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Podsumowanie

Forward genetics is a powerful approach to identify genes in intracellular pathogens important for resistance to cell autonomous immunity. The current approach uses innate immune cells, specifically macrophages, to identify novel Toxoplasma gondii genes important for immune evasion.

Streszczenie

Toxoplasma gondii, the causative agent of toxoplasmosis, is an obligate intracellular protozoan pathogen. The parasite invades and replicates within virtually any warm blooded vertebrate cell type. During parasite invasion of a host cell, the parasite creates a parasitophorous vacuole (PV) that originates from the host cell membrane independent of phagocytosis within which the parasite replicates. While IFN-dependent-innate and cell mediated immunity is important for eventual control of infection, innate immune cells, including neutrophils, monocytes and dendritic cells, can also serve as vehicles for systemic dissemination of the parasite early in infection. An approach is described that utilizes the host innate immune response, in this case macrophages, in a forward genetic screen to identify parasite mutants with a fitness defect in infected macrophages following activation but normal invasion and replication in naïve macrophages. Thus, the screen isolates parasite mutants that have a specific defect in their ability to resist the effects of macrophage activation. The paper describes two broad phenotypes of mutant parasites following activation of infected macrophages: parasite stasis versus parasite degradation, often in amorphous vacuoles. The parasite mutants are then analyzed to identify the responsible parasite genes specifically important for resistance to induced mediators of cell autonomous immunity. The paper presents a general approach for the forward genetics screen that, in theory, can be modified to target parasite genes important for resistance to specific antimicrobial mediators. It also describes an approach to evaluate the specific macrophage antimicrobial mediators to which the parasite mutant is susceptible. Activation of infected macrophages can also promote parasite differentiation from the tachyzoite to bradyzoite stage that maintains chronic infection. Therefore, methodology is presented to evaluate the importance of the identified parasite gene to establishment of chronic infection.

Wprowadzenie

Toxoplasma gondii (T. gondii) is an obligate intracellular, protozoal pathogen. It is the causative agent of toxoplasmosis, a health hazard in immunocompromised individuals. It is also the model system for other apicomplexan pathogens that infect humans including Cryptosporidium and Cyclospora. Toxoplasmosis is most commonly acquired through ingestion of food or water contaminated with the bradyzoite or oocyst stage of the parasite. Upon ingestion, these stages convert to the tachyzoite stage of the parasite that replicates within host cells and disseminates systemically. T cells, IFN-γ and, to a lesser extent, nitric oxide 1-4, are important for control of infection but are not capable of eliminating the disease, as a proportion of tachyzoites convert to the bradyzoite stage that are protected within tissue cysts resulting in a long-lived chronic infection. In fact, there are no therapeutics effective against the chronic cyst stage of the disease. Severe toxoplasmosis is most often due to the reactivation of persistent infection, with the bradyzoite stage of the parasite converting back to the rapidly replicating tachyzoite stage characteristic of primary and acute infection.

Early survival in the face of the innate immune response is important to allow the parasite to reach sufficient parasite numbers, as well as to reach distal sites, to enable establishment of chronic infection. T. gondii has evolved strategies to counteract host defense mechanisms that likely contribute to its ability to replicate and disseminate early in infection. First, T. gondii forms a unique PV during parasite invasion that is largely segregated from the endocytic and exocytic processes of the host cell compared to other intracellular pathogens 5-9. Also, like all successful intracellular pathogens T. gondii modifies its host cell to create a permissive environment for growth. This includes reprogramming host cell gene expression by altering host cell transcription factors including those important for regulating cell activation 10-15. ROP16 16-19, GRA15 20, GRA16 21 and GRA24 22 have all been shown to be important in regulating the transcriptional response and cell signaling cascades of host cells infected with T. gondii. Recent studies using genetic crosses between parasite strains with distinct phenotypes have been highly productive in identifying parasite genes that underlie parasite genotype-dependent traits including evasion of immunity related GTPases (IRGs) 16,19,23-26. In mice, immunity related GTPases (IRGs) are critical for the control of Type II and III genotypes of the parasite while the very virulent Type I genotypes have evolved mechanisms to evade the murine IRGs. However, it is also clear that the parasite has evolved mechanisms to evade antimicrobial mediators in addition to the IRGs and that some of these mechanisms may be conserved across parasite genotypes 27,28. In addition, very little is known about the critical mediators of cell autonomous immunity against T. gondii during human toxoplasmosis. Parasite genes important for resistance to mediators of cell autonomous immunity may also be important for survival during tachyzoite to bradyzoite conversion which can also be triggered by host immune responses. For example, nitric oxide at high levels can suppress parasite replication in infected macrophages but it can also stimulate tachyzoite to bradyzoite conversion resulting in cyst production30-32.

ToxoDB is a functional genomic database for T. gondii that functions as a critical resource for the field in terms of providing sequence information for the parasite genome and access to published and unpublished genomic scale data including community annotations, gene expression and proteomics data 33. Similar to many protozoal pathogens, the majority of the genome consists of hypothetical genes with no information available based on gene homology to provide insight into their potential functions. Thus, forward genetics is a powerful tool to identify novel parasite genes important for immune evasion, cyst conversion and other functions critical for parasite pathogenesis as well as for conversion between distinct developmental stages. An additional strength of forward genetics is that it can be used as a relatively non-biased approach to interrogate the parasite as to the genes that are important for specific tasks in pathogenesis, including immune evasion and cyst formation. Recent improvements in next generation sequencing for mutational profiling have made it a method of choice for identifying the responsible parasite genes from forward genetics studies using both chemical and insertional mutagenesis 34-37.

It is important to identify vulnerabilities in T. gondii that can be exploited to enhance the effectiveness of cell autonomous immune mechanisms against the parasite particularly those that may also be active against the resistant cyst stage. Toward this aim, an in vitro murine macrophage infection and activation model was developed to identify mutations in the parasite that specifically impair T. gondii fitness following activation of infected macrophages but not in naïve macrophages. This macrophage screen was used to interrogate a library of T. gondii insertional mutants in order to ultimately identify T. gondii genes important for resistance to nitric oxide 27,28. The isolation of a panel of T. gondii mutants with impaired resistance to activation of infected macrophages, particularly a marked sensitivity to nitric oxide, proved the utility of the screen to identify parasite genes important for resistance to mediators of cell autonomous immunity other than the resistance mechanisms described for the murine IRGs 28. Insertional mutagenesis has advantages over chemical mutagenesis in terms of generating a limited number of random mutations in each parasite clone and, in theory, easier identification of the site of mutation. However, identifying the genomic site of plasmid insertion in T. gondii insertional mutants, in practice, has been surprisingly difficult in many cases 37. Insertion of a plasmid into a gene is also likely to disrupt the function of a gene in contrast to chemical mutagenesis that typically results in single nucleotide changes. However, chemical mutagenesis with either N-ethyl-N-nitrosourea (ENU) or ethylmethane sulfonate (EMS) may offer an increased ability to analyze a larger portion of the parasite genome, compared to insertional mutagenesis, as it creates multiple single nucleotide polymorphisms (estimated at 10 -100) per mutant34,38. Moreover, recent advances in whole genome profiling has made it possible to use next generation sequencing to identify the most likely candidate genes responsible for the identified phenotype of a mutated parasite 34,38. Regardless of the mutagenesis approach, confirmation of the role of the parasite gene in resistance to macrophage activation ultimately requires gene deletion and complementation to fulfill molecular Koch’s postulates.

The ability to dissect the function of a gene by genetic manipulation of both the parasite and the macrophage is important as many of the genes identified via forward genetics in T. gondii, as well as other pathogens, are still characterized as hypothetical genes with little to no sequence homology to other proteins with known functions. The current paper outlines a general approach that can be used to identify whether the disrupted gene in a mutant is important for resistance to a known or unknown mediator of cell autonomous immunity. The initial analysis of host antimicrobial factors is performed by evaluating the survival of wild type and mutant parasites in macrophages from wild type mice versus those with specific gene deletions in inducible nitric oxide synthase (iNOS), gp-91 phox (NADPH oxidase), and specific immunity related GTPases (IRGs). This will determine if the identified parasite genes are important for resistance to nitric oxide, reactive oxygen intermediates or immunity related GTPases 28 respectively or if an unknown immune mechanism is involved. Activation of infected macrophages with both IFN-γ and LPS, described in the current protocol, results primarily in the isolation of parasite genes important for resistance to nitric oxide 28. The use of pharmacological agents that induce nitric oxide in the absence of macrophage activation (nitric oxide donors) confirmed that the majority of the genes identified were important for resistance to nitric oxide rather than nitric oxide in concert with additional mediators associated with macrophage activation 28.

