Cloning and characterization of a novel sigma-like glutathione S-transferase from the giant panda parasitic nematode, Baylisascaris schroederi
- Yue Xie†1,
- Xuan Zhou†2,
- Lin Chen1,
- Zhihe Zhang3,
- Chengdong Wang4,
- Xiaobin Gu1,
- Tao Wang1,
- Xuerong Peng5 and
- Guangyou Yang1Email author
© Xie et al.; licensee BioMed Central. 2015
Received: 15 December 2014
Accepted: 29 December 2014
Published: 23 January 2015
Baylisascaris schroederi, an intestinal nematode of the giant panda, is the cause of the often fatal disease, baylisascariasis. Glutathione S-transferases (GSTs) are versatile enzymes that can affect parasite survival and parasite-host interactions and, are therefore, potential targets for the development of diagnostic tests and vaccines.
In this study, we identified a full-length cDNA that encoded a novel, secretory sigma-like GST (Bsc-GSTσ) from a B. schroederi-omic dataset. Following cloning and sequencing, sequence and structural analyses and comparative modeling were performed using online-bioinformatics and proteomics tools. The recombinant Bsc-GSTσ (rBsc-GSTσ) protein was prokaryotically expressed and then used to detect antigenicity and reactivity using immunoblotting assays. In addition, the native protein in female adult B. schroederi was located via immunofluorescence techniques, while the preliminary ELISA-based serodiagnostic potential of rBsc-GSTσ was assessed in native and infected mouse sera.
Bsc-GSTσ contained a 621-bp open reading frame that encoded a polypeptide of 206 amino acids with two typical sigma GST domain profiles, including a GST_N_Sigma_like at the N-terminus and a GST_C_Sigma_like at the C-terminus. The presence of an N-terminal signal sequence indicated that Bsc-GSTσ was a secretory protein. Sequence alignment and phylogenetic analyses showed that Bsc-GSTσ was a nematode-specific member of the Sigma class GSTs and shared the closest genetic distance with its homologue in Ascaris suum. Further comparative structure analyses indicated that Bsc-GSTσ possessed the essential structural motifs (e.g., βαβαββα) and the consensus secondary or tertiary structure that is typical for other characterized GSTσs. Immunolocalization revealed strong distributions of native Bsc-GSTσ in the body hypodermis, lateral chords, gut epithelium, gut microvilli, oviduct epithelium, and ovaries of adult female worms, similar to its homologue in A. suum. Building on good immunogenic properties, rBsc-GSTσ-based ELISA exhibited a sensitivity of 79.1% and a specificity of 82.0% to detect anti-B. schroederi IgG antibodies in the sera of experimentally infected mice.
This study presents a comprehensive demonstration of sequence and structural-based analysis of a new, secretory sigma-like GST from a nematode, and its good serodiagnostic performance suggests that rBsc-GSTσ has the potential to detect B. schroederi and, therefore, could be used to develop an ELISA-based serological test to diagnose baylisascariasis in giant pandas.
KeywordsBaylisascaris schroederi Giant panda Glutathione S-transferase Sigma class Bsc-GSTσ Immunolocalization Immunodiagnosis
The giant panda (Ailuropoda melanoleuca) is one of the world’s most iconic and endangered species, and is currently confined to several small mountain habitats of western China (Qinling, Minshan, Qionglai, Daxiangling, Xiaoxiangling, and Liangshan) with a population size of ~1600 [1,2]. Wild giant pandas face the threat of extinction from human population expansion, destruction of their habitat, and the detrimental impacts of parasites and other diseases [3,4]. Baylisascariasis, caused by the nematode, Baylisascaris schroederi (Nematoda: Ascaridida), is one of the leading causes of death for both wild and captive giant pandas and has been responsible for half of the recorded deaths of pandas from 2001 to 2005 [3,5]. As with other ascaridoids, adult B. schroederi usually inhabit the intestines of the giant panda, while the larvae may disseminate into various body tissues. In pandas, damage to bodily tissues includes extensive inflammation and scarring of the intestinal wall and parenchyma of the liver and lung (also known as visceral larval migran, VLM; caused by larvae), as well as intestinal obstruction, inflammation, and even death (caused by adults) [5-8]. Currently, diagnosis and identification of B. schroederi infection in pandas relies on morphological examination of fecal eggs, which requires extensive expertise and is difficult, laborious, and prone to error (as the density of eggs in bamboos-enriched feces is low and subject to possible environmental cross-contaminating with the eggs of other parasites, including morphologically similar Baylisascaris spp. ). Recently, a new molecular method to detect B. schroederi was developed based on the PCR-based detection of mitochondrial makers (COII or 12S) [9-11]. This method, however, cannot diagnose migrating larvae or adults outside of the egg-laying period. Hence, an alternative and more efficient molecular tool is needed. Serodiagnosis, particularly the ELISA tests (enzyme-linked immunosorbent assays) equipped with target molecules that play excretory/secretory (ES) roles and function in the survival, development, and immune evasion of parasites , would be an ideal and better strategy due to its sensitivity and clinical practices.
Glutathione S-transferases (GSTs; EC 220.127.116.11) are a versatile protein superfamily that are widely distributed among all living cells and act in cellular detoxification and protection via either catalyzing toxin conjugation with reduced glutathione (GSH) or passively binding to various exogenous/endogenous toxic molecules, including carcinogens, therapeutic agents, and products of oxidative stress [13,14]. For parasites, some secretory GSTs are further believed to be associated with parasite survival, repair of damage caused by host’s immune-initiated reactive oxygen species (ROS), transportation or metabolism of essential materials, and host immune modulation [12,14-19]. Encouragingly, because of these important functions, some parasite-derived GSTs, including those of parasitic nematodes, have been selectively targeted for vaccine development and diagnosis purposes [15,16,19-23]. For example, a secretory sigma-class GST from Ascaris lumbricoides (GSTA) has recently been identified and investigated as a new allergen for clinical diagnosis of the human roundworm disease , although the frequency of the antibody (mainly IgE) sensitization to GSTA is not high and the GSTA exhibits several isoforms with differential IgE recognition. Also, another secretory GST-3 from the human filarial nematode Onchocerca volvulus (OvGST3) is under investigation as a potential antigen candidate for the diagnosis of onchocerciasis due to its high exposure to the human host’s immune system and good immunogenic properties .
Given that most recently described nematode-derived GSTs are from the Sigma class in term of their sequence homology, structure, substrate specificity, immunological and phylogenetic analyses [20,22], and that no information on GSTs of B. schroederi is available to date; importantly, B. schroederi-specific immunogenic proteins as potential diagnostic agents are lacking, herein, the aims of this study were to (i) clone and express a new, secretory sigma-like GST, Bsc-GSTσ, from B. schroederi; (ii) characterize its potential functions by locating the native protein in adult parasites; and (iii) test the immunogenicity and preliminary ELISA-based diagnostic potential of its recombinant Bsc-GST (rBsc-GSTσ) in mice using native and infected sera. The results of this work will provide the foundation for the further development of Bsc-GST as a candidate serodiagnostic antigen to detect B. schroederi in the giant panda.
This study was reviewed and approved by the Animal Ethics Committee of Sichuan Agricultural University (AECSCAU; Approval No. 2011–028). Animals were handled strictly accordance with the animal protection law of the People’s Republic of China (released on 09/18/2009) and the National Standards for Laboratory Animals in China (executed on 05/1/2002).
Female specific-pathogen-free (SPF) BALB/c mice (6–8 weeks old) were purchased from the Laboratory Animal Center of Sichuan University (Chengdu, China). New Zealand white rabbits were obtained from the Laboratory Animal Center of Sichuan Agricultural University (Ya’an, China). All animals were housed under a barrier environment in sterile cages and provided with pelleted food and sterilized water ad libitum. Animals were acclimated to these conditions for one week prior to the experiment.
B. schroederi female adults derived from naturally infected giant pandas were provided by the Department of Parasitology, College of Veterinary Medicine, Sichuan Agricultural University. Adult female Ascaris suum and Baylisascaris transfuga were isolated from infected pigs at a local slaughterhouse in Ya’an and an infected polar bear after treatment with pyrantel pamoate in Chengdu zoological garden, China, respectively. Embryonated and/or un-embryonated eggs were obtained from the respective dissections of the uteruses of B. schroederi, B. transfuga, and A. suum using established procedures . The infective egg-L2 larvae of these three ascaridoids were collected from subsequent incubation of the embryonated eggs according to the USEPA and Tulane methods [26,27]. All L2-contained eggs were stored at 4°C until use.
RNA isolation, amplification and bioinformatic analysis of Bsc-GSTσ-1
Total RNA was isolated from an adult female specimen of B. schroederi using an RNA extraction kit (Clontech, Palo Alto, CA) according to the manufacturer’s directions. The isolated RNA was subsequently subjected to first-strand cDNA synthesis using a cDNA synthesis kit and an oligo (dT)18 primer (MBI Fermentas, Germany). The resulting double-stranded cDNA was used as the template for PCR amplification with the sense primer (5′-AAGCAACATGCCGCAGTACAAG-3′) and the antisense primer (5′-CACAAAAAACAGAATAGACCCTAATA-3′) designed to target a full-length coding sequence of the GST homologue that was screened from the assembled and annotated B. schroederi genome (Scaffold ID 47) and transcriptome (Unigene ID 86248) datasets (data unpublished). The amplified product was gel-purified, cloned into the pMD19-T vector (TaKaRa, Dalian, China) and then sequenced. After a homology search by BLASTn (http://blast.ncbi.nlm.nih.gov/Blast.cgi?PROGRAM=blastn&PAGE_TYPE=BlastSearch&LINK_LOC=blasthome), the cDNA showed similarity to known sigma GSTs and therefore was designated as Bsc-GSTσ. The open reading frame (ORF) and deduced amino acid sequence of Bsc-GSTσ were derived using an Open Reading Frame Finder and the Lasergene software package for Windows (DNASTAR, Madison, WI, USA) and then assessed with ExPASy online servers (http://www.expasy.org/). Conserved domains (CD) were identified using the CD-Database-based PROSITE profile analysis (http://www.ncbi.nlm.nih.gov/Structure/cdd/cdd.shtml). The isoelectric point (pI) and molecular weight (Mw) of Bsc-GSTσ were calculated using the Compute pI/Mw tool (http://web.expasy.org/compute_pi/) and the signal sequence was predicted with the SignalP 4.0 server (http://www.cbs.dtu.dk/services/SignalP/). Similarity comparisons with previously reported sequences were conducted using DNAMAN 3.0 (Lynnon Biosoft, Quebec, Canada) and online BLASTp tool (http://blast.ncbi.nlm.nih.gov/Blast.cgi?PROGRAM=blastp&PAGE_TYPE=BlastSearch&LINK_LOC=blasthome). On the basis of observed similarities, a multiple sequence alignment and phylogenetic analysis were conducted. Sequences were aligned with ClustalW2 and the phylogenetic tree was constructed using the neighbor-joining (NJ) method  and plotted with MEGA 5.0 . In addition, for structural modeling of Bsc-GSTσ, we used the YASPIN secondary structure prediction program (http://www.ibi.vu.nl/programs/yaspinwww/) to infer secondary structure. Tertiary (3D) structure was assessed through the CPHmodels-3.2 Server online program (http://www.cbs.dtu.dk/services/CPHmodels/) and by referring to the 1.90 Å resolution crystal structure of N. americanus GSTσ2 (PDB accession no.: 2ON5).
