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  • Research article
  • Open Access
  • Open Peer Review

Protective immunity against acute toxoplasmosis in BALB/c mice induced by a DNA vaccine encoding Toxoplasma gondii elongation factor 1-alpha

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  • 1Email author
BMC Infectious Diseases201515:448

https://doi.org/10.1186/s12879-015-1220-5

©  Wang et al. 2015

  • Received: 10 December 2014
  • Accepted: 14 October 2015
  • Published:
Open Peer Review reports

Abstract

Background

Toxoplasma gondii can infect almost all warm-blood animals including human beings. The high incidence and severe damage that can be caused by T. gondii infection clearly indicates the need for the development of a vaccine. T. gondii elongation factor 1-alpha (TgEF-1α) plays an important role in pathogenesis and host cell invasion for this parasite. The aim of this study was to evaluate the immune protective efficacy of a DNA vaccine encoding TgEF-1α gene against acute T. gondii infection in mice.

Methods

A DNA vaccine (pVAX-EF-1α) encoding T. gondii EF-1a (TgEF-1α) gene was constructed and its immune response and protective efficacy against lethal challenge in BALB/c mice were evaluated.

Results

Mice inoculated with the pVAX-EF-1α vaccine had a high level of specific anti-T. gondii antibodies and produced high levels of IFN-gamma, interleukin (IL)-4, and IL-17. The expression levels of MHC-I and MHC-II molecules as well as the percentages of both CD4+ and CD8+ T cells in mice vaccinated with pVAX-EF-1α were significantly increased (p < 0.05), compared with those in all the mice from control groups (blank control, PBS, and pVAXI). Immunization with pVAX-EF-1α significantly (p < 0.05) prolonged mouse survival time to 14.1 ± 1.7 days after challenge infection with the virulent T. gondii RH strain, compared with mice in the control groups which died within 8 days.

Conclusions

DNA vaccination with pVAX-EF-1α triggered strong humoral and cellular responses and induced effective protection in mice against acute T. gondii infection, indicating that TgEF-1α is a promising vaccine candidate against acute toxoplasmosis.

Keywords

  • Toxoplasma gondii
  • TgEF-1α
  • DNA vaccine
  • Protective immunity

Background

Toxoplasma gondii, an obligate intracellular protozoan parasite, is responsible for toxoplasmosis in a wide range of hosts including humans, mammals, birds, shellfish and marine mammals [1–5]. In immunocompetent individuals, T. gondii infection is usually asymptomatic or solely causes mild symptoms but can result in severe disease, such as ocular toxoplasmosis or encephalitis in immunocompromised patients, and it causes congenital birth defects [6, 7]. In addition to the risk to human health, T. gondii infection of agriculturally important animals, such as goats, sheep, and pigs, also causes significant economic losses due to animal abortions and neonatal losses [5, 8].

Currently, chemotherapy is the primary strategy in the treatment of the acute phase of this disease, but it is not effective against T. gondii chronic infection [9]. Due to the emergence of drug-resistant parasites and the chemical residues in food that are associated with drug use [10–12], there is an urgent need for an efficient vaccine against toxoplasmosis. During the past decade, anti-T. gondii live, attenuated-live, killed and subunit vaccines have been developed [10]. Although the only licensed T. gondii vaccine, which is based on the attenuated-live T. gondii S48 strain (Toxovax®), can be used to prevent the incidence of abortion in sheep [13], further exploration of its use in other food-producing animals or in humans has been hampered by safety concerns on the possibility of its reversion to a virulence wild type. A DNA vaccine is therefore a better alternative because it does not require the preparation of a whole organism preparation and it has the potential to induce both specific humoral and cellular immune responses as well as long-lasting immunity [10]. In recent years, DNA vaccines against T. gondii have been developed and have received considerable attention as good vaccine options [14].

Elongation factor 1-alpha (EF-1α) is highly conserved and ubiquitously expressed in all eukaryotic cells [15–17]. It plays a central role in protein synthesis within eukaryotic cells, and is responsible for aminoacyl-tRNA loading onto the A site of the ribosome [18]. Additionally, it appears to have a number of other functions associated with cell growth, motility, protein turnover, and signal transduction [19]. Recent studies have also suggested that this protein is involved in DNA replication/repair protein networks [20] and apoptosis [21].

In parasites, EF-1α has been implicated in pathogenesis [22] and host cell invasion [23]. Cryptosporidium parvum (C. parvum) EF-1α protein, which localizes at the apical region of the parasite, mediates cryptosporidial cytoskeletal complex formation. An anti- EF-1α mAb significantly inhibited the host cell invasion by C. parvum in vitro. These results indicate that C. parvum EF-1α plays an essential role in mediating host cell entry by the parasite and, as such, could be a candidate vaccine antigen against cryptosporidiosis [23]. However, to our knowledge, no studies have evaluated the immunogenicity of T. gondii EF-1α (TgEF-1α) and its potential as a vaccine candidate against T. gondii infection.

The objective of the present study was to evaluate the potential of TgEF-1α as a vaccine candidate against acute T. gondii infection. Therefore, we assessed various immune responses in BALB/c mice that received DNA immunization with a eukaryotic plasmid expressing TgEF-1α.

Methods

Ethics statement

The experiments were conducted following the guidelines of the Animal Ethics Committee, Nanjing Agricultural University, China. All experimental protocols were approved by the Science and Technology Agency of Jiangsu Province (approval ID, SYXK (SU) 2010–0005).

Mice and cell culture

Five-week-old female BALB/c mice were purchased from the Center of Comparative Medicine, Yangzhou University (Yangzhou, China) and maintained under specific-pathogen-free conditions.

Baby hamster kidney (BHK) cells were grown and maintained in Dulbecco’s modified Eagle’s medium (DMEM; Gibco, Beijing, China) supplemented with L-glutamine, 10 % dialyzed fetal bovine serum (FBS; Gibco, USA), 100 IU/ml penicillin, and 100 μg/ml streptomycin in a humidified chamber containing 5 % CO2 at 37 °C.

Parasites and preparation of soluble tachyzoite antigens (STAg)

T. gondii RH strain (Type I) was provided by the Laboratory of Veterinary Molecular and Immunological Parasitology, Nanjing Agricultural University, China. The parasites were maintained and collected from the peritoneal cavity of infected BALB/c mice as described previously [24].

Purified tachyzoites were disrupted by three cycles of freezing at −20 °C and thawing at 4 °C. After that, the lysates were sonicated on ice at 60 W/s and centrifuged for 30 min at 12,000 × g. The supernatants were pooled and sterile filtered, and the protein concentration was determined via the Bradford method using bovine serum albumin (BSA) as the standard. STAg was stored in aliquots at −70 °C until use.