Step one and two describe a forward genetics screen designed to isolate parasite mutants with a fitness defect following activation of infected bone marrow-derived macrophages in vitro. Step one describes a dose titration analysis to empirically determine a dose of IFN- γ  and LPS to use for macrophage activation that reduces parasite replication but does not fully inhibit replication of the wild type T. gondii parental strain that is used for creation of the library of parasite mutants. Step two describes the forward genetic screen of the mutant clones in macrophages in 96-well plates. Step three outlines an approach to confirm the phenotype of each mutant identified in the screen of the 96 well plates and to evaluate whether the defect in each mutant affects parasite survival, replication, or cyst production in response to macrophage activation. Step four describes the use of bone marrow-derived macrophages from mice with deletions in specific antimicrobial pathways to identify the immune mediators to which the parasite mutant is specifically susceptible. Step five outlines an approach to determine if a parasite mutant is also compromised for in vivo pathogenesis as evaluated by cyst production in the brains of infected mice.

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Protokół

NOTE: All protocols that involve the use of animals were performed in accordance with the guidelines and regulations set forth by the New York Medical College’s Animal Care and Use Committee.
NOTE: Detailed protocols for chemical mutagenesis 38, isolation of parasites by limiting dilution 38, isolation of murine bone marrow derived macrophages 39, growth of T. gondii in human foreskin fibroblast (HFF) cells and cyst production in macrophages and basic immunofluorescence analysis (IFA) 32 are referenced. Carry out all cell culture at 37 °C in 5% CO2 in D10 media (Dulbecco’s Modified High Glucose Eagle Medium supplemented with 10% fetal calf serum, 2 mM L-glutamine, 100 U/ml penicillin and 100 µg/ml streptomycin). Keep all reagents sterile throughout cell isolations and cell culture.

1. Dose Titration of IFN-γ and LPS to Determine the Concentrations to Use to Activate Infected Macrophages for the Forward Genetics Screen