Expression and purification of rBsc-GSTσ
Due to the presence of the predicted signal peptide, a region encoding mature Bsc-GSTσ was amplified by PCR for expression using the following primers: 5′-CCCGGATCCATTCGTGGCCTGGGTG-3′ (forward; a BamHI site in italics) and 5′-CGCAAGCTTCACAAAAGCAGAAGAGACTCTAATA-3′ (reverse; a HindIII site in italics). After enzyme digestion with BamHI and HindIII (TaKaRa) and gel-purification, this fragment was ligated into the plasmid expression vector pET32a (+) (Novagen, Madison, USA). The correct resulting plasmid was confirmed by sequencing, transformed into E. coli BL21 (DE3) cells (Invitrogen, Carlsbad, USA), and then grown in Luria-Bertani (LB) broth with 100 mg/mL of ampicillin at 37°C until the optical density at 600 nm reached 0.6. Expression was induced by adding 1 mM isopropyl β-D-thiogalactopyranoside (IPTG) for an additional 4 h culture at 37°C. The cells were pelleted and suspended in lysis buffer [50 mM NaH2PO4 (pH 8.0), 10 mM Tris–HCl (pH 8.0), 100 mM NaCl]. The samples were subjected to sonication and centrifuging to enable collection of inclusion bodies and cellular debris and the removal of other soluble substances. His6-tagged recombinant Bsc-GSTσ proteins were expressed as inclusion bodies in the pellets after sodium dodecyl sulfate-polyacrylamide gel electrophoresis (SDS-PAGE) and then purified using Ni2+ affinity chromatography (Novagen) under denaturing conditions according to the manufacturer’s protocol. Refolding of the purified recombinant proteins was performed as recommended elsewhere . Thereafter, the refolded protein was concentrated using the vacuum freeze-drying technique and its concentration was determined with the micro-bicinchoninic acid protein assay reagent (Pierce/Thermo Fisher Scientific, Asheville, USA). Potential contamination by endotoxins was assessed using the limulus amoebocyte lysate-based gel-clot assay .
Mouse immune sera against parasites A. suum (15 samples), B. transfuga (15 samples) or B. schroederi (43 samples) were produced for serodiagnostic assays as previously described [8,31,32]. Rabbit anti-B. schroederi sera were generated as follows: 3,600 B. schroederi infective embryonated eggs were administered to one New Zealand white rabbit, followed by four repeat inoculations every 2 weeks. The rabbit was bled two weeks after the final inoculation and the serum was collected for immunoblotting analysis. To obtain mouse polyclonal sera against rBsc-GSTσ, 10 BALB/c mice were subcutaneously immunized with 50 μg of purified rBsc-GSTσ mixed with FCA (Sigma, St. Louis, USA), followed by two booster immunizations (two weeks apart) using the same route and dose in the same adjuvant. Mice were bled two weeks after the final immunization. The anti-rBsc-GSTσ sera were mixed and stored at −20°C until use. Additionally, 20 mouse native sera were provided by the Department of Parasitology, College of Veterinary Medicine, Sichuan Agricultural University.
Immunoblotting and immunolocalization
For immunoblotting analysis, rBsc-GSTσ was lysed in an electrophoresis sample buffer, run on 10% SDS-PAGE and subsequently transferred onto the nitrocellulose membrane. The blotting membrane was incubated with 5% skim milk in Tris-buffered saline (TBS) buffer for 1 h. To better test the antigenicity of rBsc-GSTσ, rabbit immune sera from animals repeatedly inoculated with B. schroederi embryonated infective eggs, anti-rBsc-GSTσ mice serum, and native rabbit or mouse serum were included here. After the membrane was washed three times with TBS-Tween 20 (TBST), it was further incubated for 2 h with 1:200 diluted alkaline phosphatase-conjugated goat anti-mouse or anti-rabbit IgG (ICN Pharmaceuticals, Costa Mesa, CA). Following the same washing steps described above, the protein signals were visualized using nitroblue tetrazolium and 5-bromo-4-chloro-3-in-dolylphosphate (NBT/BCIP; USB, Cleveland, OH) and recorded using Image Quant LAS-4000 (GE Healthcare Life Sciences, USA). For immunolocalization studies, adult female B. schroederi sections were probed with specific mouse anti-rBsc-GSTσ serum (1:100) and then with fluorescein isothiocyanate (FITC)-labeled goat anti-mouse IgG (1:100; Santa Cruz, CA, USA) as described elsewhere . The stained samples were mounted in glycerol/phosphate buffer (v/v, 9:1) and viewed under an Olympus BX50 fluorescence microscope (Olympus, Japan).
To assess the preliminary serodiagnostic potential of rBsc-GSTσ, B. schroederi-specific IgG antibodies of mice were detected by ELISA following the methodology described by Vlaminck et al. , with some modifications. In brief, ELISAs were performed in polystyrene 96-well microtiter plates (Invitrogen) using 100 μL reaction mixtures with rBsc-GSTσ antigen coated at three different concentrations (1, 2, and 4 μg/mL) in 0.1 M carbonate buffer (pH 9.6). After overnight incubation at 4°C, all plates were washed with PBS + 0.5% Tween 20 (PBST20) and then the wells were blocked with 100 μL of PBS-2% bovine serum albumin (BSA) for 2 h at 37°C. A serial two-fold dilutions (100 μL; ranging from 1:100 to 1:1600) of the positive serum sample (provided by our lab) and goat anti-mouse IgG-HRP conjugate (100 μL; 1:500) (Boster Bio-project Co., Wuhan, China) were used in the following steps, and positive sera and conjugates were diluted in PBS. Antibody binding was detected with 100 μL of O-phenylenediamine dihydrochloride substrate (0.4 mg/mL OPD, 50 mM dibasic sodiumphosphate, 25 mM citric acid, and 30% H2O2), and the optical density (OD) was measured at 492 nm. Negative and blank controls were included on each plate. After the best dilutions of rBsc-GSTσ antigen and mouse serum were determined, 93 mouse serum samples (43 for B. schroederi-positive, 30 for A. suum/B. transfuga-positive, and 20 for control) were serodiagnosed with the ELISA. The sensitivity of the assay was calculated as follows: sensitivity (%) = ELISA positive/true positive × 100, while the specificity was evaluated by the cross-reaction with the heterosera derived from mice infection with the congeneric species, B. transfuga, and the related ascaridoid, A. suum.
ELISA data were expressed as the mean value ± standard deviation (SD). Comparisons between test sera groups were carried out using one-way ANOVA in SPSS version 17.0 for Windows (SPSS Inc., Chicago, IL). P values <0.05 were considered to be significant. The negative cut-off was calculated as the mean value + 3× SD from the OD values of the normal sera, as previously described . Additionally, the nucleotide sequence determined in the present study was deposited in the GenBank database under accession number KM435257.
Molecular characterization of Bsc-GSTσ
Annotation of Bsc-GSTσ structural model
Phylogenetic characterization of Bsc-GSTσ
Expression, purification, and reactivity of rBsc-GSTσ
Immunolocalization of native Bsc-GSTσ in adult female B. schroederi
Diagnostic potential of rBsc-GSTσ protein
Detection of anti- B. schroederi IgG antibodies in serum samples of experimentally infected mice (N = sample size)
Sera of mice infected with parasites
r Bsc -GSTσ-ELISA
OD value (means ± SD)
No. of positive serum samples (%)
1.249 ± 0.0575
0.396 ± 0.5223
0.432 ± 0.5118
0.113 ± 0.0270
Baylisascariasis, caused by the parasite B. schroederi, is today recognized as a significant cause of mortality of giant pandas, yet the diagnostic tools to detect B. schroederi infections in pandas are still lacking [3,39-42]. Numerous studies have highlighted the importance of parasite GSTs, particularly secretory GSTs, in parasite survival and host immune regulation, and thus, as potential candidates for the development of vaccines or diagnostic tools [15,16,20-22,37]. With this in mind, in this study we identified and characterized a novel, secretory sigma-class GST from B. schroederi (Bsc-GSTσ) and assessed its potential for serodiagnosis in an experimentally challenged mouse model.
The ongoing annotations of the genome and transcriptome of B. schroederi (within our research group) provide a comprehensive bioinformatics platform for probing the accurate complete reference sequence to design primers to amplify and express Bsc-GSTσ. By means of the His fusion-based pET32a (+) prokaryotic vector system, a ~42 kDa recombinant Bsc-GSTσ protein was generated here. Excluding the tag peptides, this ~22-kDa Mw was well within the range of 21–29 kDa reported for other GSTs  and agreed with the findings of a previous review that the average molecular mass of sigma GSTs in parasites is 22 kDa . Further sequencing and structural analyses revealed that Bsc-GSTσ possessed the typical structural features of representatives of GSTs in the Sigma class: a coding domain for the GST_N_Sigma_like (PSSM: cd03039) and another for the GST_C_Sigma_like (PSSM: cd03192). Meanwhile, the signal peptide analysis implied that Bsc-GSTσ was a secretory protein. Previous studies have demonstrated that most parasite GSTs isolated to date, including some secretory GSTs, can be grouped independently of their host species into thirteen classes based on their sequence, structure, substrate specificity, and sensitivity to inhibitors (namely alpha, beta, kappa, delta, sigma, theta, mu, omega, pi, tau, zeta, psi, and epsilon) [13,44,45]. Combined, the results suggest that Bsc-GSTσ characterized here should be a secretory GST and is affiliated with the Sigma class.