Construction of the DNA vaccine plasmid

The complete open reading frame (ORF) of TgEF-1α (GenBank accession no. XM_002370208.1) was amplified by reverse transcription-polymerase chain reaction (RT-PCR) using designed specific primers (forward primer: 5′- CGCGGATCCATGGGTAAGGAAAAGACTCACATTAAC −3′ and reverse primer: 5′- CCGCTCGAGCGAAGCGGTAGATTTGTTCCAAT −3′), in which the BamHI and XhoI restriction sites, respectively, were introduced and are shown in italics here. Following ligation of the obtained RT-PCR product with the pMD19-T vector (Takara, Dalian, China) to form pMD-EF-1a, the TgEF-1α fragment was cleaved from pMD-EF-1a by BamHI and XhoI and subcloned into the corresponding sites of pVAXI vector (Invitrogen, Carlsbad, CA, USA). The resulting plasmid was named pVAX-EF-1α. The concentration of the extracted pVAX-EF-1α was determined by spectrophotometry at OD260 and OD280.

Sequence analysis

The sequence similarity of TgEF-1α to EF-1α from other species was studied using BLASTP and BLASTX (http://blast.ncbi.nlm.nih.gov/Blast.cgi). EF-1α sequences were aligned using MEGA4.0.

Expression of recombinant plasmids in vitro

Before transfection, BHK cells were transferred to 6-well plates (Corning Costar, Cambridge, MA, USA). When the confluency of the cells reached 80 %–90 %, 5 μg of the recombinant eukaryotic plasmid (pVAX-EF-1α) was used to transfect the cells using Lipofectamine 3000 regent (Invitrogen, Carlsbad, CA, USA) according to the manufacturer’s instructions. The empty vector pVAXI (5 μg) was also transfected into BHK cells as a negative control. Lipofectamine 3000 reagent was respectively mixed with pVAX-EF-1α or pVAXI at a concentration of 10 μg/ml in DMEM without Fetal Bovine Serum (FBS) and antibiotics, and was incubated at room temperature for 30 min. The mixture of lipofectamine and plasmid was then added into BHK cells. The cells were incubated with the transfection mixture for 6 h at 37 °C in the presence of 5 % CO2. At the end of this incubation, fresh growing medium was supplemented and plates were returned to the cell incubator for further incubation. After 48 h of incubation, the transfected cells were treated on ice with RIPA lysis buffer (50 mM Tris pH 7.4, 150 mM NaCl, 1 % Triton X-100, 1 % Sodium deoxycholate and 0.1 % SDS) containing 1 mM protease inhibitor phenylmethanesulfonyl fluoride (PMSF) and centrifuged at 13,000 × g for 10 min. The translation of the transfected genes in BHK cells was detected by western blot analysis with anti-T. gondii polyclonal antibody (from chicken) as a primary antibody and a horseradish peroxidase (HRP)-labeled goat anti-chicken IgG antibody (SouthernBiotech, Birmingham, AL, USA) as a secondary antibody. Finally, the membrane was soaked in DAB Reagents (Boshide Biotech Co, Wuhan, China) for signal development.

BALB/c mice immunization and challenge

To assess the immunogenicity of the recombinant plasmids, BALB/c mice were randomly divided into four groups of 30 mice per group. Before vaccination, plasmids were diluted and suspended in sterile phosphate buffered saline (PBS) to a final concentration of 1 μg/μl. All experimental groups were injected intramuscularly (i.m.) three times at weeks 0, 2, and 4 with plasmid DNA (100 μg/each), PBS (100 μl/each) or empty plasmid (100 μg/each), respectively, and one group of mice was not inoculated, which served as a blank control. Blood samples of mice were collected from the tail vein plexus on the day before each vaccination and 2 weeks after the last vaccination. The sera were obtained from the blood samples and stored at −20 °C for evaluation of antibody content and cytokine measurement. At weeks 0, 2, 4, and 6, five mice from each group were sacrificed, and the spleens were collected and used to isolate the splenic lymphocytes for flow cytometry analyses. The remaining ten mice in each group were used for the challenge experiment. Two weeks after the last injection, mice from all four groups were challenged intraperitoneally (i.p) with 1 × 104 tachyzoites of T. gondii RH strain. The survival times of the mice were observed and recorded on a daily basis.

Determination of antibodies by ELISA

The levels of antibodies in mouse sera were determined by enzyme-linked immunosorbent assay (ELISA) as previously described [25]. In brief, the microtiter plates (Corning Costar, Cambridge, MA, USA) were coated overnight at 4 °C with 10 μg /ml STAg in 50 mM carbonate buffer pH 9.6 (100 μl per well). After three washes, the plates were blocked with 3 % Bovine Serum Albumin (BSA) for 2 h at 37 °C and subsequently incubated with the mouse sera diluted 1:10 in PBS for 1 h at 37 °C. HRP-conjugated goat anti-mouse IgA, IgM, IgE, IgG, IgG1, or IgG2a (SouthernBiotech, Birmingham, AL, USA) was used as the secondary antibody to detect bound antibodies. Finally, the immune complexes were developed by incubation with 3,3,5,5-tetramethylbenzidine (TMB) for 20 min. The reaction was stopped by adding 2 M H2SO4, and the absorbance was measured at 450 nm with an automated ELISA reader (Multiskan FC, Thermo scientific, Waltham, MA, USA). All samples were run in triplicate.

Cytokine assays

To assay cytokine production levels, sera from each experimental group were obtained as described above. Interferon gamma (IFN-γ), interleukin-4 (IL-4), interleukin-17 (IL-17) and transformation growth factor-β1 (TGF-β1) were measured using ELISA kits according to the manufacturer’s instructions (Boster Systems, Wuhan, China). Cytokine concentrations were determined by reference to standard curves constructed with known amounts of mouse recombinant IL-4, IL-17, IFN-γ or TGF-β1. The analysis was performed with the data from three independent experiments.

Flow cytometry analysis of T cell subsets and MHC molecules

The levels of CD4+ and CD8+ T cell subsets and the levels of MHC-I and MHC-II molecules in the splenocytes of mice from the four test groups, pVAX-EF-1α, pVAXI, PBS, and blank, were determined using flow cytometry as previously described [26]. Splenocyte suspensions (1 × 106 cells/ml) were dually stained with anti-mouse CD3e-FITC + anti-mouse CD8-PE, anti-mouse CD3e-FITC + anti-mouse CD4-PE, anti-mouse CD3e-FITC + anti-mouse MHC-I-PE or anti-mouse CD3e-FITC + anti-mouse MHC-II-PE (eBioscience, San Diego, CA, USA) for 30 min at 4 °C in the dark. Cell population analyses were conducted with a FACScan flow cytometer with CellQuest software (BD Biosciences, Franklin Lakes, NJ, USA). Lymphocyte specific gating was set according to the forward and side scatter profiles. The percentages of CD4+ and CD8+ T lymphocytes or, MHC-I and MHC-II molecules in mouse splenocytes were determined as previously described [27].

