REC.1399.124).

Consent for publication

All of the authors gave their full consent for the publication of this article.

Competing interests

The authors declare that they have no competing interests.

Additional information

Publisher's Note

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

Rights and permissions

Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons licence, and indicate if changes were made. The images or other third party material in this article are included in the article's Creative Commons licence, unless indicated otherwise in a credit line to the material. If material is not included in the article's Creative Commons licence and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this licence, visit The Creative Commons Public Domain Dedication waiver ( applies to the data made available in this article, unless otherwise stated in a credit line to the data.

Reprints and permissions

About this article

Check for updates. Verify currency and authenticity via CrossMark

Cite this article

Sherafati, J., Dayer, M.S. & Ghaffarifar, F. Therapeutic effects of Lucilia sericata larval excretion/secretion products on Leishmania major under in vitro and in vivo conditions. Parasites Vectors 15, 212 (2022).

Download citation

  • Received:

  • Accepted:

  • Published:

  • DOI: