Introduction
A wound is known as an injury occurs to a part of the body due to an accidental damage or a surgical procedure, especially one in which a skin breakage is observed [
1,
2]. Wounds include delayed acute wounds and chronic wounds, which regularly enter a state of pathologic inflammation as a result of a postponed, incomplete, or impaired healing process. Most chronic wounds are ulcers that are linked with diabetes mellitus, venous stasis diseases, ischemia or pressure [
3]. The non-healing wounds affect about 3 to 6 million people in the United States resulting in enormous health care expenditures, with the total cost estimated at more than US $3 billion per year [
4,
5]. Chronic wounds are also a significant health care problem in Australia, affecting more than half a million patients a day and the treatment costing more than AUD 3.5 billion per year [
6]. Ulcers secondary to peripheral vascular disease and diabetes mellitus are a major problem particularly in the aging population. In Sri Lanka, wound infections are rampant and it is one of the major health burden especially the chronic wounds [
7]. The chronicity of these wounds increases the risk of bacterial colonization and infection, hindering tissue healing which in most cases, eventually leads to amputations or life-threatening infection [
6]. It provides an entry point for systemic infections [
8]. As such, proper wound care as well as timely treatment of infections is vital.
Wound healing is a specific process of regeneration of the injured connective tissue of wounds leading to the restoration of injured tissues [
9,
10]. It is evident that the chronic wound is prevalent in 4.5 per 1000 life quality by the currently available treatments in geriatric population [
11] as well as cutaneous wound are frequent in diabetic’s patients [
12,
13]. Wound dressings loaded with antimicrobial agents have gathered much attention in recent times as an avenue for preventing and treating wound infections [
14]. Common antibacterial dressings that have shown benefits in wound healing contain silver compounds such as silver nitrate and silver sulfadiazine, however silver-containing products may cause tissue toxicity [
15]. Given the diminishing efficacy of currently used topical wound healing agents against many skin pathogens such
Methicillin Resistant Staphylococcus aureus (MRSA)-inflicted wounds [
16], new topical wound healing regimens are much needed. A topical treatment with no significant harmful effect on fibroblast proliferation and wound healing can reduce bacterial burden and lead towards better control of inflammation, wound malodor and purulent secretions.
Although there has been an enormous development in the pharmaceutical drug industry, wound healing drugs are not still satisfactory because of their low availability, high cost, and various detrimental side effects [
17]. Therefore, natural products-based drugs derived from medicinal plants and marine natural products are in demand in many developing countries that are rich in herbal traditions due to a common belief that they are safe, reliable, clinically effective, low cost, globally competitive and better tolerated by patients [
18,
19]. Natural products would be also useful as therapeutic agent for prevention of wound infections [
20]. However, marine natural products including seaweeds and seagrass remain less explored for medicinal applications especially in treating wounds. It is likely that these species are producing diverse secondary metabolites with novel chemical structures, which can be easily manipulated and developed as novel wound-healing drug candidates. There is an enormity of biodiversity within the Sri Lankan marine flora, some of them used in ethnomedicines which remains relatively undiscovered.
Seaweeds are used as functional foods and medicinal herbs in Asian countries [
21]. A variety of biological activities are attributed to seaweeds including neuroprotection, anti-tumor, anti-cancer, antioxidant, anti-obesity, anti-inflammatory, and anti-microbial and other biological activities [
22]. Biologically active compounds of these plants/marine flora include tannins, triterpenoids, and alkaloids and these chemicals have been found to affect one or more phases of wound healing process [
17]. Alkaloids in particular are known to possess exciting biological activities including antibacterial, anti-inflammatory and anti-Alzheime’s disease [
23]. Although there are a large number of studies conducted to investigate wound healing activity of different types of terrestrial plant extracts, there is inadequate data on seaweeds.
Herbal preparations thereof have been used to accelerate wound healing since ancient times [
24]. The use of these substances is often based only on tradition, without any scientific evidence of their efficacy and with little understanding of the mechanism of action of putative active compounds [
25]. The brown seaweed
S. ilicifolium is reported to exhibit several biological properties that are beneficial to human health, such as anticancer, antimicrobial, anti-inflammatory, and anti-diabetic properties [
26,
27]. In vitro study suggests that
S. ilicifolium stimulates fibroblast migration and proliferation to heal skin wounds [
28]. Furthermore, in vivo studies as well as in vitro studies have demonstrated the immunomodulatory properties of
S. ilicifolium. Specially antioxidant-mediated mechanisms activate the immune system to enhance the host's defense [
29]. Using streptozotocin-induced diabetic mice, alginate extract from
S. ilicifolium was found to be effective in re-epithelializing wound areas, increasing neutrophils, macrophages, fibroblasts, and fibrocytes, as well as collagen density [
30]. Previous research study showed, aqueous extracts of
S. ilicifolium showed no toxic effects on mice [
31]. An in vitro and in vivo study found that aqueous extracts of
S. ilicifolium have better healing effects than control groups [
32], but no detailed study seems to have been conducted. The objective of this study was to determine wound healing of
S. ilicifolium extracts by using rabbit models, and the wound healing evidence was supported by hematological and histopathological data. However, the active compound in this study was reported.
S. ilicifolium wound healing activity was evaluated using an in vivo model using more precise methods for evaluation. Our previous in vitro study on
S. ilicifolium extracts using scratch wound healing assay on the L929 cells, showed high rate of cell proliferation and migration. Guided by this preliminary data, in this study, we have investigated the wound healing properties of
S. ilicifolium extracts using in vitro and in vivo wound-repair model and highlighted its potential therapeutic applications.
Materials and Methods
Seaweed material
Fresh brown seaweed,
S. ilicifolium was collected from the southern coastal algae beds at Ahangama, in Sri Lanka [
33]. The collected brown seaweed sample was authenticated at the “National Herbarium of Peradeniya Botanical Garden” and a voucher specimen of
S. ilicifolium (Specimen number; SW23/B7) was deposited for future application. Fresh seaweeds were washed thoroughly with tap water, followed by washing with seawater on site to remove all sand particles, impurities, and epiphytes. Finally, the purified seaweeds were washed with distilled water prior to extracts preparation.
S. ilicifolium sample was dried to remove water, at 40 °C for four days until a constant weight obtained. Then, it was ground with an electric grinder (Herbal Grinder CS-700, China) to obtain 0.5 mm particle size powder and stored at -20 ºC. Then CE preparation was conducted using modified method of Premarathna et al., 2019 [
28]. The seaweed powder (100 g) was mixed with 500 mL distilled water and was kept for 1 h at 40 ºC in an ultrasound sonicator (Branson 2510, Danbury, USA) to soak and permit full extraction of bioactive compounds of
S. ilicifolium into aqueous medium. Then, the soaked seaweed sample was shaken in a tube roller mixer (Denley-spiramix 5, UK) at room temperature. Followed by three days of soaking the preparation was filtered by using a nylon mesh (0.50 μm) to collect CE of
S. ilicifolium. Finally, the extract was kept in the refrigerator at 4 ºC in a sealed container prior to use the in vivo experiments. Then CE was centrifuged for 10 min at 8000 rpm. After that, the supernatant was filter sterilized through a 0.2 μm filter and used for In vitro study.
Characterization of algal crude extracts
The FTIR spectra of extracts of S. illicilolum material were recorded using the iS50 (Nicolet) Fourier infrared spectrophotometer (Thermo Fisher Scientific, Waltham, MA, USA). The spectra were scanned at room temperature in absorption mode in the wavelength of 400 - 4000 cm-1, with the Omnic software version 9.2.
Nuclear magnetic resonance (NMR) spectroscopy
NMR samples were prepared by dissolving the sonicated extract material from S. illicilolum (1.5%) and commercially available D-mannitol (98%, Sigma-Aldrich) in D2O containing 10mM sodium trimethylsilylpropanesulfonate (DSS) as the internal standard. NMR spectra were recorded on Agilent DD500 NMR spectrometer operating at 500 MHz proton resonance frequency. For 1H spectra, 32 transients utilizing 90° pulse, 3 s acquisition time, and 25 s relaxation delay were acquired. Samples were analyzed at 25 °C and the chemical shift was referenced to DSS signal at 0 ppm.
In vitro assays
Cell culture
Human Dermal Fibroblast (HDF, Catalog 106-05a: purchased from Cell Applications, Inc.), RAW 264.7 and Human Epidermal Keratinocyte line (HaCaT, purchased from ATCC) cells were maintained in Dulbecco’s Modified Eagle’s medium (DMEM) supplemented with 10% (v/v) heat-inactivated fetal bovine serum (FBS, Sigma-Aldrich) and 1% penicillin/streptomycin. Cell cultures were maintained at 37 °C in a humidified 5% CO2 incubator atmosphere.
Cell viability on HDF, RAW 264.7 and HaCaT
HDF, RAW 264.7 and HaCaT cells were seeded onto 96-well plates (Corning Glasswork, Corning, NY) at a concentration of 2 x 104 cells/well followed by the addition of CE extracts (ten separate concentrations between 16 μg/μL and 0.02 μg/μL) prepared in cell culture media. A two-fold dilution series were used and eight replicates in each concentration. Negative and positive control tests were also prepared using Milli-Q water and 70% ethanol, respectively. Then contents were removed after 24 h and washed by PBS. 10 µL of MTT (5 mg/mL in PBS) solution and 90 µL DMEM culture media were added and further incubated for 4 h at 37 °C. Next, MTT solution was removed and 100 µL DMSO (dimethyl sulfoxide, spectrophotometric grade) was added. Finally, absorbance was measured using OPTIMA microplate reader (FLUOstar, UK) at the wave lengths of 540 nm. All experiments were triplicated.
Cell proliferation
In order to determine cell proliferation in the presence of CE extracts on HDF, RAW 264.7 and HaCaT cell lines, alamarBlue assay was conducted as described [
34]. Cells were grown in DMEM supplemented with 10% FBS to a final cell density of 2 × 10
4 cells/well and plates were incubated for approximately at 37 °C for 24 h with 5% CO
2. Extracts were two-fold serial diluted (16 μg/μL to 0.02 μg/μL) into supplemented media using a separate 96-well plate, applied to the cells, and incubated for different time interval (24 and 48 h) at 37 °C with 5% CO
2 and examined and photographed periodically. Next, 10 μL alamarBlue regent and 90 μL culture media were mixed and directly added to the wells. Following 4 h incubation, the experimental results were collected using the OPTIMA microplate reader (FLUOstar, UK) at 540 nm. The growth rates were compared to the growth of the negative and positive control.
Scratch wound healing assay
Cell migration of CE extracts on cells were determine by method of Premarathna et al. 2020. [
35] HaCaT cells were seeded (1 × 10
5 cells/well) into a 48-well tissue culture plate and incubated at 37 °C with 5% CO
2 until 90% confluent. Cell layer was scratched with a sterile yellow pipette tip (200 μL) across the center of the well and were washed with PBS to remove the debris/detached cells. Then, DMEM medium (150 µL) and CE extracts (150 μL, 0.02 μg/μL) were added to each well photographed and scratch wound closure analyzed (Carl Zeiss Microscopy GmbH software) during time interval at 0, 24 and 48 h.
Anti-inflammatory activity
Anti-inflammatory activity of S. illicilolum extract was observed through nitric oxide (NO) inhibition level in RAW 264.7 cells. Cells were firstly seeded at a density of 1 × 106 cells/well in a 96-microwell plate overnight in a humidified atmosphere (CO2 5%, 37 °C). Subsequently, cells were treated by S. illicilolum extract at 4 µg/µL concentrations and incubated at 37 °C for 24 h. Then S. illicilolum extract was discarded from 96 well plate. Further this plate was washed with phosphate buffer saline (PBS) to remove test solution. Consequently, NO assay was performed according to the manufacture protocol by using nitrite assay kit (Griess reagent, Sigma-aldrich). Accordingly, the amount of accumulated nitrite was used as an indicator of NO production in the cells. Finally, the absorbance was measured at 540 nm using a OPTIMA microplate reader (FLUOstar, UK). The standard calibration curve was also prepared using according to the kit protocol.
Phagocytosis activity
The phagocytic ability of macrophage (RAW 264.7) was measured by neutral red uptake assay [
36]. RAW 264.7 cells (1 × 10
5 cells/well) were treated with a series of concentrations of
S. illicilolum extract (16 - 0.02 μg/μL) in the culture medium at 37 °C and Lipopolysaccharide (LPS) (25 µg/mL) was used as positive control in 96-well plates. After 24 h incubation, the medium was removed, and 50 µL of 0.1% neutral red dissolved in phosphate buffer (PBS) and 50 µL DMEM culture media were added to each well and incubated for 24 h. The cells were washed with PBS three times, and then 100 µL of 1% acetic acid (v/v) in 50% ethanol (v/v) was added to each well to extract the dye phagocytized by macrophages. The absorbance at 540 nm was measured using a OPTIMA microplate reader (FLUOstar, UK).