Statistical analysis

All statistical analyses were performed by IBM SPSS 20.0 Data Editor (SPSS Inc., Chicago, IL, USA). The differences of the data (e.g., antibody responses and, cytokine production) between all groups were compared by one-way ANOVA. Survival times of the mice were compared using the Kaplan–Meier method. The differences between groups were considered statistically significant if the p value was less than 0.05.

Results

Successful construction of the eukaryotic expression plasmids

The DNA vaccine pVAX-EF-1α was constructed as described in the Methods. To test that the construction was successful, an enzyme digestion was performed with BamH I and Xho I, yielding a fragment of the expected size, 1,347 pb (Fig. 1). A sequence analysis was also performed and its results showed that the insert in the vector was the ORF of TgEF-1α. Together, these results indicate that the DNA vaccine pVAX-EF-1α was constructed correctly.
Fig. 1
Fig. 1

Identification of the recombinant plasmid with restriction enzyme digestion. Lanes 1, the eukaryotic construct pVAX-EF-1α was double digested by BamH I and Xho I enzymes and the product was resolved by 1 % agarose gel to verify a band of size 1347 bp. (M) Represents DNA Molecular marker

TgEF-1α multiple sequence alignment and cladogram

When compared with the known EF-1α protein sequences on the NCBI database (http://blast.ncbi.nlm.nih.gov/Blast.cgi), the TgEF-1α amino acid sequence had 74 % identity to Bos taurus (gi|14422440), Gallus gallus (gi|488468), and Homo sapiens (gi|15421129), 73 % identity to Mus musculus (gi|50797) and Sus scrofa (gi|350588388), 70 % to Capra hircus (gi|548523658), and 67 % identity to Canis lupus familiaris (gi|545523055).

In contrast, the TgEF-1α sequence had 99 % identity to the EF-1α of T. gondii ME49 and T. gondii GT1, 98 % identity to Neospora caninum (gi|401395932), 86 % identity to Cryptosporidium hominis (gi|67601420), 85 % identity to Eimeria acervulina (gi|557118408), and 83 % identity to Babesia bovis (gi|156087152).

The phylogenetic tree of amino acid sequences was built using MEGA4.0, and the resulting cladogram (Fig. 2) showed that the kinship of TgEF-1α protein with other species of apicomplexan parasites (Neospora caninum, Babesia bovis, Cryptosporidium hominis, and Eimeria acervulina) was high when compared with its kinship with other host species (Mus musculus, Bos taurus, Gallus gallus, Canis lupus familiaris, Capra hircus, Sus scrofa, and Homo sapiens).
Fig. 2
Fig. 2

The phylogenetic tree of amino acid sequences between TgEF-1α and those of EF-1α from other species

Western blot analyses of proteins synthesized in vitro

BHK cells were transfected with pVAX-EF-1α. The lysates of transfected cells were analyzed on immunoblots (Fig. 3). The lysate of BHK cells transfected with pVAX-EF-1α was specifically recognized by serum obtained from a T. gondii infected chicken. In contrast, cells transfected with pVAX I were not recognized by this serum.
Fig. 3
Fig. 3

Identification of TgEF-1α in BHK cells by western blot analysis. Lane 1, lysates of BHK cells transfected with pVAX-EF-1α was probed with chicken anti-T. gondii sera. Lane 2, Lysates of BHK cells transfected with empty pVAXI vector probed with chicken anti-T. gondii sera. (M) Pre-stained protein molecular marker

Humoral response induced by DNA immunization

To evaluate the level of antibody induced by three consecutive DNA immunizations, we collected serum samples prior to each vaccination as well as at 2 weeks after the last immunization. Then, we performed ELISAs to determine the total IgG, the distribution of IgG1 and IgG2a isotypes, and the IgA, IgM, and IgE two weeks after the last immunization. Compared with the three control groups, a significantly higher level of IgG antibody was detected in the sera of mice immunized with pVAX-EF-1α (p < 0.01), and the OD values of IgG continuously increased with successive DNA immunizations. There were no statistically significantly differences in the IgG levels among the three control groups (Fig. 4a).
Fig. 4
Fig. 4

The dynamics of humoral response in BALB/c mice induced by DNA vaccination. a. Determination of IgG antibodies in the sera of BALB/c mice immunized with pVAX-EF-1α, pVAXI, PBS and Blank controls on weeks 0, 2, 4, 6. Determination of IgG subclass (b) IgG1 and (c) IgG2a, (d) levels of class IgA, (e) levels of class IgM and (f) levels of class IgE in the sera of the immunized BALB/c mice two weeks after the last immunization. Results are expressed as mean of the OD450 ± SD. (n = 5) and statistically significant difference (P < 0.05) and (P < 0.01) are indicated by (*) and (**), respectively

The levels of IgG1 and IgG2a in the pVAX-EF-1α group were also the highest in comparison with those in the three control groups (p < 0.01) (Fig. 4b & c). An apparent predominance of IgG2a over IgG1 was observed in immunized mice, demonstrating that a Th1-type cell immune response was elicited by immunization with pVAX- EF-1α.

Regarding the IgA, IgM, and IgE levels, in comparison with the levels in the control groups, the dynamics of IgA and IgM demonstrated significantly higher OD values (p < 0.01) in the immunized group: 0.533 ± 0.037 and 0.701 ± 0.048, respectively (Fig. 4d & e). However, IgE activity showed no significant differences between any of the groups at the time of evaluation (Fig. 4f).

Cytokine production

Sera samples collected at weeks 0, 2, 4, and 6 were used to measure the amounts of IFN-γ, IL-4, IL-17, and TGF-β1 produced in the different experimental groups. As shown in Fig. 5a, significantly higher levels of IFN-γ were observed in mice immunized with pVAX-EF-1α compared to the three control groups at 2, 4, and 6 weeks post-immunization. Small amounts of IL-4 and IL-17 were also secreted by mice in the pVAX-EF-1α group post-immunization, which although modest, were still significantly higher than the amounts secreted by mice in any of the three control groups post-immunization (p < 0.05) (Fig. 5b & c). In contrast, the levels of TGF-β1 displayed no significant changes between any of the groups at similar times of evaluation (Fig. 5d).
Fig. 5
Fig. 5

Cytokine production. Antibody-captured ELISA was used to determine the production levels of (a) IFN-γ, (b) IL-4, (c) IL-17 and (d) TGF-β1, in sera samples (n = 5) collected at weeks 0, 2, 4 and 6, and the comparison results were expressed as means ± SD of pg/ml. The asterisk designates statistically significant differences (* represents p < 0.05; ** represents p < 0.01) between groups. Results presented here were from three independent experiments

T lymphocytes CD4+ and CD8+subpopulations and MHC molecule changes

As illustrated in Table 1 and Fig. 6a, the percentage of CD4+ T cells was significantly increased (p < 0.01) in the pVAX-EF-1α group 2 weeks after the last vaccination (32.43 ± 3.23), compared with that in the pVAXI (18.84 ± 1.83), PBS (17.93 ± 2.31) and the blank (18.17 ± 1.54) groups. Meanwhile, pVAX-EF-1α group showed the highest percentage of CD8+ T cells after the last immunization (14.36 ± 1.76), which was significantly different at (p < 0.01) when compared with the percentages in the control groups: pVAXI (8.27 ± 1.96), PBS (8.01 ± 1.54) and blank (8.11 ± 1.12) (Table 1 and Fig. 6b).
Table 1

Flow cytometry analysis of the percentages of T lymphocyte subsets

Marker (%)

Time point

Groups (n = 5)

Blank

PBS

pVAXI

pVAX-EF-1a

CD4+

Week 0

18.01 ± 2.95

18.53 ± 2.76

18.23 ± 2.85

17.98 ± 2.45

 

Week 2

18.41 ± 1.85

18.55 ± 1.96

17.90 ± 2.53

28.18 ± 3.05a

 

Week 4

18.03 ± 2.84

18.80 ± 2.88

18.15 ± 1.93

30.46 ± 3.59a

 

Week 6

18.17 ± 1.54

17.93 ± 2.31

18.84 ± 1.83

32.43 ± 3.23a

CD8+

Week 0

8.20 ± 1.55

8.13 ± 1.28

8.47 ± 1.81

8.32 ± 1.65

 

Week 2

8.32 ± 1.94

8.00 ± 1.48

7.94 ± 1.15

13.23 ± 2.41a

 

Week 4

8.37 ± 2.07

8.13 ± 1.58

8.25 ± 1.52

12.50 ± 3.11a

 

Week 6

8.11 ± 1.12

8.01 ± 1.54

8.27 ± 1.96

14.36 ± 1.76a

Data are presented as the mean ± SD (n = 5). a represents statistically highly significant difference (p < 0.01) as compared with control groups: Blank, PBS and pVAXI

Fig. 6
Fig. 6

Flow cytometry strategy. Detection of T lymphocyte subpopulation and MHC molecules using flow cytometry technique (CD3 gated), a CD4+ T lymphocytes (CD3+CD4+, region Q2). b CD8+ T lymphocytes (CD3+CD8+, region Q2). c MHC-I molecules (CD3+MHC-I, region Q2). d. MHC-II molecules (CD3+MHC-II, region Q2)

After the last immunization, the immunized group had a significantly higher percentage of MHC-I+ cells (32.96 ± 3.04), in contrast to pVAXI (18.14 ± 2.30), PBS (17.76 ± 1.16), and blank (17.88 ± 1.78) groups (Fig. 6c). The amount of MHC-II+ cells increased over time in the vaccinated group (Fig. 6d), starting at week 2 of the experiment and reaching a peak point (8.26 ± 1.23) at week 6 of the experiment that was significantly higher (p < 0.01) than the levels of MHC-II+ cells in the control groups: pVAXI (3.24 ± 0.53), PBS (3.11 ± 0.73), and blank (3.22 ± 0.56) (Table 2).
Table 2

Dynamics of MHC-I and MHC-II molecules in spleen lymphocytes

Marker (%)

Time point

Groups (n = 5)

Blank

PBS

PVAXI

PVAX-EF-1a

MHC-I

Week 0

18.19 ± 2.46

17.17 ± 2.62

16.99 ± 1.38

17.29 ± 2.34

 

Week 2

16.55 ± 2.15

17.13 ± 1.91

17.06 ± 2.44

24.23 ± 3.33a

 

Week 4

17.64 ± 1.82

18.02 ± 1.91

17.62 ± 1.46

31.44 ± 3.54a

 

Week 6

17.88 ± 1.78

17.76 ± 1.16

18.14 ± 2.30

32.96 ± 3.04a

MHC-II

Week 0

3.07 ± 0.97

2.88 ± 0.37

3.31 ± 0.49

3.27 ± 0.61

 

Week 2

2.99 ± 0.71

3.17 ± 0.38

3.07 ± 0.97

4.84 ± 1.86a

 

Week 4

3.25 ± 0.45

3.17 ± 0.38

3.27 ± 0.59

7.52 ± 1.42a

 

Week 6

3.22 ± 0.56

3.11 ± 0.73

3.24 ± 0.53

8.26 ± 1.23a

Data are presented as the mean ± SD (n = 5). a represents statistically highly significant difference (p < 0.01) as compared with control groups: Blank, PBS and pVAXI

Assessment of the protective efficacy of DNA immunization of mice against acute T. gondii infection

To analyze the protective efficacy of DNA vaccination against T. gondii, we assessed the survival time of mice after infection with 104 tachyzoites of the virulent RH strain. The mice immunized with pVAX-EF-1α had a significantly prolonged survival time (14.1 ± 1.7 days, p < 0.05) compared with the control mice that received either pVAX I or PBS. All of the mice in the control groups died within 8 days (Fig. 7).
Fig. 7
Fig. 7

Survival curve of mice after challenge infection with Toxoplasma gondii RH strain. Mice were challenged with 104 tachyozoites of the RH strain intraperitoneally two weeks after the third immunization

Discussion

In the present study, a DNA vaccine encoding TgEF-1α was constructed and its capacity to induce highly significant immune responses and subsequent protection of BALB/c mice against a lethal dose challenge of the highly virulent T. gondii RH strain was demonstrated.

Humoral immunity in the form of antigen specific IgG antibodies seems to be important in controlling T. gondii invasion [28]. These specific antibodies can inhibit parasite attachment to the host cell receptors and can promote macrophages to kill intracellular parasites, which seem to be important in controlling T. gondii infection and its reactivation [29]. Here, the high level of anti-T. gondii IgG antibody was induced in the experimental group (pVAX-EF-1α vaccinated mice) compared with the levels in the three control groups (p < 0.05). Further analyses of the IgG subclasses (IgG1 and IgG2a) revealed a predominance of IgG2a over IgG1, indicating that pVAX-EF-1α could elicit a Th1-biased humoral immune response, which is considered to play a critical role in the protective immunity against T. gondii [30, 31]. This result is consistent with those described in previous studies [31–33].