  1. Culture murine bone marrow-derived macrophages O/N in eight chamber glass slides at a concentration of 3 × 105 cells/ml in 250 μl of D10 media per chamber. Use macrophages one to two-weeks after isolation from bone marrow.
    NOTE: Chamber slides are purchased that have a growth enhancing RS wash.
  2. Use a hemocytometer to count wild type parasites harvested from human foreskin fibroblast (HFF) cells grown in a T25 tissue culture flask. Resuspend parasites at a concentration of 5 x 105 wild type parasites per ml in D10 media. This concentration will result in a multiplicity of infection of approximately 1:1 as the macrophages will have proliferated O/N . Use polystyrene or PET tubes for all manipulations with parasites as the parasite sticks to polypropylene.
  3. Remove the D10 media in the chamber slides and replace with 250 μl of the suspension of wild type parasites. Gently add the parasite suspension to each chamber of the slide by allowing it to flow down the inner face of each chamber. Do not allow macrophages to dry out at any point during the protocol.
  4. Cover chamber slides infected with parasites with the chamber slide cover and place in an incubator at 37 ° C in 5% CO2 for 4 hr to allow time for the parasite to invade and establish a PV.
  5. Make dilutions of LPS and IFN-γ in 1 ml of D10 media in sterile tubes for the dose titrations. For dose titrations keep either LPS or IFN- concentration constant and vary the other stimulus 40.
    1. For example, keep LPS constant at 10 ng LPS per ml and vary the concentration of IFN- γ (0, 1 unit/ml, 10 units/ml, 100 units/ml, 1,000 units/ml). Keep IFN- γ constant at 100 units/ml and vary the concentration of LPS (0, 0.1 ng/ml, 1 ng/ml, 10 ng/ml, 100 ng/ml). Briefly sonicate LPS stock for 2 min without heating in a bath sonicator (not with a tip sonicator) prior to dilution.
      NOTE: Sonication is recommended to disrupt micelle aggregates formed by LPS that may not bind properly to host cells.
  6. 4 hr after initiation of co-culture between the parasites and adherent macrophages in the chamber slide, discard the D10 media in each chamber and replace it with 300 μl of the appropriate dilutions of IFN- γ and LPS in D10 media. Include a control with only D10 media to evaluate parasite replication in the absence of macrophage activation.
  7. Re-cover chamber slides with the chamber slide cover and place in an incubator at 37 ° C in 5% CO2 for 24 to 30 additional hr.
    NOTE: Incubation time depends on the doubling time of the wild type parasite strain that can range from 6-12 hr depending on the parasite strain. A time point is chosen prior to parasite lysis of naïve macrophages but long enough to enable at least 3-4 doubling times.
  8. Make a 2.5% formaldehyde solution in Dulbecco’s phosphate buffered saline (PBS). Discard the media in the chamber slide and replace with 300 μl of the 2.5% formaldehyde solution. Fix for 20 min at RT.
  9. Rinse slide(s) twice with 300 μl of PBS per chamber. For each rinse, discard the PBS in the slide and add new PBS gently down the inner face of each slide chamber to avoid disrupting the macrophages adhered to the slide. Add 300 μl of PBS per chamber and place cover on chamber slide to prevent slides from drying out prior to staining.
    NOTE: Slides can be placed at 4 C for up to 3 days at this point prior to staining.
  10. Staining protocol for T. gondii detection by immunofluorescence microscopy (IFA).
    1. Make a 0.2% Triton X-100 solution in PBS (permeabilization buffer). Place the solution in a tube in a 37 °C water bath and briefly vortex it to ensure the Triton X-100 goes into solution. Discard the PBS in the chamber slides and replace with 300 μl of the permeabilization buffer. Leave at RT for 30 min.
    2. Make a solution of 10% goat serum in PBS (blocking solution). Discard the permeabilization buffer in the slide and replace with 300 μl of blocking solution per chamber. Leave at RT for 30 min.
      NOTE: Fetal calf serum can be substituted for goat serum in all staining protocols.
    3. For a one step IFA staining protocol, make a 1:1,000 dilution of a fluorescently-conjugated antibody to T. gondii in blocking solution. Remove blocking solution from slide and add 150 μl of antibody solution per chamber. Replace cover slide on chamber slide to prevent cells from drying out. Incubate for 1 hr at RT .
      NOTE: Antibody concentration must be empirically determined depending on the source. Antibody is purchased directly conjugated to a fluorochrome or conjugated to a fluorochrome by the user.
      1. For a two-step IFA staining protocol with an unconjugated antibody to T. gondii and a fluorescently conjugated secondary antibody, stain slides with 150 μl of unconjugated primary antibody against T. gondii in blocking buffer for 1 hr at RT . Rinse 3x with 300 μl of PBS plus 1% goat serum (wash buffer).
      2. Add 150 μl of fluorescently-conjugated secondary antibody specific for the species of origin for the primary antibody. Replace cover slide on chamber slide to prevent cells from drying out. Incubate for 1 hr at RT .
    4. Rinse slides 3x with PBS plus 1% goat serum (washing buffer). For each rinse, remove the solution in the chamber slides by dumping out its contents and replace with 300 μl of washing buffer.
    5. Rinse slides 2x with 300 μl of PBS.
    6. Remove the chamber from the chamber slide as per manufacturer’s instructions.
    7. Mount slides with mounting media containing DAPI (4’6-diamidino-2-phenylindole, dilactate) and a 22 mm x 50 mm coverslip.
  11. Examine slides using phase contrast and fluorescence microscopy. Determine the average number of parasites per vacuole by examining a minimum of 100 PVs per chamber well. The chosen dose of IFN- γ and LPS for the screen needs to be sufficient to suppress, but not prevent, replication of wild type parasites (see Figure 1).