Sequence alignment and phylogenetic analyses classified Bsc-GSTσ along with nematode-specific GSTσs, and it together with homologues of other nematodes and trematodes described to date formed a unique, major invertebrate subgroup and were distinct from those of the vertebrates in the Sigma class GSTs (Figure 4), which was consistent with a recently published report . Within the nematode-specific GSTσs, eight homologous proteins derived form six parasite species, including B. schroederi, were further subjected to pair comparisons on primary, second, and tertiary structure levels. Although Bsc-GSTσ was most similar to A. suum GSTσ at the amino acid level, the N-terminal seven GSH-binding moieties responsible for the G-site were highly conserved (100% identity) across all the nematode species included here. Similar conservations were also indicated by their higher (secondary or 3D) structures where a classical GSTσ βαβαββα motif was present in the N-terminal domain (see Figure 2) . In contrast with G-sit, the C-terminal substrate binding H-site seemed to be greatly variable. Studies confirm that the amino acid identity in the H-site of GSTs is usually very low, even between intra-class members (<35%) . This provides the opportunity to screen the region-specific sites for immune responses or to design drugs to inhibit the parasite enzyme only. Furthermore, the distinction of Bsc-GSTσ from its counterpart in giant pandas further enhances its potential as a diagnostic or therapeutic target due to impossible autoimmune responses caused by cross-reactivity. Under this context, we explored the antigenicity and reactivity of Bsc-GSTσ using its recombinant form. The results of our immunoblotting analysis showed that rBsc-GSTσ was strongly recognized by rabbit anti-B. schroederi serum and mouse anti-rBsc-GSTσ serum and became visible at 42 kDa. These findings confirm the strong immunogenicity of this compound and its potential as a diagnostic tool or candidate target for vaccine development. Two recent studies have successfully used recombinant GSTσ antigens in vaccines against human hookworm N. americanus (e.g., rNa-GST-1) [47,48] and liver fluke Fasciola hepatica (e.g., rFhGST-S1) . This work suggests that immunoprotective assays to determine the vaccine potential of this recombinant protein in B. schroederi are warranted. On the other hand, we characterized Bsc-GSTσ as a secretory antigen of B. schroederi. Previous studies have demonstrated the potential of parasite-specific E/S antigens in diagnostics [12,49-53], thus we thought it prudent to assess the potential of this compound in the serodiagnosis of B. schroederi infections in giant pandas. B. schroederi infections in wild pandas are not associated with specific clinical symptoms, and the infection can only be confirmed until worms are expelled or eggs are shed in the feces . The development of a serodiagnostic tool will enhance existing diagnostic methods and improve treatment options, especially during the larval migrating stages (L2-L4). After optimizing conditions, a rBsc-GSTσ-based ELISA was established in the present study. Our results revealed that rBsc-GSTσ could clearly detect the B. schroederi-specific IgG antibodies in experimental mouse sera, with a sensitivity of 79.1% and a specificity of 82.0%, although cross-reactions were observed in several B. transfuga- or A. suum-positive mouse sera. The presence of cross-reactions may be associated with a similar distribution of epitopes in the GSTσ homologues of the two ascaridoids that are closely related to B. schroederi. A similar phenomenon was also described between other parasitic nematodes (between Toxocara canis and A. suum and Toxascaris leonina , between Anisakis simplex and A. suum and Anisakis physeteris , and between Baylisascaris procyonis and Toxocara spp. ). The sensitivity of the assay was not high, and is likely a consequence of using a recombinant antigen for a serodiagnostic assay. Recombinant antigens are often produced as single proteins and lack the post-translational chemical or structural modifications present in its native counterpart, which can weaken their sensitivity. Interestingly, it has been shown that combining recombinant antigens can improve the sensitivities of recombinant antigens in the serodiagnosis of parasitic infections [56,57]. Nevertheless, it is important to note that the geographic range of giant pandas does not overlap with that of bears (the hosts for B. transfuga) or swine (the hosts for A. suum). Hence, the chance of cross-reactivity in the wild is low and the serodiagnostic ELISA developed here would be able to detect B. schroederi in pandas with a respectable sensitivity.
Finally, our localization analysis showed that native Bsc-GSTσ was present in the intestine, reproductive tissues, and body hypodermis of female adult B. schroederi. Within the intestine a strong immunofluorescent signal for Bsc-GSTσ was observed in the brush border of the microvilli, as has been reported for its homologue AsGST1 in A. suum . Surprisingly, this intestinal location was distinct from its homologue OvGST1 in the filaria O. volvulus: the endogenous OvGST1 was distributed in the hypodermis . This discrepancy may be associated with species-specific differences amongst nematodes. With respect to filarial nematodes, they are being considered to become specialized and adopt a blood-based or lymph-based nutrition parasitism, especially their intestines . As compensation for the degeneration or loss of intestinal function, the presence of OvGST1 in the hypodermis of O. volvulus is probably responsible for the metabolism of extrinsic materials and the excretion or secretion of molecules from the parasite, similar to that which occurs in the intestines [14,15]. This finding suggests that Bsc-GSTσ in B. schroederi and AsGST1 in A. suum may both be involved in metabolism and detoxification as well as nutrition during the development of ascaridoids. In addition, we also observed strong fluorescent signals of Bsc-GSTσ in the ovaries, oviduct epithelium and egg walls, but not in the muscles or ooplasm of B. schroederi. This contrasts to the results reported for their counterparts in A. suum . Whether the expression of this gene in these tissues is also nematode species-specific is not known, but the expression of GSTs in trematode parasites has been reported to be tissue-specific and developmentally regulated. For example, Sm26GST and Sm28GST in Schistosoma mansoni were located in the parenchymal cells of adults but were absent from the musculature, gut and reproductive tissues [60,61]. In F. hepatica, a more recent study showed that FhGST-S1 was present in the parasite tegument, parenchyma, musculature and eggs, and was also found in the excretory/secretory fraction of adults. Thus, the authors inferred that the FhGST-S1 of the adult fluke may play a role in parasite development and the interaction between host and parasite . Perhaps, with the advent of readily available genomic tools, the combination of high-throughput genome sequencing and mass spectrometry techniques for exploring pan-nematode proteomics will provide a comprehensive platform for an in-depth structure and function analyses of these GSTσs. This should contribute to a better understanding of the biological roles of nematode-specific GSTσs.
The full-length cDNA encoding a novel Sigma class glutathione S-transferases (Bsc-GSTσ) from B. schroederi was identified by screening the genome and trancriptome datasets and subsequently cloned and expressed. We determined some of the structural characteristics and tissue-specific distributions of this compound, providing insights into the biological functions of this protein. Furthermore, we showed that rBsc-GSTσ has strong immunogenicity and we confirmed via a serodiagnostic assay that rBsc-GSTσ is a suitable diagnostic antigen and could be used to develop an ELISA-based serological test for the diagnosis, seroepidemiology, and serosurveillance of B. schroederi in giant pandas.