In vivo assay
Experimental animals
Fifteen, 8-week-old, female New Zealand rabbits weighing 1.6 - 2.2 kg were obtained from the Medical Research Institute in Sri Lanka (MRI). The animals were hold on temperature range 28 ± 2 °C, humidity level 65 ± 5%, and with a 12 h light/dark cycle and fed with a standard pellet diet and water ad-libitum. The study was conducted in accordance with relevant ARRIVE guidelines for reporting animal experiments. The rabbits were acclimatized for 7 days in the experimental site prior to the study. Then, the rabbits were randomly grouped and all the groups were starved for 12 h before the wound formation and seaweed administration. Bedding in the individual cages was covered by a small mesh net, changed daily and cages were kept clean to avoid infection of wounds.
Experimental design
Rabbits were randomly separated into five experimental groups (n=3) as follows and the treatment was done in all the cases:
Group I/Treatment I (TI): Wounds were created and orally treated with 100 mg/kg per day S. ilicifolium extract for 14 days.
Group II/Control (C): Wounds were created and not given any cream or drug treatment.
Group III/Treatment II (TII): Wounds were created and orally treated with 100 mg/kg per day S. ilicifolium extract for 21 days (Treatment were started before the induction of skin wounds).
Group IV/Treatment III (TIII): Without any wounds and orally treated with 100 mg/kg per day S. ilicifolium for 14 days.
Group V/Normal (N): Normal Rabbit; kept intact without any treatment and wounds.
The quantity of treatment given to the animals during the experimental time period was calculated with respect to the body weight of animals [
37]. Since our previous studies have proven that the CE of
S. ilicifolium does not possess any cytotoxic effect [
35], 100 mg/kg dose was used for the in vivo assay.
Wound creation
Excision skin wounds (10.40 ± 0.60 mm) were induced in groups I, II, and III. The animals were anesthetized by using ketamine Hydrochloride (ilium Ketamil™ 10% Injection is a dissociative anaesthetic for use singly or in combination with muscle relaxants or tranquilisers 50 mL/Vial, Troy Laboratories Pty Ltd; Australia, 10 mg/kg, IM) and xylazine (ilium Xylazil-100™ 2% is an analgesic, sedative and muscle relaxant injection 50 mL/Vial, Troy Laboratories Pty Ltd; Australia, 2 mg/kg, IM) [
38]. The animal was held in standard crouching position, and the mobile skin of flank was gently stretched and held by the fingers. At the first, hair of the test animals’ lower back was completely shaved (60 × 60 mm
2) and cleared. Following surgery, an outline of the template was traced on the skin using a punch biopsy (10 mm). The four-full thickness circular wounds were made by excising the skin, within the border of the template to the level of loose subcutaneous tissue, using scalpel blade and forceps. Disinfected wounds were washed with sterile saline and povidone-iodine (Win Medicare, India) immediately. All dressings and animal maintenance were in accordance with the ethical rules of standard surgery procedures.
Size and rate of wound contraction
The size and rate of contraction of wounds were photographed using the digital camera (Nikon Coolpix 4500: Nikon, Tokyo, Japan). Images were analyzed by computerized Carl Zeiss Microscopy GmbH software (Germany) and wound area was measured as the change in pixels. In order to determine the rate of wound healing, animals from both test groups and control groups were held in the standard crouching position. Measurement errors were minimized by repeating each measurement on three times and using an average of the measurements in calculations.
Wound healing percentage in N day = Wound area in the first day - Wound area during the Nth day/Wound area in the first day×100
Histopathological tissue analysis
The tissue samples were collected from the center of the wound and part of the tissue adjacent to the edges of the lesions on 5, 10, 15 and 20 days. The tissue sample from each group was subjected to epidermicrographs (biopsies) was placed in a fixative solution (10 % neutral- buffered formalin), tissue blocks were placed in formalin, dehydrated in a graded series of ethanol, embedded in paraffin, cut into 5 μm thick serial sections. Then the sections were stained with hematoxylin and eosin and examined for the healing process, to identify inflammatory cells, granulation tissue, and tissue structure. H & E grading was performed on the basis of the extent of distance cells migrated from the wound margin and for the analysis of fibroblasts and blood vessels [
39]. Van Gieson stain was performed in a differential staining of collagen and other connective tissue and highlight elastic fibers in particular [
40].
Biochemical analysis
Body weights and temperature of all rabbits were recorded once a week, including acclimatization week. Behavioral changes, food and water consumption of rabbit were recorded daily throughout the experimental period. Blood from these groups were collected on 0, 5, 10, 15 and 20 days. The serum enzyme levels of aspartate aminotransferase (AST) and alanine aminotransferase (ALT), and creatinine of serum separated from the collected blood samples [
41] using the spectrophotometer (Erba Mannheim, Model: chem- 7, Germany).
Hematological and serological parameters
Blood smears were prepared to evaluate the white blood cell differential count (WBC-DC) in all groups once a week. The WBC were counted under oil immersion (×100). Furthermore, the following tests were conducted: red blood cells (RBCs) and white blood cells (WBCs), total serum protein (TSP) and packed cell volume (PCV).
Statistical analysis
All statistical data analysis was performed using Graph Pad Prism Version 9.3.0 (San Diego, CA, USA) software. One-way and two-way analysis of variance was carried out for data analysis whereas Turkey’s method was used for multiple comparisons between the significant levels of interactions of the variables. Each point in the diagrams were shown the mean ± SEM, and differences were considered significant when p<0.05.
Discussion
Natural products including terrestrial and marine flora are rich in secondary metabolites that have unique structural orientations, which are easily malleable for drug development [
53]. The main categories of secondary metabolites derived from natural products and that have been developed into drugs are: terpenes (34%), glycosides (32%), polyketides and others (18 %) and alkaloids (16%) [
40]. An analysis of the origin of the drugs developed between 1981 and 2001 showed that 80% of 122 plant-derived drugs were discovered as a result of chemical studies directed at isolating the biologically active substances from the natural products used in traditional medicines [
54]. Between 2000 and 2005, about five medicinal natural products-based drugs including antimicrobial drugs were introduced in the United States market and another seven natural products-derived compounds are currently in clinical trials around the world [
55,
56]. Despite many natural products especially medicinal plants are used in traditional medicine for treating wounds, not much of them have been clinically tested as wound healing agents. Wound healing is a dynamic process involving a complex interplay of various cells, extracellular matrices, and soluble mediators [
57,
58]. The wound healing immediately begins after an injury to a smooth interaction among different types of tissues and cells [
59] and specific process leading to the restoration of injured tissues [
9]. This is followed by attraction and proliferation of fibroblast, which is the connective tissue cell responsible for collagen deposition that is needed to repair the tissue injury [
60]. Cell migration or proliferation is known to be involved in skin regeneration, granulation and wound healing [
61]. Recently, our laboratory developed an in vivo rabbit model to investigate a healing process and understand the wound healing ability of orally treated seaweed extracts. Initial findings observing the wound healing activity showed a reduced healing time. In this study, the
S. ilicifolium has significantly enhanced wound healing in rabbits and reduced the days needed for complete healing compared with the non-treated control groups. This could be due to an effect of several groups present in the seaweed extracts which may enhance some stage in the wound healing process. The wound healing activity of
S. ilicifolium treated rabbits has demonstrated significant healing effects when compared to the control group (P<0.05).
According to the histopathological findings, it is clear that the wound healing activity was significantly faster in the rabbit group (treatment I and II) treated orally with
S. ilicifolium CE than other wounded rabbit groups (treatment III and control). Enhanced wound healing activity could be attributed to increased collagen formation and angiogenesis [
32,
62]. Oral administration is non-painful, safest route and has immediately responded for the wound healing process. Tissue granulation in the wounded sites was significantly increased in the histopathological sections of the animals treated with
S. ilicifolium CE compared to the control. Furthermore, this group has exhibited an increased rate of epithelialization and wound contraction of wound. Wound contraction was evaluated by analyzing the change in diameter of the wound, to differentiate it from re-epithelialization. This study highlighted that re-epithelialization plays one of the major roles in wound healing activity when treated with
S. ilicifolium CE. It is worthwhile in future to determine the bioactive compound(s) of
S. ilicifolium or seaweeds.
Previous studies on its close relative - brown algae - showed that their main components are polysaccharides, which mainly consist of fucoidan, laminarin, cellulose, alginates, mannitol, algal fucans, galatians and alginates [
63]. Polysaccharides such as fucoidans are reported to have an effect on the traditional medicine for immunomodulatory and inflammatory [
64]. Natural products in general has been known to possess a strong potential for the treatment of skin wounds [
53,
65,
66]. The presence of complex halogenated and non-halogenated terpenoids [
67] in seaweeds may be responsible for their wound healing capacity. Since mannitol are reported to improve wound healing and protect tissues from oxidative damage [
68], it is likely that the mannitol-rich
S. ilicifolium extract is exerting the wound healing activity observed in this study.
This study demonstrated that an oral administration of
S. ilicifolium CE enhanced cutaneous healing of wound within first 12 days.
S. ilicifolium CE (100 mg/kg) did not show any significant toxicity effect on rabbits. Further, any significant effect on serum protein level and pack cell volume was also not reported compared to the wounded control group. Generally, body weight is considered as a sensitive indicator of experimental animals and the change in body weight is used to estimate the toxic effects of drugs for animals in toxicological studies [
69,
70]. Toxicity effect can be investigated on liver cells, which get damaged as a result of the introduction of infectious agents or chemicals, and as a result the serum levels of ALT and AST tend to increase significantly [
41,
71]. This was not observed in the present study. The serum enzymes such as ALT, AST, and creatinine were found to be within the normal range in the seaweed extract (
S.ilicifolum) treated groups (Group I, II and III) and without treatment of the control groups (Group IV and V). The toxicity result indicates that
S. ilicifolum seaweed extract is safe for human consumption.
According to the findings,
S. ilicifolium CE can be used as an immunostimulant for analysing macrophage-related inflammatory responses. Furthermore, these crude extractions may also be clinically useful in modifying macrophage function in diseases where it is impaired or needs to be enhanced. Due to the central role macrophages play in both innate and acquired immune responses, we investigated whether the combination of D-Mannitol and aromatic compounds obtained from
S. ilicifolium could modify the activity of RAW 264.7 murine macrophages in vitro.
S. ilicifolium CE can be produced by activated macrophages during inflammatory responses. The presence of NO in the body suggests that it is necessary for maintaining health. One of the most significant molecules for blood vessel health is NO, produced by nearly all types of cells in the human body [
72,
73]. In the present study,
S. ilicifolium CE stimulated the release of nitric oxide from RAW 264.7 macrophages. Inflammatory responses are regulated by NO, which has a wide range of biological activities. As well as enhancing physical performance and reducing muscle soreness, nitric oxide helps manage type 2 diabetes and erectile dysfunction [
74].
Wounds - particularly chronic wounds - are the major concerns for the patient and clinician alike. Research on wound healing agents is one of the developing areas in modern biomedical sciences. The seaweeds are used as medicines, especially in the Asian countries, where modern health services are limited [
28]. However, the mechanism of wound healing process remains unknown. In this study, oral administration of
S. ilicifolum has enhanced the rate of wound healing increase in collagen synthesis and tensile strength of the wound tissues. As we know in a moist environment, exudate provides the cells involved in wound repair with nutrients, controls infections, and provides the best environment for healing [
75]. Developing countries have to spend a large sum of money on importing drugs and machines used in wound healing treatment. Finding alternative, effective and less expensive methods for treatments of wound healing would bring immense benefits.
Acknowledgements
A special thanks to Miss. Krinsli Pius (Research Laboratory Manager) at the School of Natural Science and Health, Tallinn University, Estonia for her technical support. Support given by Miss. Sanjida Humayan is also appreciated. Special thanks to Professor Ruth Shimmo, Miss. Tiina Aavik and Dr. Sirje Vaask in School of Natural Sciences and Health, Tallinn University, Estonia. The authors wish to thank Mr. N.G.J Perera and Mr. K.L.M.S Bandara, staff of Animal House, Faculty of Medicine, University of Peradeniya, Sri Lanka. Technical support given by Mr. NAND Perera, Mr. K.B.A.T Bandara, Mr. W.M.D Wickramaarachchi, Mr. K.A Wijesekera and Mr. D.P.G.S.P Jayasinghe, Department of Veterinary Pathobiology, Faculty of Veterinary Medicine and Animal Science is appreciated.
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