2. Isolation of Parasite Mutants with a Fitness Defect Following Activation of Infected Macrophages

NOTE: A library of random T. gondii mutants is required for the forward genetics screen. Random mutagenesis of T. gondii can be performed by chemical (ENU/EMS) or insertional mutagenesis 27,28,38. Following mutagenesis, clone parasites by limiting dilution and grow individual clones in 96-well plates containing adherent HFF cells in a volume of 200 µl of D10 media 32,38. It is critical that 96-well plates for screening of parasites in macrophages by microscopy have optical bottoms to enable microscopic screening. Phase contrast and fluorescence microscopy for screening stained 96-well plates requires an inverted fluorescence microscope with phase contrast 4, 10, 20 or 40X objective equipped for long working distances. A 4X objective is useful for seeing the entire well but better resolution of the parasites is achieved with the 20X objective.

  1. Transfer 50 µl of tachyzoite mutants grown in confluent HFF cells in 96-well tissue culture plates into two replicate 96-well plates containing murine bone marrow-derived macrophages (1-2 weeks after isolation) in 100 µl of D10 media.
    NOTE: Perform the initial screen in 96-well plates of the parasite based on volume of parasite culture to avoid having to count the number of parasites transferred per each well. Thus, the microscopy analysis in 2.6 is based qualitatively on whether parasites have generally replicated or not replicated. Step 3 describes the approach to confirm the phenotype of the mutants in chamber slides using equal numbers of wild type or mutant parasites to infect the macrophages.
    1. Directly add parasites to the D10 media already in each well. Infect two wells with wild type tachyzoites as a positive control for parasite replication.
  2. Place the infected cells into an incubator (37 ° C and 5% CO2) for 4 hr to allow parasites time to invade the cells and create their PV.
  3. Remove media from one plate by dumping the contents of the plate. Use a single flip of the wrist to dump the media in the plate into a discard basin containing a detergent cidal for the parasites.
    1. Add 100 µl of “macrophage activation media” using a sterile basin for the media and a multichannel pipette. Use the optimal concentration of LPS and IFN-γ determined from Step 1 for the macrophage activation media. Similarly remove media from the duplicate control plate and replace with 100 µl of D10 media.
  4. Place the infected cells into an incubator (37 ° C and 5% CO2) for an additional 24-30 hr.
  5. Staining protocol for 96-well plates for IFA.
    1. Discard the media in the plate and replace with 100 µl of 2.5% formaldehyde in PBS. Incubate for 20 min at RT . Use a sterile basin for the formaldehyde and a multichannel pipette.
    2. Discard the formaldehyde solution in the plate and add 100 µl PBS to rinse the formaldehyde from the plate.
    3. Discard the solution in the plate and add 100 µl of permeabilization buffer (PBS with 0.2% Triton X-100) to each well. Incubate for 30 min at RT .
    4. Discard the solution in the plate and add 100 µl of blocking solution (PBS with 10% goat serum) to each well. Incubate for 30 min at RT .
    5. Discard the solution in the plate. Add 50 µl/well of a fluorescently-conjugated anti-T. gondii antibody diluted 1:1,000 in PBS plus 1% goat serum. Incubate for 1 hr at RT with the plate cover on and on a rocker.
      1. Alternatively use an unconjugated primary antibody against T. gondii followed by staining with a fluorescently-conjugated secondary antibody as described in 1.10.3.1.
    6. Discard the antibody solution in the plate and replace with 100 µl/well of PBS plus 1% goat serum. Perform this rinse 3x followed by 2 additional rinses with PBS alone. Leave 200 µl of PBS in each well and replace the cover on the 96 well plate to prevent the wells from drying.
      NOTE: The plate with the cover on can be wrapped in parafilm and placed at 4 ° C for up to 3 days prior to analysis by microscopy.
  6. Examine cells under an inverted fluorescent microscope using a 20-40X objective. Select mutants that replicate in the naïve macrophage plate but predominantly fail to replicate beyond one parasite/vacuole in “activated macrophages” or that appear amorphous or degraded in “activated macrophages”.
    NOTE: The number of wild type parasites per vacuole will depend on the dose of IFN-γ and LPS used but ideally is around 4 parasites per vacuole; a number that reflects growth suppression but not complete inhibition of replication by the activation stimulus.

3. Evaluate the Mutants to Determine if the Defect is at the Level of Parasite Survival or Replication Following Activation of Infected Macrophages

  1. Transfer selected parasite mutants from 96-well plates (contents of entire well) to T25s containing HFF cells and allow replication.
  2. Culture bone marrow derived macrophages O/N in 8 chamber glass slides at a concentration of 3 × 105 cells/ml in 250 μl of D10 media. Prepare one slide to compare parasite replication in naïve macrophages and an additional slide to compare parasite replication following activation of infected macrophages.
  3. Harvest tachyzoite parasites and count in a hemocytometer. Add 5 × 104 T. gondii parasites to a chamber well containing macrophages in D10 media and culture for 4 hr. Include one well with wild type parental parasites as a control. Inoculate an identical replicate slide with the same parasite clone that will not receive activation media in order to monitor replication of parasites in naïve macrophages.
  4. Discard D10 media from 1 of the replicate chamber slides and replace with 250 µl of “activation media”. Discard D10 media from the other replicate chamber slide and replace with 250 µl of D10 media. Incubate both the “activated” and “naïve” macrophage slide with the chamber slide cover on at 37 ° C and 5% CO2 for an additional 24-30 hr.
  5. Fix, permeabilize, and block slides for IFA staining and analysis of parasites as described in Step 1. Perform IFA staining with the chambers intact.
    1. Co-stain cells with an antibody to lysosomal membrane associated 1 (LAMP1) or Lysotracker and antibody to T. gondii to evaluate whether activation of infected macrophages is triggering fusion of the mutant PVs with lysosomes (Figure 4).
    2. Use antibodies to specific compartments/organelles within the parasite/PV for staining by IFA to identify alterations in the parasite mutant that are evident early following macrophage activation 28.
      NOTE: Such alterations may provide insight into the mechanism that underlies the deficient survival/replication of the mutant following macrophage activation.
  6. Examine slides using a 100X phase oil objective and fluorescence microscopy.
    1. Evaluate parasite replication by determining the number of parasites per PV in 100 random vacuoles. Perform at least 2 counts of 100 vacuoles each for statistical analysis.
    2. Evaluate general parasite morphology using both fluorescence analysis as well as phase contrast microscopy. View parasites under phase 100x objective. Healthy parasites have parasites tightly enclosed within a close-fitting parasitophorous vacuole. Parasites that have amorphous spacious vacuoles with phase dense rims or amorphous parasites suggest parasite death rather than just a defect in replication (Figures 1 and 3).

4. Evaluate whether the Susceptibility of Mutant Parasites to Activation of Infected Macrophages is Associated with Known Anti-microbial Mediators

  1. Isolate bone marrow-derived macrophages from wild type C57/BL6 mice, iNOS-/-, gp91-phox-/- or Irgm1/Irgm3-/- mice 32.
  2. Culture respective bone marrow derived macrophages O/N in 8 chamber glass slides at a concentration of 3 × 105 cells/ml in 250 μl of D10 media.
  3. Proceed with parasite challenge, IFA staining, and analysis as described in Step 3.
  4. Determine if the ability of the mutant parasites to survive and replicate following activation of infected macrophages is restored in the absence of reactive oxygen or nitrogen species or specific immunity related GTPases 28.
  5. Use pharmacological agents, such as nitric oxide donors, to evaluate whether specific anti-microbial mediators are sufficient by themselves to impair mutant parasites in HFF cells or naïve macrophages or if they only act in concert with other mediators of macrophages activation 28.

5. Evaluate whether the Defect in the Mutant Parasite Compromises Chronic Infection

  1. Isolate tachyzoites from wild type, mutant or targeted gene deleted parasites grown in T25s containing HFF cells. Parasites must be freshly lysed from HFF cultures.
  2. Count parasites using a hemocytometer. Resuspend parasites in Hanks balanced salt solution (HBSS) at a concentration per ml appropriate for a sub-lethal dose of the parasite delivered in 200 μl by intraperitoneal (IP) injection.
  3. Use a 1 ml tuberculin syringe and 25 G needle to inject parasites with a 200 μl volume intraperitoneally (IP). The dose depends on the wild type strain of the parasite and the mouse genotype.
    NOTE: Type I genotypes of the parasite are lethal to mice during the acute stage of infection regardless of parasite dose and are not appropriate for studies of chronic infection in the absence of chemotherapy for T. gondii to suppress parasite replication.
  4. Thirty days after parasite challenge, sacrifice mice by inhalation of CO2 from a pressurized tank in an uncrowded chamber (a standard size mouse cage may contain no more than 5 mice) followed by cervical dislocation.
  5. Isolate the brain from the mouse using established procedures41-43.
    1. Lay the mouse on its front side. Spray the head with 70% ethanol to sterilize the area.
    2. Use sharp scissors to cut through the brain stem. Use dissecting scissors to make a shallow cut laterally around the right and then the left side of the skull starting from the base of the brain stem. Use forceps to gently peel back the skull to expose the brain.
    3. Gently lift the brain and place scissors between the brain and base of the skull to cut the olfactory nerve to free the brain. Lift out the brain with sterile forceps or a spatula and place in a bacteriological Petri plate containing 10 ml of sterile PBS.
  6. Cut the brain in half with a sterile scalpel through the center between the right and left hemispheres.
  7. Add half of the brain to a small mortar containing 1 ml of PBS. Use the mortar and pestle to make a fine tissue suspension of the brain that can pass through a wide bore 20-200 μl pipette tip.
    NOTE: The other half of the brain should be fixed in 2.5% formaldehyde for 1 hr if tissue sections are needed for histopathology.
  8. Place 100 μl of the brain lysate in a 1.7 ml microcentrifuge tube. Add 1 ml of 2.5% formaldehyde in PBS into the tube containing the brain lysate to fix the brain suspension for staining. Incubate at RT for 30 min.
  9. Centrifuge the lysate at 8,000 x g for 5 min in a microcentrifuge and carefully discard the supernatant.
  10. Add 1 ml of permeabilization/blocking buffer to the lysate (10% goat serum, 0.2% Triton X-100 in PBS). Incubate at RT for 30 min.
  11. Centrifuge lysate at 8,000 x g for 5 min and remove supernatant.
  12. Add 200 μl of FITC-conjugated dolichos biflorus agglutin (DBA). Use a 1:100 dilution of the lectin in PBS plus 10% goat serum. Gently resuspend the lysate by pipetting. Incubate for 1 hr at RT .
    NOTE: DBA is a ligand that binds to CST1 on the parasite cyst wall.
  13. Centrifuge lysate at 8,000 x g for 5 min and discard supernatant. Add 1 ml of PBS to the pellet. Incubate at RT for 5 min. Repeat PBS wash 3x. Remove the supernatant following the final wash using a pipette.
  14. Use a wide bore 20-200 μl pipette tip to draw up 5 μl of the stained brain lysate and place on a microscope slide. Mount the slide with a 25 x 25 mm cover slip to create a wet mount of the brain lysate. Make 3 replicate slides using 5 μl of brain lysate each.
  15. Count the number of cysts per each 5 μl aliquot by fluorescence microscopy using a 10X objective (Figure 6).
    NOTE: Some cysts are large (8 or more parasites approximately) while some are very small (1-2 parasites per cyst). Count total number of cysts per each slide but document number of large versus number of small cysts.
  16. Add the number of cysts detected in the three different 5 µl aliquots and multiply by the total dilution factor x 2 (only half of the brain was made into a lysate) to estimate the number of total cysts per brain.

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Wyniki

Toxoplasma gondii replicates freely in naïve macrophages and has a doubling time between 6-12 hr depending on the strain of the parasite. Figure 1 shows representative parasites in naïve versus activated bone marrow-derived macrophages. Figure 2 shows the general morphology of parasites in HFF host cells at 2, 4, 8, 16 and 32 parasites/PV. In the current protocol, the parasite is allowed to invade naïve macrophages and establish a nascent parasitophorous vacu...

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Dyskusje

The described protocol provides a non-biased approach that uses activation of murine bone marrow-derived macrophages and forward genetics to isolate T. gondii mutants with a defect in their ability to survive activation of infected macrophages. The phenotype of the mutants following macrophage activation typically falls into one of two broad categories: 1) The parasites appear intact but fail to replicate beyond 1 parasite per PV; 2) The parasites appear degraded and may be in spacious, amorphous PVs. The fact t...

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Ujawnienia

The authors have no competing financial interests.

Podziękowania

Special thanks to Dr. Peter Bradley for the antibody to detect the T. gondii mitochondria. The work was supported by National Institute of Health Grants AI072028 and AI107431 to D.G.M and a generous donation to New York Medical College for the study of tropical medicine.

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Odniesienia

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