This work was supported by the grant from the Research Fund for the Chengdu Giant Panda Breeding (No. CPF-2012-13). We would like to thank Mei Liu and Yu Wang (College of Veterinary Medicine, Sichuan Agricultural University, China) for technical assistance; Caiwu Li (Ya’an Bifengxia Research Base of Giant Panda Breeding, China) for materials.
- Wei F, Hu Y, Zhu L, Bruford MW, Zhan X, Zhang L. Black and white and read all over: the past, present and future of giant panda genetics. Mol Ecol. 2012;21:5660–74.PubMedView ArticleGoogle Scholar
- Yang B, Busch J, Zhang L, Ran J, Gu X, Zhang W, et al. Eco-compensation for giant panda habitat. Science. 2013;339:521.PubMedView ArticleGoogle Scholar
- Zhang JS, Daszak P, Huang HL, Yang GY, Kilpatrick AM, Zhang S. Parasite threat to panda conservation. Ecohealth. 2008;5:6–9.PubMedView ArticleGoogle Scholar
- Wildt DE, Zhang AJ, Zhang HM, Janssen DL, Ellis S. Giant Pandas: Biology,Veterinary Medicine and Management. Cambridge: Cambridge University Press; 2006.View ArticleGoogle Scholar
- Loeffler K, Montali RJ, Rideout BA. Diseases and pathology of giant pandas. In: Wildt DE, Zhang ZA, Zhang HM, Janssen DL, Ellis S, editors. Giant Pandas: Biology,Veterinary Medicine and Management, Cambridge. Cambridge: Cambridge University Press; 2006. p. 377–409.View ArticleGoogle Scholar
- Wang T, He G, Yang G, Fei Y, Zhang Z, Wang C, et al. Cloning, expression and evaluation of the efficacy of a recombinant Baylisascaris schroederi Bs-Ag3 antigen in mice. Vaccine. 2008;26:6919–24.PubMedView ArticleGoogle Scholar
- Lin Q, Li H, Gao M, Wang X, Ren W, Cong M, et al. Characterization of Baylisascaris schroederi from Qinling subspecies of giant panda in China by the first internal transcribed spacer (ITS-1) of nuclear ribosomal DNA. Parasitol Res. 2012;110:1297–303.PubMedView ArticleGoogle Scholar
- Xie Y, Chen S, Yan Y, Zhang Z, Li D, Yu H, et al. Potential of recombinant inorganic pyrophosphatase antigen as a new vaccine candidate against Baylisascaris schroederi in mice. Vet Res. 2013;44:90.PubMed CentralPubMedView ArticleGoogle Scholar
- Zhou X, Yu H, Wang N, Xie Y, Liang Y, Li D, et al. Molecular diagnosis of Baylisascaris schroederi infections in giant panda (Ailuropoda melanoleuca) feces using PCR. J Wildl Dis. 2013;49:1052–5.PubMedView ArticleGoogle Scholar
- Zhang W, Yie S, Yue B, Zhou J, An R, Yang J, et al. Determination of Baylisascaris schroederi infection in wild giant pandas by an accurate and sensitive PCR/CE-SSCP method. PLoS One. 2012;7:e41995.PubMed CentralPubMedView ArticleGoogle Scholar
- Wang N, Li D, Zhou X, Xie Y, Liang Y, Wang C, et al. A sensitive and specific PCR assay for the detection of Baylisascaris schroederi eggs in giant panda feces. Parasitol Int. 2013;62:435–6.PubMedView ArticleGoogle Scholar
- Ranganathan S, Garg G. Secretome: clues into pathogen infection and clinical applications. Genome Med. 2009;1:113.PubMed CentralPubMedView ArticleGoogle Scholar
- Salinas AE, Wong MG. Glutathione S-transferases-a review. Curr Med Chem. 1999;6:279–310.PubMedGoogle Scholar
- Torres-Rivera A, Landa A. Glutathione transferases from parasites: a biochemical view. Acta Trop. 2008;105:99–112.PubMedView ArticleGoogle Scholar
- Brophy P, Barrett J. Glutathione transferase in helminths. Parasitology. 1990;100:345–9.PubMedView ArticleGoogle Scholar
- Cervi L, Rossi G, Masih DT. Potential role for excretory-secretory forms of glutathione-S-transferase (GST) in Fasciola hepatica. Parasitology. 1999;119:627–33.PubMedView ArticleGoogle Scholar
- Guillou F, Roger E, Moné Y, Rognon A, Grunau C, Théron A, et al. Excretory–secretory proteome of larval Schistosoma mansoni and Echinostoma caproni, two parasites of Biomphalaria glabrata. Mol Biochem Parasitol. 2007;155:45–56.PubMedView ArticleGoogle Scholar
- Brophy P, Patterson L, Brown A, Pritchard D. Glutathione S-transferase (GST) expression in the human hookworm Necator americanus: potential roles for excretory-secretory forms of GST. Acta Trop. 1995;59:259–63.PubMedView ArticleGoogle Scholar
- Liebau E, Höppner J, Mühlmeister M, Burmeister C, Lüersen K, Perbandt M, et al. The secretory omega-class glutathione transferase OvGST3 from the human pathogenic parasite Onchocerca volvulus. FEBS J. 2008;275:3438–53.PubMedView ArticleGoogle Scholar
- LaCourse EJ, Perally S, Morphew RM, Moxon JV, Prescott M, Dowling DJ, et al. The Sigma class glutathione transferase from the liver fluke Fasciola hepatica. PLoS Negl Trop Dis. 2012;6:e1666.PubMed CentralPubMedView ArticleGoogle Scholar
- Kampkötter A, Volkmann TE, de Castro SH, Leiers B, Klotz LO, Johnson TE, et al. Functional analysis of the glutathione S-transferase 3 from Onchocerca volvulus (Ov-GST-3): a parasite GST confers increased resistance to oxidative stress in Caenorhabditis elegans. J Mol Biol. 2003;325:25–37.PubMedView ArticleGoogle Scholar