Immunoglobulins IgA, IgM, and IgE have also been reported to participate in the immunological responses against T. gondii infection [34–37]. However, less attention has been paid to these immunoglobulins during vaccination trials, where the focus has been almost entirely directed to IgG [25, 38, 39]. IgA is important in mucosal immunity to oral infection with toxoplasma cysts [40]. Since antibodies of this isotype are important in preventing re-infection with T. gondii, inducing IgA may be a major strategic aspect of vaccine development [35]. IgM has been reported to increase the phagocytic capacity of neutrophils and to be potentially capable of activating the complement cascade, which may result in killing of the parasite [41, 42]. Moreover, it could reduce the spread of the parasite by blocking cell invasion [43]. In our study, high titers of IgA and IgM were detected in the immunized group, indicating that TgEF-1α had successfully induced the release of these antibodies as part of the response generated after immunization.

The induction of IgE has been previously recognized during the T. gondii infection [37, 44]. However, our data revealed no significant traces of this immunoglobulin after vaccination with TgEF-1α, an observation consistent with findings from previous studies [25, 45, 46].

Cytokines play an important role in the activities of T helper (Th) cells. It is well known that IFN-γ is the central cytokine that is responsible for resistance against T. gondii during both the early and late stages of infection [47–50]. Compared with the three control treatments, immunization with pVAX-EF-1α enhanced the Th1 mediated immunity by inducing a high level of IFN-γ. In addition, as a factor of Th2 type immune response, a slight increase of cytokine IL-4 was also observed. These results therefore demonstrated that pVAX-EF-1α could elicit strong Th1 cellular immune responses, which is essential for cell-mediated immunity and resistance against intracellular pathogens [51, 52]. Similarly, several other studies reported a distinct pattern of Th1 response to DNA-based vaccines against T. gondii [30, 45, 53].

IL-17 is produced by Th17 cells and functions as a tissue inflammatory modulator [54]. This cytokine is also involved in the resistance against T. gondii infection [55, 56]. In this investigation, a significant increase of IL-17 concentration was detected in pVAX-EF-1α vaccinated mice over the levels in the control group mice. This finding indicated that TgEF-1a was capable of inducing Th17 differentiation and resulted in an inflammatory reaction. Additional research regarding this T helper type of cells is required to further clarify the roles played by this cell type and the cytokines it releases during vaccination against T. gondii.

The cytokine TGF-β produced by regulatory T cells (Treg cells) plays an integral role in regulating immune responses. TGF-β has pleiotropic effects on adaptive immunity, especially in the regulation of effector and regulatory CD4+ T cell responses [57]. TGF-β signaling was activated in astrocytes during toxoplasmic encephalitis and inhibition of astrocytic TGF-β signaling increases immune cell infiltration, uncouples proinflammatory cytokine and chemokine production from the central nervous system parasite burden, and increases neuronal injury [58]. Our results showed that no significant production of TGF-β1 was detected in pVAX-EF-1α vaccinated group. This finding could be due to its antagonistic relationship with other cytokines, such as IFN-γ [59–61].

Among the subclasses of T lymphocytes, CD4+ and CD8+ T lymphocytes play an important role in host resistance to T. gondii infection [62]. CD3+ CD4+ CD8− is the surface marker of T helper (Th) cells that can participate in the adaptive immune responses, while CD3+ CD8+ CD4− is expressed on cytotoxic T cells (CTLs) which is classified as a pre-defined cytotoxic role player within the immune system [63]. In the present study, we observed differences in the relative proportions of CD4+ and CD8+ T cells between the vaccinated and control groups. Specifically, we found an increase in both of these components in immunized mice. This observation suggests that immunization with pVAX-EF-1α may induce the activation of both CD4+ and CD8+ T cells, which may contribute synergistically to cytotoxic activity against T. gondii infection.

DNA vaccines stimulate both the exogenous (MHC class II restricted) and the endogenous (MHC class I restricted) antigen presentation pathways [53]. This study found that both the MHC class I and MHC class II molecules were up-regulated in the pVAX-EF-1α vaccinated group compared with their levels in the control groups. The enhancement of MHC class I expression might be related to the significant increase of IFN-γ that we observed in the pVAX-EF-1α vaccinated group. IFN-γ up-regulates MHC class I expression as well as antigen processing and presentation on cells via activation of Janus kinase /Signal transducer and activator of transcription 1 (JAK/STAT1) signal transduction pathway. Briefly, MHC class I antigen presentation-associated gene expression is initiated by interferon regulatory factor-1 (IRF-1). IRF-1 expression is initiated by phosphorylated STAT1. IFN-γ binds to IFN receptors, and then activates JAK1/JAK2/STAT1 signal transduction via phosphorylation of JAK and STAT1 in cells [64, 65]. An up-regulation of MHC class I molecules would generally facilitate the CD8+ cytotoxic T cell killing of T. gondii-infected cells and may serve to limit parasite multiplication [66]. The up-regulated MHC-II molecules would be able to present more T. gondii-derived antigenic peptides to CD4+ T cells and induce stronger immune responses during T. gondii infection, leading to inhibition of the parasite [62].

To evaluate the protection efficacy of the DNA vaccine, immunized BALB/c mice were intraperitoneally challenged with 1 × 104 tachyzoites of the highly virulent T. gondii RH strain. In this acute infection model, mice immunized with pVAX-EF-1α had a significantly prolonged survival time, demonstrating the protective efficacy of this vaccine, which was similar to the results of previous studies employing several other single gene DNA vaccines [25, 45, 67]. but it is not as good as that of other pVAX vaccination candidates such as pVAX-eIF4A [68], pVAX-ROP9 [33] and pVAX-ROP8 [69].

Conclusion

In summary, this study revealed that the DNA vaccine pVAX-EF-1α encoding TgEF-1α can trigger strong humoral and cellular immune responses, and can induce a prolonged survival time against lethal T. gondii challenge. Although TgEF-1α elicited only partial protection against acute toxoplasmosis, it could be used as a potential vaccine candidate in further studies of multi-component T. gondii vaccines against toxoplasmosis.

Declarations

Acknowledgements

This work was supported by the Special Fund for Public Welfare Industry of Ministry of Agriculture of China (200903036–04) and the Priority Academic Program Development of Jiangsu Higher Education Institutions (PAPD).