- Zhan B, Perally S, Brophy PM, Xue J, Goud G, Liu S, et al. Molecular cloning, biochemical characterization, and partial protective immunity of the heme-binding glutathione S-transferases from the human hookworm Necator americanus. Infect Immun. 2010;78:1552–63.PubMed CentralPubMedView ArticleGoogle Scholar
- Brophy PM, Krause S, Walter RD, Liebau E, Fischer P, Sommer A. Gene structure of the extracellular glutathione S-transferase from Onchocerca volvulus and its overexpression and promoter analysis in transgenic Caenorhabditis elegans. Mol Biochem Parasitol. 2001;117:145–54.PubMedView ArticleGoogle Scholar
- Acevedo N, Mohr J, Zakzuk J, Samonig M, Briza P, Erler A, et al. Proteomic and immunochemical characterization of glutathione transferase as a new allergen of the nematode Ascaris lumbricoides. PLoS One. 2013;8:e78353.PubMed CentralPubMedView ArticleGoogle Scholar
- Crompton D. Ascaris and ascariasis. Adv Parasitol. 2001;48:285–375.PubMedView ArticleGoogle Scholar
- Bowman DD, Little MD, Reimers RS. Precision and accuracy of an assay for detecting Ascaris eggs in various biosolid matrices. Water Res. 2003;37:2063–72.PubMedView ArticleGoogle Scholar
- Unites States Environmental Protection Agency (USEPA). Environmental regulations and technology: Control of pathogens and vectorattractionin sewage sludge. Ohio: EPA/625/R-92/013; 2003.Google Scholar
- Thompson JD, Higgins DG, Gibson TJ. CLUSTAL W: improving the sensitivity of progressive multiple sequence alignment through sequence weighting, position-specific gap penalties and weight matrix choice. Nucleic Acids Res. 1994;22:4673–80.PubMed CentralPubMedView ArticleGoogle Scholar
- Tamura K, Peterson D, Peterson N, Stecher G, Nei M, Kumar S. MEGA5: molecular evolutionary genetics analysis using maximum likelihood, evolutionary distance, and maximum parsimony methods. Mol Biol Evol. 2011;28:2731–9.PubMed CentralPubMedView ArticleGoogle Scholar
- Bell BA, Wood JF, Bansal R, Ragab H, Cargo III J, Washington MA, et al. Process development for the production of an E. coli produced clinical grade recombinant malaria vaccine for Plasmodium vivax. Vaccine. 2009;27:1448–53.PubMedView ArticleGoogle Scholar
- Tsuji N, Suzuki K, Kasuga-Aoki H, Isobe T, Arakawa T, Matsumoto Y. Mice intranasally immunized with a recombinant 16-kilodalton antigen from roundworm Ascaris parasites are protected against larval migration of Ascaris suum. Infect Immun. 2003;71:5314–23.PubMed CentralPubMedView ArticleGoogle Scholar
- Fu Y, Nie HM, Niu LL, Xie Y, Deng JB, Wang Q, et al. Comparative efficacy of ivermectin and levamisole for reduction of migrating and encapsulated larvae of Baylisascaris transfuga in mice. Korean J Parasitol. 2011;49:145–51.PubMed CentralPubMedView ArticleGoogle Scholar
- Cui J, Wei T, Liu LN, Zhang X, Qi X, Zhang ZF, et al. Molecular characterization of a Spirometra mansoni antigenic polypeptide gene encoding a 28.7 kDa protein. Parasitol Res. 2014;113:3511–6.PubMedView ArticleGoogle Scholar
- Vlaminck J, Nejsum P, Vangroenweghe F, Thamsborg SM, Vercruysse J, Geldhof P. Evaluation of a serodiagnostic test using Ascaris suum haemoglobin for the detection of roundworm infections in pig populations. Vet Parasitol. 2012;189:267–73.PubMedView ArticleGoogle Scholar
- Erlwein O, Robinson MJ, Kaye S, Wills G, Izui S, Wessely S, et al. Investigation into the presence of and serological response to XMRV in CFS patients. PLoS One. 2011;6:e17592.PubMed CentralPubMedView ArticleGoogle Scholar
- Breathnach R, Chambon P. Organization and expression of eucaryotic split genes coding for proteins. Annu Rev Biochem. 1981;50:349–83.PubMedView ArticleGoogle Scholar
- Liebau E, Eckelt VH, Wildenburg G, Teesdale-Spittle P, Brophy PM, Walter RD, et al. Structural and functional analysis of a glutathione S-transferase from Ascaris suum. Biochem J. 1997;324:659–66.PubMed CentralPubMedGoogle Scholar
- Babu RO, Moorkoth D, Azeez S, Eapen SJ. Virtual screening and in vitro assay of potential drug like inhibitors from spices against Glutathione-S-Transferase of Meloidogyne incognita. Bioinformation. 2012;8:319–25.PubMed CentralPubMedView ArticleGoogle Scholar
- Zhang L, Yang X, Wu H, Gu X, Hu Y, Wei F. The parasites of giant pandas: individual-based measurement in wild animals. J Wildl Dis. 2011;47:164–71.PubMedView ArticleGoogle Scholar
- Xie Y, Zhang Z, Wang C, Lan J, Li Y, Chen Z, et al. Complete mitochondrial genomes of Baylisascaris schroederi, Baylisascaris ailuri and Baylisascaris transfuga from giant panda, red panda and polar bear. Gene. 2011;482:59–67.PubMedView ArticleGoogle Scholar