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

Authors’ Affiliations

(1)
College of Veterinary Medicine, Nanjing Agricultural University, Nanjing, Jiangsu, 210095, PR China

References

  1. Zhao G, Shen B, Xie Q, Xu LX, Yan RF, Song XK, et al. Detection of Toxoplasma gondii in free-range chickens in China based on circulating antigens and antibodies. Vet Parasitol. 2012;185:72–7.View ArticlePubMedGoogle Scholar
  2. Zhang M, Yang Z, Wang S, Tao L, Xu L, Yan R, et al. Detection of Toxoplasma gondii in shellfish and fish in parts of China. Vet Parasitol. 2014;200:85–9.View ArticlePubMedGoogle Scholar
  3. Alvarado-Esquivel C, Sanchez-Okrucky R, Dubey JP. Serological evidence of Toxoplasma gondii infection in captive marine mammals in Mexico. Vet Parasitol. 2012;184:321–4.View ArticlePubMedGoogle Scholar
  4. Vado-Solis IA, Suarez-Solis V, Jimenez-Delgadillo B, Zavala-Velazquez JE, Segura-Correa JC. Toxoplasma gondii presence in women with spontaneous abortion in Yucatan, Mexico. J Parasitol. 2013;99:383–5.View ArticlePubMedGoogle Scholar
  5. Edwards JF, Dubey JP. Toxoplasma gondii abortion storm in sheep on a Texas farm and isolation of mouse virulent atypical genotype T. gondii from an aborted lamb from a chronically infected ewe. Vet Parasitol. 2013;192:129–36.View ArticlePubMedGoogle Scholar
  6. Pfaff AW, de-la-Torre A, Rochet E, Brunet J, Sabou M, Sauer A, et al. New clinical and experimental insights into Old World and neotropical ocular toxoplasmosis. Int J Parasitol. 2014;44:99–107.View ArticlePubMedGoogle Scholar
  7. Atreya AR, Arora S, Gadiraju VT, Martagon-Villamil J, Skiest DJ. Toxoplasma encephalitis in an HIV-infected patient on highly active antiretroviral therapy despite sustained immune response. Int J STD AIDS. 2014;25:383–6.View ArticlePubMedGoogle Scholar
  8. Kim JH, Kang KI, Kang WC, Sohn HJ, Jean YH, Park BK, et al. Porcine abortion outbreak associated with Toxoplasma gondii in Jeju Island, Korea. J Vet Sci. 2009;10:147–51.View ArticlePubMedPubMed CentralGoogle Scholar
  9. Rodriguez JB, Szajnman SH. New antibacterials for the treatment of toxoplasmosis; a patent review. Expert Opin Ther Pat. 2012;22:311–33.View ArticlePubMedGoogle Scholar
  10. Kur J, Holec-Gasior L, Hiszczynska-Sawicka E. Current status of toxoplasmosis vaccine development. Expert Rev Vaccines. 2009;8:791–808.View ArticlePubMedGoogle Scholar
  11. Garrison EM, Arrizabalaga G. Disruption of a mitochondrial MutS DNA repair enzyme homologue confers drug resistance in the parasite Toxoplasma gondii. Mol Microbiol. 2009;72:425–41.View ArticlePubMedPubMed CentralGoogle Scholar
  12. Nagamune K, Moreno SN, Sibley LD. Artemisinin-resistant mutants of Toxoplasma gondii have altered calcium homeostasis. Antimicrob Agents Chemother. 2007;51:3816–23.View ArticlePubMedPubMed CentralGoogle Scholar
  13. Buxton D, Innes EA. A commercial vaccine for ovine toxoplasmosis. Parasitology. 1995;110(Suppl):S11–16.View ArticlePubMedGoogle Scholar
  14. Zhang NZ, Chen J, Wang M, Petersen E, Zhu XQ. Vaccines against Toxoplasma gondii: new developments and perspectives. Expert Rev Vaccines. 2013;12:1287–99.View ArticlePubMedGoogle Scholar
  15. Parkhill J, Achtman M, James KD, Bentley SD, Churcher C, Klee SR, et al. Complete DNA sequence of a serogroup A strain of Neisseria meningitidis Z2491. Nature. 2000;404:502–6.View ArticlePubMedGoogle Scholar
  16. Strausberg RL, Feingold EA, Grouse LH, Derge JG, Klausner RD, Collins FS, et al. Generation and initial analysis of more than 15,000 full-length human and mouse cDNA sequences. Proc Natl Acad Sci U S A. 2002;99:16899–903.View ArticlePubMedGoogle Scholar
  17. Kristensen R, Torp M, Kosiak B, Holst-Jensen A. Phylogeny and toxigenic potential is correlated in Fusarium species as revealed by partial translation elongation factor 1 alpha gene sequences. Mycol Res. 2005;109:173–86.View ArticlePubMedGoogle Scholar
  18. Condeelis J. Elongation factor 1 alpha, translation and the cytoskeleton. Trends Biochem Sci. 1995;20:169–70.View ArticlePubMedGoogle Scholar
  19. Ridgley EL, Xiong ZH, Kaur KJ, Ruben L. Genomic organization and expression of elongation factor-1 alpha genes in Trypanosoma brucei. Mol Biochem Parasitol. 1996;79:119–23.View ArticlePubMedGoogle Scholar
  20. Toueille M, Saint-Jean B, Castroviejo M, Benedetto JP. The elongation factor 1A: a novel regulator in the DNA replication/repair protein network in wheat cells? Plant Physiol Biochem. 2007;45:113–8.View ArticlePubMedGoogle Scholar
  21. Lamberti A, Longo O, Marra M, Tagliaferri P, Bismuto E, Fiengo A, et al. C-Raf antagonizes apoptosis induced by IFN-alpha in human lung cancer cells by phosphorylation and increase of the intracellular content of elongation factor 1A. Cell Death Differ. 2007;14:952–62.PubMedGoogle Scholar
  22. Nandan D, Reiner NE. Leishmania donovani engages in regulatory interference by targeting macrophage protein tyrosine phosphatase SHP-1. Clin Immunol. 2005;114:266–77.View ArticlePubMedGoogle Scholar
  23. Matsubayashi M, Teramoto-Kimata I, Uni S, Lillehoj HS, Matsuda H, Furuya M, et al. Elongation factor-1alpha is a novel protein associated with host cell invasion and a potential protective antigen of Cryptosporidium parvum. J Biol Chem. 2013;288:34111–20.View ArticlePubMedPubMed CentralGoogle Scholar
  24. Wang S, Zhao G, Wang W, Xie Q, Zhang M, Yuan C, et al. Pathogenicity of two Toxoplasma gondii strains in chickens of different ages infected via intraperitoneal injection. Avian Pathol. 2014;43:91–5.View ArticlePubMedGoogle Scholar
  25. Hassan IA, Wang S, Xu L, Yan R, Song X, Li X. DNA vaccination with a gene encoding Toxoplasma gondii Deoxyribose Phosphate Aldolase (TgDPA) induces partial protective immunity against lethal challenge in mice. Parasites Vectors. 2014;7:431.View ArticlePubMedPubMed CentralGoogle Scholar
  26. Sasai K, Aita M, Lillehoj HS, Miyamoto T, Fukata T, Baba E. Dynamics of lymphocyte subpopulation changes in the cecal tonsils of chickens infected with Salmonella enteritidis. Vet Microbiol. 2000;74:345–51.View ArticlePubMedGoogle Scholar
  27. Song H, Yan R, Xu L, Song X, Shah MA, Zhu H, et al. Efficacy of DNA vaccines carrying Eimeria acervulina lactate dehydrogenase antigen gene against coccidiosis. Exp Parasitol. 2010;126:224–31.View ArticlePubMedGoogle Scholar
  28. Correa D, Canedo-Solares I, Ortiz-Alegria LB, Caballero-Ortega H, Rico-Torres CP. Congenital and acquired toxoplasmosis: diversity and role of antibodies in different compartments of the host. Parasite Immunol. 2007;29:651–60.View ArticlePubMedGoogle Scholar
  29. Kang H, Remington JS, Suzuki Y. Decreased resistance of B cell-deficient mice to infection with Toxoplasma gondii despite unimpaired expression of IFN-gamma, TNF-alpha, and inducible nitric oxide synthase. J Immunol. 2000;164:2629–34.View ArticlePubMedGoogle Scholar
  30. Xu Y, Zhang NZ, Tan QD, Chen J, Lu J, Xu QM, et al. Evaluation of immuno-efficacy of a novel DNA vaccine encoding Toxoplasma gondii rhoptry protein 38 (TgROP38) against chronic toxoplasmosis in a murine model. BMC Infect Dis. 2014;14:525.View ArticlePubMedPubMed CentralGoogle Scholar
  31. Qu D, Han J, Du A. Evaluation of protective effect of multiantigenic DNA vaccine encoding MIC3 and ROP18 antigen segments of Toxoplasma gondii in mice. Parasitol Res. 2013;112:2593–9.View ArticlePubMedGoogle Scholar
  32. Chen J, Li ZY, Huang SY, Petersen E, Song HQ, Zhou DH, et al. Protective efficacy of Toxoplasma gondii calcium-dependent protein kinase 1 (TgCDPK1) adjuvated with recombinant IL-15 and IL-21 against experimental toxoplasmosis in mice. BMC Infect Dis. 2014;14:487.View ArticlePubMedPubMed CentralGoogle Scholar
  33. Chen J, Zhou DH, Li ZY, Petersen E, Huang SY, Song HQ, et al. Toxoplasma gondii: protective immunity induced by rhoptry protein 9 (TgROP9) against acute toxoplasmosis. Exp Parasitol. 2014;139:42–8.View ArticlePubMedGoogle Scholar
  34. Gomez-Marin JE, Montoya-De-Londono MT, Castano-Osorio JC, Heine FA, Duque AM, Chemla C, et al. Frequency of specific anti-Toxoplasma gondii IgM, IgA and IgE in colombian patients with acute and chronic ocular toxoplasmosis. Mem Inst Oswaldo Cruz. 2000;95:89–94.View ArticlePubMedGoogle Scholar
  35. Lynch LF, Lynch MI, Ferreira RS, Vasconcelos MS, Melo N, Ferreira S, et al. Ocular toxoplasmosis: evaluation of lacrimal-specific secretory IgA levels in both patients with active and inactive phases of the disease. Mem Inst Oswaldo Cruz. 2011;106:625–8.View ArticlePubMedGoogle Scholar
  36. Amin A, Mazloomzadeh S, Haniloo A, Mohammadian F, Fazaeli A. Evaluation of anti-toxoplasma IgG, IgM, and IgA in mothers with spontaneous abortion in Zanjan, Northwest Iran. Korean J Parasitol. 2012;50:371–4.View ArticlePubMedPubMed CentralGoogle Scholar
  37. Vouldoukis I, Mazier D, Moynet D, Thiolat D, Malvy D, Mossalayi MD. IgE mediates killing of intracellular Toxoplasma gondii by human macrophages through CD23-dependent, interleukin-10 sensitive pathway. PLoS One. 2011;6:e18289.View ArticlePubMedPubMed CentralGoogle Scholar
  38. Cong H, Yuan Q, Zhao Q, Zhao L, Yin H, Zhou H, et al. Comparative efficacy of a multi-epitope DNA vaccine via intranasal, peroral, and intramuscular delivery against lethal Toxoplasma gondii infection in mice. Parasites & vectors. 2014;7:145.View ArticleGoogle Scholar
  39. Wang HL, Zhang TE, Yin LT, Pang M, Guan L, Liu HL, et al. Partial Protective Effect of Intranasal Immunization with Recombinant Toxoplasma gondii Rhoptry Protein 17 against Toxoplasmosis in Mice. PLoS One. 2014;9:e108377.View ArticlePubMedPubMed CentralGoogle Scholar
  40. Schulthess J, Fourreau D, Darche S, Meresse B, Kasper L, Cerf-Bensussan N, et al. Mucosal immunity in Toxoplasma gondii infection. Parasite. 2008;15:389–95.View ArticlePubMedGoogle Scholar
  41. Konishi E, Nakao M. Naturally occurring immunoglobulin M antibodies: enhancement of phagocytic and microbicidal activities of human neutrophils against Toxoplasma gondii. Parasitology. 1992;104(Pt 3):427–32.View ArticlePubMedGoogle Scholar
  42. Kaneko Y, Takashima Y, Xuaun X, Igarashi I, Nagasawa H, Mikami T, et al. Natural IgM antibodies in sera from various animals but not the cat kill Toxoplasma gondii by activating the classical complement pathway. Parasitology. 2004;128:123–9.View ArticlePubMedGoogle Scholar
  43. Couper KN, Roberts CW, Brombacher F, Alexander J, Johnson LL. Toxoplasma gondii-specific immunoglobulin M limits parasite dissemination by preventing host cell invasion. Infect Immun. 2005;73:8060–8.View ArticlePubMedPubMed CentralGoogle Scholar
  44. Matowicka-Karna J, Kemona H. IgE antibodies in toxoplasmosis. Postepy Hig Med Dosw. 2014;68:597–602.View ArticleGoogle Scholar
  45. Hassan IA, Wang S, Xu L, Yan R, Song X, Li X. Immunoglobulin and cytokine changes induced following immunization with a DNA vaccine encoding Toxoplasma gondii selenium-dependent glutathione reductase protein. Exp Parasitol. 2014;146C:1–10.View ArticleGoogle Scholar
  46. Hassan IA, Wang S, Xu L, Yan R, Song X, XiangRui L. Immunological response and protection of mice immunized with plasmid encoding T. gondii glycolytic enzyme Malate Dehydrogenase. Parasite Immunol. 2014;36:674–83.View ArticlePubMedGoogle Scholar
  47. Takacs AC, Swierzy IJ, Luder CG. Interferon-gamma restricts Toxoplasma gondii development in murine skeletal muscle cells via nitric oxide production and immunity-related GTPases. PLoS One. 2012;7:e45440.View ArticlePubMedPubMed CentralGoogle Scholar
  48. Suzuki Y, Sa Q, Gehman M, Ochiai E. Interferon-gamma- and perforin-mediated immune responses for resistance against Toxoplasma gondii in the brain. Expert Rev Mol Med. 2011;13:e31.View ArticlePubMedPubMed CentralGoogle Scholar
  49. Niedelman W, Sprokholt JK, Clough B, Frickel EM, Saeij JP. Cell death of gamma interferon-stimulated human fibroblasts upon Toxoplasma gondii infection induces early parasite egress and limits parasite replication. Infect Immun. 2013;81:4341–9.View ArticlePubMedPubMed CentralGoogle Scholar
  50. Sturge CR, Yarovinsky F. Complex immune cell interplay in the gamma interferon response during Toxoplasma gondii infection. Infect Immun. 2014;82:3090–7.View ArticlePubMedPubMed CentralGoogle Scholar
  51. Tan F, Hu X, Luo FJ, Pan CW, Chen XG. Induction of protective Th1 immune responses in mice by vaccination with recombinant Toxoplasma gondii nucleoside triphosphate hydrolase-II. Vaccine. 2011;29:2742–8.View ArticlePubMedGoogle Scholar
  52. Gigley JP, Fox BA, Bzik DJ. Cell-mediated immunity to Toxoplasma gondii develops primarily by local Th1 host immune responses in the absence of parasite replication. J Immunol. 2009;182:1069–78.View ArticlePubMedPubMed CentralGoogle Scholar
  53. Yuan ZG, Zhang XX, Lin RQ, Petersen E, He S, Yu M, et al. Protective effect against toxoplasmosis in mice induced by DNA immunization with gene encoding Toxoplasma gondii ROP18. Vaccine. 2011;29:6614–9.View ArticlePubMedGoogle Scholar
  54. Song X, Gao H, Qian Y. Th17 Differentiation and Their Pro-inflammation Function. Adv Exp Med Biol. 2014;841:99–151.View ArticlePubMedGoogle Scholar
  55. Guiton R, Vasseur V, Charron S, Arias MT, Van Langendonck N, Buzoni-Gatel D, et al. Interleukin 17 receptor signaling is deleterious during Toxoplasma gondii infection in susceptible BL6 mice. J Infect Dis. 2010;202:427–35.View ArticlePubMedGoogle Scholar
  56. Kelly MN, Kolls JK, Happel K, Schwartzman JD, Schwarzenberger P, Combe C, et al. Interleukin-17/interleukin-17 receptor-mediated signaling is important for generation of an optimal polymorphonuclear response against Toxoplasma gondii infection. Infect Immun. 2005;73:617–21.View ArticlePubMedPubMed CentralGoogle Scholar
  57. Travis MA, Sheppard D. TGF-beta activation and function in immunity. Annu Rev Immunol. 2014;32:51–82.View ArticlePubMedGoogle Scholar
  58. Cekanaviciute E, Dietrich HK, Axtell RC, Williams AM, Egusquiza R, Wai KM, et al. Astrocytic TGF-beta signaling limits inflammation and reduces neuronal damage during central nervous system Toxoplasma infection. J Immunol. 2014;193:139–49.View ArticlePubMedPubMed CentralGoogle Scholar
  59. Langermans JA, Nibbering PH, Van Vuren-Van Der Hulst ME, Van Furth R. Transforming growth factor-beta suppresses interferon-gamma-induced toxoplasmastatic activity in murine macrophages by inhibition of tumour necrosis factor-alpha production. Parasite Immunol. 2001;23:169–75.View ArticlePubMedGoogle Scholar
  60. Schluter D, Bertsch D, Frei K, Hubers SB, Wiestler OD, Hof H, et al. Interferon-gamma antagonizes transforming growth factor-beta2-mediated immunosuppression in murine Toxoplasma encephalitis. J Neuroimmunol. 1998;81:38–48.View ArticlePubMedGoogle Scholar
  61. Rozenfeld C, Martinez R, Seabra S, Sant'anna C, Goncalves JG, Bozza M, et al. Toxoplasma gondii prevents neuron degeneration by interferon-gamma-activated microglia in a mechanism involving inhibition of inducible nitric oxide synthase and transforming growth factor-beta1 production by infected microglia. Am J Pathol. 2005;167:1021–31.View ArticlePubMedPubMed CentralGoogle Scholar
  62. Dupont CD, Christian DA, Selleck EM, Pepper M, Leney-Greene M, Harms Pritchard G, et al. Parasite fate and involvement of infected cells in the induction of CD4+ and CD8+ T cell responses to Toxoplasma gondii. PLoS Pathog. 2014;10:e1004047.View ArticlePubMedPubMed CentralGoogle Scholar
  63. Miceli MC, Parnes JR. The roles of CD4 and CD8 in T cell activation. Semin Immunol. 1991;3:133–41.PubMedGoogle Scholar
  64. Martini M, Testi MG, Pasetto M, Picchio MC, Innamorati G, Mazzocco M, et al. IFN-gamma-mediated upmodulation of MHC class I expression activates tumor-specific immune response in a mouse model of prostate cancer. Vaccine. 2010;28:3548–57.View ArticlePubMedGoogle Scholar
  65. Zhou F. Molecular mechanisms of IFN-gamma to up-regulate MHC class I antigen processing and presentation. Int Rev Immunol. 2009;28:239–60.View ArticlePubMedGoogle Scholar
  66. Lyons RE, Anthony JP, Ferguson DJ, Byrne N, Alexander J, Roberts F, et al. Immunological studies of chronic ocular toxoplasmosis: up-regulation of major histocompatibility complex class I and transforming growth factor beta and a protective role for interleukin-6. Infect Immun. 2001;69:2589–95.View ArticlePubMedPubMed CentralGoogle Scholar
  67. Zhao G, Zhou A, Lu G, Meng M, Sun M, Bai Y, et al. Identification and characterization of Toxoplasma gondii aspartic protease 1 as a novel vaccine candidate against toxoplasmosis. Parasites & vectors. 2013;6:175.View ArticleGoogle Scholar
  68. Chen J, Huang SY, Li ZY, Yuan ZG, Zhou DH, Petersen E, et al. Protective immunity induced by a DNA vaccine expressing eIF4A of Toxoplasma gondii against acute toxoplasmosis in mice. Vaccine. 2013;31:1734–9.View ArticlePubMedGoogle Scholar
  69. Parthasarathy S, Fong MY, Ramaswamy K, Lau YL. Protective immune response in BALB/c mice induced by DNA vaccine of the ROP8 gene of Toxoplasma gondii. AmJTrop Med Hyg. 2013;88:883–7.View ArticleGoogle Scholar

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