- Zhao GH, Xu MJ, Zhu XQ. Identification and characterization of microRNAs in Baylisascaris schroederi of the giant panda. Parasit Vectors. 2013;6:216.PubMed CentralPubMedView ArticleGoogle Scholar
- Yang GY, Zhang ZH. Parasitic diseases of wildlife. Beijing: Science Press; 2013.Google Scholar
- Mannervik B, Danielson UH. Glutathione transferases-structure and catalytic activity. CRC Crit Rev Biochem. 1988;23:283–337.PubMedView ArticleGoogle Scholar
- Umasuthan N, Saranya Revathy K, Lee Y, Whang I, Choi CY, Lee J. A novel molluscan sigma-like glutathione S-transferase from Manila clam, Ruditapes philippinarum: cloning, characterization and transcriptional profiling. Comp Biochem Physiol C Toxicol Pharmacol. 2012;155:539–50.PubMedView ArticleGoogle Scholar
- Lee AJ, Huntley J, Van den Broek A, Coates D, Isaac RE. Expression and characterisation of a Psoroptes ovis glutathione S-transferase. Vet Parasitol. 2002;105:49–63.PubMedView ArticleGoogle Scholar
- Blanchette B, Feng X, Singh BR. Marine glutathione S-transferases. Mar Biotechnol. 2007;9:513–42.PubMedView ArticleGoogle Scholar
- Hotez PJ, Diemert D, Bacon KM, Beaumier C, Bethony JM, Bottazzi ME, et al. The human hookworm vaccine. Vaccine. 2013;31:B227–32.PubMed CentralPubMedView ArticleGoogle Scholar
- Curti E, Seid CA, Hudspeth E, Center L, Rezende W, Pollet J, et al. Optimization and revisions of the production process of the Necator americanus glutathione S-transferase 1 (Na-GST-1), the lead hookworm vaccine recombinant protein candidate. Hum Vaccin Immunother. 2014;10:1914–25.PubMedView ArticleGoogle Scholar
- Kennedy MW, Qureshi F. Stage-specific secreted antigens of the parasitic larval stages of the nematode Ascaris. Immunology. 1986;58:515–22.PubMed CentralPubMedGoogle Scholar
- Odoevskaia IM. Diagnostic efficiency of excretory-secretory Trichinella antigens in enzyme immunoassay. Med Parazitol (Mosk). 2007;4:19–24. in Russian.Google Scholar
- Watthanakulpanich D, Smith HV, Hobbs G, Whalley AJ, Billington D. Application of Toxocara canis excretory-secretory antigens and IgG subclass antibodies (IgG1-4) in serodiagnostic assays of human toxocariasis. Acta Trop. 2008;106:90–5.PubMedView ArticleGoogle Scholar
- Gómez-Morales MA, Ludovisi A, Amati M, Pozio E. Validation of an excretory/secretory antigen based-ELISA for the diagnosis of Opisthorchis felineus infection in humans from low trematode endemic areas. PLoS One. 2013;8:e62267.PubMed CentralPubMedView ArticleGoogle Scholar
- Burk SV, Dangoudoubiyam S, Brewster-Barnes T, Bryant UK, Howe DK, Carter CN, et al. In vitro culture of Parascaris equorum larvae and initial investigation of parasite excretory-secretory products. Parasitol Res. 2014;113:4217–24.PubMedView ArticleGoogle Scholar
- Cuéllar C, Fenoy S, Guillén JL. Cross-reactions of sera from Toxocara canis-infected mice with Toxascaris leonina and Ascaris suum antigens. Int J Parasitol. 1992;22:301–7.PubMedView ArticleGoogle Scholar
- Lozano MJ, Martín HL, Díaz SV, Mañas AI, Valero LA, Campos BM. Cross-reactivity between antigens of Anisakis simplex s.l. and other ascarid nematodes. Parasite. 2004;11:219–23.PubMedView ArticleGoogle Scholar
- Dangoudoubiyam S, Vemulapalli R, Ndao M, Kazacos KR. Recombinant antigen-based enzyme-linked immunosorbent assay for diagnosis of Baylisascaris procyonis larva migrans. Clin Vaccine Immunol. 2011;18:1650–5.PubMed CentralPubMedView ArticleGoogle Scholar
- Greve JH, O’Brien SE. Adult Baylisascaris infections in two dogs. Comp Anim Pract. 1989;19:41–3.Google Scholar
- Liebau E, Wildenburg G, Walter RD, Henkle-Dührsen K. A novel type of glutathione S-transferase in Onchocerca volvulus. Infect Immun. 1994;62:4762–7.PubMed CentralPubMedGoogle Scholar
- Striebel HP. Proposed form to evaluate some histological aspects of macrofilarial morphology, its age dependent alterations and drug related changes in nodules of Onchocerca volvulus and O. gibsoni. Trop Med Parasitol. 1988;39:367–89.PubMedGoogle Scholar
- Porchet E, McNair A, Caron A, Kusnierz JP, Zemzoumi K, Capron A. Tissue expression of the Schistosoma mansoni 28 kDa glutathione S-transferase. Parasitology. 1994;109:565–72.PubMedView ArticleGoogle Scholar
- Trottein F, Kieny MP, Verwaerde C, Torpier G, Pierce RJ, Balloul JM, et al. Molecular cloning and tissue distribution of a 26-kilodalton Schistosoma mansoni glutathione S-transferase. Mol Biochem Parasitol. 1990;41:35–44.PubMedView ArticleGoogle Scholar
This is an Open Access article distributed under the terms of the Creative Commons Attribution License (http://creativecommons.org/licenses/by/4.0), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly credited. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated.