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In This Article

  • Summary
  • Abstract
  • Introduction
  • Protocol
  • Results
  • Discussion
  • Disclosures
  • Acknowledgements
  • Materials
  • References
  • Reprints and Permissions

Summary

All pathogenic Leishmania species reside and replicate inside macrophages of their vertebrate hosts. Here, we present a protocol to infect murine bone marrow-derived macrophages in culture with Leishmania, followed by precise quantification of intracellular growth kinetics. This method is useful for studying individual factors influencing host-pathogen interaction and Leishmania virulence.

Abstract

The lifecycle of Leishmania, the causative agent of leishmaniasis, alternates between promastigote and amastigote stages inside the insect and vertebrate hosts, respectively. While pathogenic symptoms of leishmaniasis can vary widely, from benign cutaneous lesions to highly fatal visceral disease forms depending on the infective species, all Leishmania species reside inside host macrophages during the vertebrate stage of their lifecycle. Leishmania infectivity is therefore directly related to its ability to invade, survive and replicate within parasitophorous vacuoles (PVs) inside macrophages. Thus, assessing the parasite's ability to replicate intracellularly serves as a dependable method for determining virulence. Studying leishmaniasis development using animal models is time-consuming, tedious and often difficult, particularly with the pathogenically important visceral forms. We describe here a methodology to follow the intracellular development of Leishmania in bone marrow-derived macrophages (BMMs). Intracellular parasite numbers are determined at 24 h intervals for 72 - 96 h following infection. This method allows for a reliable determination of the effects of various genetic factors on Leishmania virulence. As an example, we show how a single allele deletion of the Leishmania Mitochondrial Iron Transporter gene (LMIT1) impairs the ability of the Leishmania amazonensis mutant strain LMIT1/ΔLmit1 to grow inside BMMs, reflecting a drastic reduction in virulence compared to wild-type. This assay also allows precise control of experimental conditions, which can be individually manipulated to analyze the influence of various factors (nutrients, reactive oxygen species, etc.) on the host-pathogen interaction. Therefore, the appropriate execution and quantification of BMM infection studies provide a non-invasive, rapid, economical, safe and reliable alternative to conventional animal model studies.

Introduction

Leishmaniasis refers to a broad spectrum of human diseases caused by protozoan parasite species of the genus Leishmania. Approximately 12 million people are currently infected with Leishmania worldwide, and more than 350 million are at risk. The disease pathology depends on the Leishmania species and on host factors, and symptoms vary from innocuous self-healing skin lesions to lethal visceralizing forms. If untreated, visceral leishmaniasis is fatal, ranking only after malaria as the deadliest human disease caused by infection with a protozoan parasite1. In spite of the wide-ranging differences in disease pathology and symptoms, all Leishmania species have a digenic life-cycle alternating between promastigote and amastigote stages inside insect and vertebrate hosts, respectively. Inside vertebrates, Leishmania target host macrophages for invasion and induce the formation of parasitophorous vacuoles (PVs), acidic compartments with properties of phagolysosomes where the highly virulent amastigote forms replicate. Amastigotes persist in host tissues during chronic infections and can be passed forward to uninfected sandflies, completing the transmission cycle. Therefore, in the context of human disease development, amastigotes are the most important Leishmania lifecycle form2. Investigating how amastigotes replicate inside macrophage PVs is critical for understanding Leishmania virulence3,4,5,6,7 and for the development of novel efficacious therapies.

We describe here a method regularly used by our laboratory to study Leishmania infection and replication in bone marrow-derived macrophages (BMMs), which involves quantitative assessment of the number of intracellular Leishmania over time. The process involves harvesting of monocytes from mouse bone marrow and differentiation to macrophages in culture, in vitro infection with infective forms (metacyclic promastigotes or amastigotes) of Leishmania and quantification of the number of intracellular parasites at every 24 h interval for a period of 72 - 96 h following infection. This assay has been used in our laboratory to determine the impact of several environmental factors and parasite genes, including identification of the critical role of iron in promoting L. amazonensis virulence that was further validated by footpad lesion development studies in mice6,8,9,10,11,12,13,14,15. Since all pathogenic Leishmania species establish their replicative niche inside host macrophages, this assay can be used universally for virulence determinations in all Leishmania species.

Performing BMM infections allows analysis of host-parasite interactions at the single cell level, and thus a more extensive understanding of how Leishmania parasites interact with their preferred host microenvironment, the PVs of macrophages. Macrophage infection assays have been successfully used by multiple groups16,17,18,19,20,21,22 to explore functions of both the host macrophage and Leishmania specific genes, and their potential involvement in the complex interplay that characterizes intracellular infection. BMM infections allow quantification of parasite growth as a read-out of the impact of host factors that influence intracellular survival, such as microbicidal nitric oxide production, generation of reactive oxygen species and other adverse conditions encountered inside the lysosome-like PVs23. Macrophage infection assays have also been utilized to identify potential anti-leishmanial drug leads for therapeutic development13,24.

The in vitro nature of BMM infections provides several advantages over other methods to assess Leishmania virulence. However, several previous studies examining mechanisms of intracellular parasite survival over time did not quantify infection as a rate20,21,24. Furthermore, many studies focused on following in vivo infections over time did so by measuring cutaneous lesion size and other physiological symptoms that are only indirectly related to parasite replication25,26,27. In vivo infection is a stringent approach to assess parasite virulence, but lesion size measurements based on footpad swelling alone are often inadequate, as they reflect the inflammatory response in infected tissues and not the absolute number of parasites. For this reason, footpad lesion development assays have to be followed by quantification of the parasite load in infected tissues, a procedure that requires lengthy limiting dilution assays28. Additionally, in vivo studies often involve sacrificing multiple animals at different points in time to extract tissues of interest6,8,9,10,11,13. In contrast, large numbers of BMMs can be obtained from just one animal, and these cells can be plated under conditions that allow assessment of infection at various points in time. Furthermore, compared to in vivo studies, performing in vitro BMM infections allows greater control over experimental conditions. Quantifying the macrophages to be infected along with the parasites themselves allows precise control of the multiplicity of infection (MOI) and of culture conditions. Fine control over these factors can be key in identifying characteristics of discrete cellular pathways and in understanding their impact on the course of infection.

Given these advantages, it is somewhat surprising that very few groups studying Leishmania virulence have so far taken full advantage of quantitative assessment of intracellular replication in macrophages. In this article, we discuss common pitfalls that may be hampering the more extensive utilization of this assay, and provide a step-by-step protocol to facilitate its proper implementation. Considering its precision and versatility, the BMM infection assay we describe here can not only be utilized to explore host-pathogen interactions influencing Leishmania virulence, but also to study other microorganisms that replicate inside macrophages29. Importantly, this assay can also be developed as a rapid and economical pre-clinical screening method for anti-leishmanial drug development.

Protocol

All experimental procedures were conducted in accordance with the recommendations in the Guide for the Care and Use of Laboratory Animals by the National Institutes of Health and were approved by University of Maryland's IACUC. All steps described in sections 1 through 4 should be carried out aseptically inside biological laminar flow cabinets. Personal protection should be used, and caution should be exercised during handling of live Leishmania parasites throughout all stages of experimentation.

1. Isolation and Differentiation of Bone Marrow-derived Macrophages (BMMs)8,30,31

  1. Day 0: Sacrifice 4 - 6-week-old female C57BL/6 or BALB/c mouse in a CO2 chamber and confirm death via cervical dislocation. Ensure sterilization of scissors and forceps by keeping them soaked in 70% ethanol. Spray gloves with 70% ethanol to allow sterile handling throughout the bone marrow cell isolation process.
  2. Secure sacrificed mouse to dissection board by pinning its forelimbs and disinfect by spraying copiously with 70% ethanol.
  3. Make a small incision (about 1 cm) with scissors near the hip joint. Carefully insert scissors under the skin to separate the underlying muscle and cut the skin all the way around the hip joint.
    NOTE: The dissection board may be rotated to allow improved access to the hip joint.
  4. Carefully deglove skin from the leg by pulling towards the ankle and remove. Cut the foot off at the ankle, being very careful to cut at or below the ankle joint to leave the tibia fully intact.
    NOTE: The fibula at this stage is loosely attached and can be easily separated with the forceps.
  5. Manually locate the hip joint by manipulating the femur to identify the point of rotation. Carefully use scissors to sever the leg above the hip joint to leave the proximal head of the femur intact.
  6. Remove as much muscle and connective tissue as possible from the leg with scissors. Remove any remaining skin from the ankle and any excess bone material above the hip joint.
  7. Place the cleaned leg bones in sterile RPMI supplemented with penicillin/streptomycin (1% final concentration) in a Petri dish on ice.
  8. Repeat steps 1.4 through 1.6 to isolate tibia and femur from the other hind leg.
  9. Remove any remaining muscle and connective tissue from the bones soaking in RPMI using sterilized forceps and sterile #10 blade.
  10. Place bones on the Petri dish lid. Cut the tibia carefully with the blade immediately above the ankle joint to access the marrow. Remove the tibia from the rest of the leg by cutting immediately below the knee joint.
  11. Draw 10 mL sterile RPMI supplemented with penicillin/streptomycin (1% final concentration) into a 10-mL syringe and attach a 25G needle.
  12. Hold the tibia firmly with forceps, vertically over a 50-mL conical tube on ice. Use the syringe to gently inject approximately 5 mL RPMI into the end of the bone to flush the bone marrow out of the other end into the conical tube. Flush the bone marrow with a total of 10 mL RPMI until the bone turns white.
    NOTE: After thorough flushing, the bone should turn white. If not, continue flushing to remove marrow. The distal end of the tibia may need to be trimmed back with the blade if it is too narrow to insert the needle.
  13. Cut the femur immediately above the knee joint and immediately below the hip joint to expose both ends of the bone to access the marrow. Flush bone marrow from the femur with a total of 10 mL RPMI in the same fashion as the tibia.
  14. Repeat cleaning and flushing steps 1.6 through 1.13 with the remaining bones and collect the bone marrow flushed cells in a single 50 mL conical tube
    NOTE: If a bone breaks at any point during dissection prior to bone flushing, do not use the marrow from this bone.
  15. Centrifuge the conical tube used to collect bone marrow flushed from all four bones for 10 min at 4 °C at 300 x g.
  16. Place 60 mL of sterile BMM medium (RPMI with a final concentration of 20% FBS, 1% penicillin/streptomycin, 1.2 mM Na-pyruvate, 25 µg/mL human M-CSF) into a 175 cm2 cell culture flask with filter cap.
  17. Discard the supernatant following centrifugation and resuspend the cell pellet by gentle up and down pipetting using 5 mL of BMM medium from the flask.
  18. Transfer cell suspension to the culture flask and rinse the conical tube twice with BMM medium from the culture flask to ensure maximal cell recovery. Ensure cell suspension is thoroughly mixed into medium and distribute 30 mL from the initial 175 cm2 cell culture flask to a second 175 cm2 cell culture flask with filter cap.
  19. Incubate both flasks containing 30 mL cell suspension each overnight at 37 °C, 5% CO2 to allow separation of any contaminating fibroblasts, resident macrophages, and other adherent cells.
  20. DAY 1: Transfer the supernatant containing undifferentiated bone marrow cells from flasks to 100 mm x 15 mm non-TC-treated polystyrene Petri dishes at approximately 10 mL/dish and incubate at 37 °C, 5% CO2. Discard the flasks.
  21. DAY 3 or 4: Add an additional 5 mL BMM medium (pre-warmed to 37 °C) to each Petri dish and continue incubation at 37 °C, 5% CO2.

2. Plating BMMs on Coverslips for Infection (DAY 7 or 8)

  1. Prepare 6-well tissue culture plates by placing four (4) sterile 12 mm glass coverslips (autoclaved and stored in a closed glass container) in the bottom of each empty well.
    NOTE: Pick each sterile 12 mm coverslip up with an aspirating tip fitted to a vacuum line. Place coverslips into the wells without overlap, releasing at the desired position by pinching the tube to interrupt vacuum.
  2. Aspirate media (and any non-adherent cells) from Petri dishes coated with adherent bone marrow derived macrophages and gently rinse adherent cells 2x with sterile Dulbecco's Phosphate buffered saline without calcium and magnesium chloride (PBS -/-) pre-warmed to 37 °C.
  3. Add dropwise, 5 mL sterile 1x PBS -/- with a final concentration of 1 mM EDTA to each Petri dish and incubate for 5 min at 37 °C to detach adherent BMMs. Verify that the cells are detached using a microscope.
  4. Collect all detached cells suspended in 1x PBS -/- supplemented with 1 mM EDTA in a 50 mL conical tube. Rinse each dish 2x with 5 mL PBS -/- and add to cell suspension pool.
    NOTE: Cell suspension may be diluted with additional PBS -/- to protect macrophages from EDTA toxicity during the collection process.
  5. Centrifuge at 300 x g for 10 min at 4 °C. Discard supernatant and resuspend macrophages in 5 - 10 mL BMM medium by pipetting. Place resuspended cells on ice to prevent attachment to tubes and clumping.
  6. Count viable cells using Trypan blue exclusion in the hemocytometer.
    NOTE: To count BMM cells resuspended in 5 mL medium, a dilution-mix of 25 µL cell suspension in 445 µL PBS -/- and 30 µL 0.4% Trypan blue solution typically allows easy quantification in a hemocytometer (taking into account a 20x dilution factor for the final calculation). Count only cells that did not get stained with Trypan blue (viable cells). The volume of cell suspension may be altered if this mixture is too concentrated or diluted. In general, the yield of BMM per preparation varies between 2 x 107 and 5 x 107 cells from a single mouse.
  7. Prepare the cell suspension in BMM medium at desired plating concentration (5 x 105/mL) and disperse suspension to 6 well plates in 2 mL medium per well so that each well receives 1 x 106 macrophages.
    NOTE: This is a critical step that ensures every well gets the adequate number of macrophages to cover the coverslips uniformly. Check that coverslips in wells are not overlapping or floating in the medium. If so, gently adjust with a sterile pipette tip.
  8. Incubate overnight at 37 °C, 5% CO2.

3. Purification of Infective Forms of L. amazonensis

NOTE: Prepare Leishmania for infections- purify metacyclic promastigotes from stationary promastigote cultures8,13, or differentiate promastigotes in culture into amastigote form using standard L. amazonensis axenic differentiation protocol6,8.

  1. Purification of Leishmania metacyclic promastigotes using density gradient media(Materials)33
    1. Prepare 40% stock solution of density gradient media in sterile, endotoxin-free water.
    2. Dilute density gradient solution in 10x M199 medium (without serum) to prepare 10% concentration in the M199 medium.
    3. Filter all solutions through 0.22 µm filter.
      NOTE: Stock solutions can be stored at 4 oC in darkness for no longer than 1 month.
    4. Add 2 mL of 40% density gradient media solution in the bottom of a 15-mL conical centrifuge tube.
    5. Layer 2 mL of 10% density gradient media solution in M199 on top of the 40% density gradient media layer carefully, using a Pasteur pipette to avoid any mixing between the two layers.
    6. Collect 1 x 109 parasites from stationary-phase culture by centrifugation at 1,900 x g for 10 min.
    7. Resuspend cells in 6 mL Dulbecco's Modified Essential Medium (DMEM).
    8. Layer 2 mL of the cell suspension directly on top of the 10% density gradient media layer, gently, using a Pasteur pipette to avoid mixing between layers.
    9. Centrifuge the gradient for 10 min at 1,300 x g at room temperature.
      NOTE: Due to differences in physical properties between Leishmania species, centrifugation conditions for each might have to be slightly adjusted to ensure maximum yield.
    10. Collect parasites (enriched in metacyclic promastigote form) from the band formed at the upper 10% density gradient media boundary (interface between the 0% and 10% density gradient media layers).
    11. Dilute parasites with one volume of DMEM and collect by centrifugation (1,900 x g for 10 min at room temperature).
    12. Resuspend in 500 µL DMEM medium and count in a hemocytometer to quantify yield.
  2. Generation of L. amazonensis amastigotes under axenic culture conditions (low pH / elevated temperature)6,8,13
    1. Mix 5 mL of log-phase promastigote culture (pH 7.4 at 26 oC) with an equal volume of amastigote medium (pH 4.5), using 25 cm2 flasks (total 10 mL medium) and incubate at 26 °C overnight.
    2. Shift the flask from 26 °C to 32 °C.
    3. After 3 or 4 days, split culture 1:5 in amastigote media at 32 °C.
    4. Check the parasites in the next 3 - 4 days (maximum 7 days) to see if they are ready for use in infections.
      NOTE: Healthy axenic amastigotes should have an oval shape, without visible flagella. Partially differentiated amastigotes have a large oval shape with short flagella. The culture should not have a lot of clumps - many clumps are an indication of non-growing, dying parasites. The amastigote culture can be split 1:5 and maintained for a maximum of 3 weeks.

4. Infection with L. amazonensis

  1. Dilute parasite suspensions according to desired MOI (usually 3-5 metacyclic promastigotes per macrophage [MOI of 1:3 or 1:5] and 1 amastigote per macrophage [MOI 1:1]). Add Leishmania in PBS -/- in a volume of 50 - 100 µL to each well already containing 2 mL medium.
  2. Incubate BMMs for 1 h with amastigotes and 3 h with metacyclic promastigotes at 34 oC for infection.
    NOTE: Optimal infection temperature may vary by species.
  3. Following incubation, thoroughly wash away free parasites in each well 3x with 2 mL PBS -/- pre-warmed to 37 °C.
    NOTE: Disperse PBS gently to ensure that coverslips do not float over each other. Gently swirl the plate and then aspirate out the liquid. Use separate aspirating tip if using multiple strains of parasites to avoid cross-contamination.
  4. Fix 1 h or 3 h time-point samples by incubating each well with 1.5 - 2 mL of 2% PFA in PBS -/- for 10 min. Wash 3x with PBS -/-. Do not aspirate last wash and refrigerate plates containing coverslips in PBS until staining.
  5. Add 2 mL fresh BMM medium to each well on plates for further time-points and incubate at 34 °C.
  6. Fix remaining time-points as desired as described in step 4.3, and refrigerate plates until staining.

5. DAPI Staining and Coverslip Mounting

  1. Aspirate PBS from wells containing coverslips and add 1.5 mL PBS -/- with 0.1% non-ionic detergent. Incubate for 10 min at room temperature, followed by 3x wash with 2 mL PBS -/-.
  2. Add 1 mL PBS -/- with 2 µg/mL DAPI (diluted from 5 mg/mL stock solution in water) to wells containing coverslips and incubate for another 1 h at room temperature.
    NOTE: The incubation time with DAPI is critical for proper visualization of intracellular Leishmania parasites. Macrophage nuclei stain rapidly, due to their larger size and DNA content but staining of nuclei of the intracellular parasites is slower. Thus, extending incubation time beyond what is required to visualize the BMM nuclei is necessary to allow DAPI to permeate through and the parasite plasma membrane, and the parasite nuclear membrane. With proper DAPI stain, the mitochondrial kinetoplast DNA near the flagellar pocket of the parasite can also be visualized, in addition to the nuclear DNA.
  3. Wash each well containing coverslips 3x with 2 mL PBS -/- and then lift and flip coverslips with forceps to place the cell side down and mount on glass microscope slides with a commercially available antifade mounting reagent.
    NOTE: Coverslips are extremely fragile and need cautious handling. Avoid putting pressure on them, especially against the sidewall of the wells when lifting. Adding a few drops of PBS -/- reduces surface tension between the coverslip and well and facilitates the lifting process. A fine gauge needle may be used to assist in prying the coverslips from the bottom of the well. After placing a coverslip on the slide, gently press down with forceps to push out any air bubbles in the mounting media. If a coverslip is broken or has possibly flipped during the lifting process, do not remount; simply use the spare fourth coverslip.
  4. Refrigerate slides until quantification.

6. Infection Quantification

  1. Examine DAPI-stained slides under a fluorescence microscope by focusing on macrophages using 100X objective lens with immersion oil (excitation at 358 nm; optimal emission at 461 nm).
    Ensure that focus is on the layer of macrophages between the glass slide and coverslip.
  2. Quantify the number of macrophages (large nuclei stained with DAPI) and the number of smaller amastigote nuclei clustered around each macrophage nucleus (see Figure 2A, DAPI) for each field of vision, using a manual counter.
    NOTE: Amastigote nuclei may not all be visible in one plane of focus due to their small size. Count those that are visible when focused on macrophage nuclei, and then use fine focus to check for parasite nuclei in planes above and below the macrophage nuclei.
  3. Move to another field of vision to repeat quantification. Use a separate counter key to track the number of fields counted. Move through visual fields in parallel rows across each coverslip, to prevent counting overlap.
  4. Quantify a minimum of 200 macrophages per coverslip. Quantify each time-point of infection in triplicate (3 coverslips). Count the fourth coverslip if one of the previous is not suitable for counting due to coverslip overlap, poor mounting, glass breakage, etc.
    NOTE: If 200 macrophages cannot be counted on any one coverslip, count the spare fourth.
  5. Calculate infection rates as amastigotes/macrophage or amastigotes/100 macrophages and determine percent infected macrophages from the raw quantification data.

Results

Leishmania has two infective forms - metacyclic promastigotes that differentiate from procyclic promastigotes at the stationary phase of culture, and amastigotes, which are the intracellular stages (Figure 1). In some Leishmania species such as L. amazonensis, amastigotes can also be differentiated in axenic culture by shifting the promastigote cells to lower pH (4.5) and elevated temperature (32 °C), conditions similar to thos...

Discussion

The quantitative data produced by the BMM infection assay described above, allows investigators to obtain rates of infection and a reliable determination of changes in virulence properties in a relatively shorter time period (maximum 2 weeks, compared to the 2 months required for in vivo experiments). This method relies on the DNA specific dye DAPI, which specifically stains macrophage and parasite nuclei, and allows rapid identification and quantification of infected cells. In comparison, other stains such as G...

Disclosures

The authors declare they have no competing financial interests,

Acknowledgements

This work was supported by National Institutes of Health grant RO1 AI067979 to NWA.
YK is recipient of undergraduate fellowship from the Howard Hughes Medical Institute/University of Maryland College Park.

Materials

NameCompanyCatalog NumberComments
6 well cell culture plateCellstar657160
AdenineAcros OrganicsAC147440250
Aerosol Barrier Pipet Tips (100-1000 μL)Fisherbrand02-707-404
Aerosol Barrier Pipet Tips (20-200 μL)Fisherbrand02-707-430
Aerosol Barrier Pipet Tips (2-20 μL)Fisherbrand02-707-432
Bard-Parker Rib-Back Carbon Steel Surgical Blade #10Aspen Surgical371110
BD Luer-Lok Tip 10 mL SyringeBecton Dickinson (BD)309604
BD Precisionglide Needle, 25G Becton Dickinson (BD)305124
Cell Culture Dish 35 mm x 10 mmCellstar627 160
Cell Culture FlaskCellstar660175
Cover Glasses: 12 mm circlesFisherbrand12-545-80
DAPI (4',6-Diamidino-2-Phenylindole, Dihydrochloride)InvitrogenD1306
D-BiotinJ.T. BakerC272-00
EDTASigma AldrichEDS
Ethyl alcohol 200 proofPharmco-AAPER111000200
Falcon 100 mm x 15 mm non-TC-treated polystyrene Petri dishCorning351029
Fetal Bovine SerumSeradigm1500-500
Ficoll400Sigma AldrichF8016
Fluorescence MicroscopeNikonE200
Goat anti-mouse IgG Texas redInvitrogenT-862
Goat anti-rabbit IgG AlexaFluor488InvitrogenA-11034
HeminTokyo Chemical Industry Co. LTDH0008
HEPES (1M)Gibco15630-080
Isoton II DiluentBeckman Coulter8546719
L-GlutamineGemini400-106
Medium 199 (10X)Gibco11825-015
Na pyruvate (100 mM)Gibco11360-070
ParaformaldehydeAlfa Aesar43368
Penicillin/StreptomycinGemini400-109
Phosphate Buffered Saline (-/-)ThermoFisher14200166
Polypropyline conical Centrifuge Tubes 15 mLCellstar188 271
Polypropyline conical Centrifuge Tubes 50 mLCellstar227 261
ProLong Gold antifade reagentThermoFisherP36930
Rat anti-mouse Lamp-1 antibodyDevelopmental Studies Hybridoma Bank1D4B
Recombinant Human M-CSFPeproTech300-25
Reichert Bright-Line  Hemocytometer Hausser Scientific1492
RPMI Medium 1640 (1X)Gibco11875-093
Triton X-100 SurfactantMillipore SigmaTX1568-1
Trypan BlueSigma AldrichT8154
Delicate Scissors, 4 1/2"VWR82027-582
Dissecting Forceps, Fine TipVWR82027-386
Microscope SlidesVWR16004-368
Z1 Coulter Particle Counter, Dual ThresholdBeckman Coulter6605699

References

  1. WHO. Control of the leishmaniases. World Health Organ Tech Rep Ser. (949), (2010).
  2. Naderer, T., McConville, M. J. Intracellular growth and pathogenesis of Leishmania parasites. Essays Biochem. 51, 81-95 (2011).
  3. Rosenzweig, D., et al. Retooling Leishmania metabolism: from sand fly gut to human macrophage. FASEB J. 22 (2), 590-602 (2008).
  4. Lahav, T., et al. Multiple levels of gene regulation mediate differentiation of the intracellular pathogen Leishmania. The FASEB Journal. 25 (2), 515-525 (2011).
  5. Saunders, E. C., et al. Induction of a stringent metabolic response in intracellular stages of Leishmania mexicana leads to increased dependence on mitochondrial metabolism. PLoS Pathog. 10 (1), e1003888 (2014).
  6. Mittra, B., et al. Iron uptake controls the generation of Leishmania infective forms through regulation of ROS levels. J Exp Med. 210 (2), 401-416 (2013).
  7. Kloehn, J., et al. Using metabolomics to dissect host-parasite interactions. Curr Opin Microbiol. 32, 59-65 (2016).
  8. Huynh, C., Sacks, D. L., Andrews, N. W. A Leishmania amazonensis ZIP family iron transporter is essential for parasite replication within macrophage phagolysosomes. J Exp Med. 203 (10), 2363-2375 (2006).
  9. Flannery, A. R., Huynh, C., Mittra, B., Mortara, R. A., Andrews, N. W. LFR1 Ferric Iron Reductase of Leishmania amazonensis Is Essential for the Generation of Infective Parasite Forms. J Biol Chem. 286 (26), 23266-23279 (2011).
  10. Miguel, D. C., Flannery, A. R., Mittra, B., Andrews, N. W. Heme uptake mediated by LHR1 is essential for Leishmania amazonensis virulence. Infect Immun. 81 (10), 3620-3626 (2013).
  11. Cortez, M., et al. Leishmania Promotes Its Own Virulence by Inducing Expression of the Host Immune Inhibitory Ligand CD200. Cell Host Microbe. 9 (6), 463-471 (2011).
  12. Mittra, B., Andrews, N. W. IRONy OF FATE: role of iron-mediated ROS in Leishmania differentiation. Trends Parasitol. 29 (10), 489-496 (2013).
  13. Mittra, B., et al. A Trypanosomatid Iron Transporter that Regulates Mitochondrial Function Is Required for Leishmania amazonensis Virulence. PLoS Pathog. 12 (1), e1005340 (2016).
  14. Ben-Othman, R., et al. Leishmania-mediated inhibition of iron export promotes parasite replication in macrophages. PLoS Pathog. 10 (1), e1003901 (2014).
  15. Renberg, R. L., et al. The Heme Transport Capacity of LHR1 Determines the Extent of Virulence in Leishmania amazonensis. PLoS Negl Trop Dis. 9 (5), e0003804 (2015).
  16. McConville, M. J. Metabolic Crosstalk between Leishmania and the Macrophage Host. Trends Parasitol. 32 (9), 666-668 (2016).
  17. Carrera, L., et al. Leishmania promastigotes selectively inhibit interleukin 12 induction in bone marrow-derived macrophages from susceptible and resistant mice. J Exp Med. 183 (2), 515-526 (1996).
  18. Hsiao, C. H., et al. The effects of macrophage source on the mechanism of phagocytosis and intracellular survival of Leishmania. Microbes Infect. 13 (12-13), 1033-1044 (2011).
  19. Murray, A. S., Lynn, M. A., McMaster, W. R. The Leishmania mexicana A600 genes are functionally required for amastigote replication. Mol Biochem Parasitol. 172 (2), 80-89 (2010).
  20. Farias Luz, N., et al. RIPK1 and PGAM5 Control Leishmania Replication through Distinct Mechanisms. J Immunol. 196 (12), 5056-5063 (2016).
  21. Franco, L. H., et al. Autophagy downstream of endosomal Toll-like receptor signaling in macrophages is a key mechanism for resistance to Leishmania major infection. J Biol Chem. 292 (32), 13087-13096 (2017).
  22. da Silva, M. F., Zampieri, R. A., Muxel, S. M., Beverley, S. M., Floeter-Winter, L. M. Leishmania amazonensis arginase compartmentalization in the glycosome is important for parasite infectivity. PLoS One. 7 (3), e34022 (2012).
  23. Carneiro, P. P., et al. The Role of Nitric Oxide and Reactive Oxygen Species in the Killing of Leishmania braziliensis by Monocytes from Patients with Cutaneous Leishmaniasis. PLoS One. 11 (2), e0148084 (2016).
  24. Siqueira-Neto, J. L., et al. An image-based high-content screening assay for compounds targeting intracellular Leishmania donovani amastigotes in human macrophages. PLoS Negl Trop Dis. 6 (6), e1671 (2012).
  25. Pastor, J., et al. Combinations of ascaridole, carvacrol, and caryophyllene oxide against Leishmania. Acta Trop. 145, 31-38 (2015).
  26. Giarola, N. L., et al. Leishmania amazonensis: Increase in ecto-ATPase activity and parasite burden of vinblastine-resistant protozoa. Exp Parasitol. 146, 25-33 (2014).
  27. Sacks, D. L., Melby, P. C. Animal models for the analysis of immune responses to leishmaniasis. Curr Protoc Immunol. , 12 (2001).
  28. Tabbara, K. S., et al. Conditions influencing the efficacy of vaccination with live organisms against Leishmania major infection. Infect Immun. 73 (8), 4714-4722 (2005).
  29. Price, J. V., Vance, R. E. The macrophage paradox. Immunity. 41 (5), 685-693 (2014).
  30. Huynh, C., Andrews, N. W. Iron acquisition within host cells and the pathogenicity of Leishmania. Cell Microbiol. 10 (2), 293-300 (2008).
  31. Blackwell, J. M., et al. SLC11A1 (formerly NRAMP1) and disease resistance. Cell Microbiol. 3 (12), 773-784 (2001).
  32. Pinto-da-Silva, L. H., et al. The 3A1-La monoclonal antibody reveals key features of Leishmania (L) amazonensis metacyclic promastigotes and inhibits procyclics attachment to the sand fly midgut. Int J Parasitol. 35 (7), 757-764 (2005).
  33. Spath, G. F., Beverley, S. M. A lipophosphoglycan-independent method for isolation of infective Leishmania metacyclic promastigotes by density gradient centrifugation. Exp Parasitol. 99 (2), 97-103 (2001).
  34. Zilberstein, D., Shapira, M. The role of pH and temperature in the development of Leishmania parasites. Annu Rev Microbiol. 48, 449-470 (1994).
  35. Bates, P. A. Transmission of Leishmania metacyclic promastigotes by phlebotomine sand flies. Int J Parasitol. 37 (10), 1097-1106 (2007).
  36. Bates, P. A., Robertson, C. D., Tetley, L., Coombs, G. H. Axenic cultivation and characterization of Leishmania mexicana amastigote-like forms. Parasitology. 105 (Pt 2), 193-202 (1992).
  37. Frickmann, H., et al. Rapid identification of Leishmania spp. in formalin-fixed, paraffin-embedded tissue samples by fluorescence in situ hybridization. Trop Med Int Health. 17 (9), 1117-1126 (2012).
  38. Seguin, O., Descoteaux, A. Leishmania, the phagosome, and host responses: The journey of a parasite. Cell Immunol. 309, 1-6 (2016).
  39. Wanderley, J. L., Thorpe, P. E., Barcinski, M. A., Soong, L. Phosphatidylserine exposure on the surface of Leishmania amazonensis amastigotes modulates in vivo infection and dendritic cell function. Parasite Immunol. 35 (3-4), 109-119 (2013).
  40. Crauwels, P., et al. Apoptotic-like Leishmania exploit the host's autophagy machinery to reduce T-cell-mediated parasite elimination. Autophagy. 11 (2), 285-297 (2015).
  41. Bringmann, G., et al. A novel Leishmania major amastigote assay in 96-well format for rapid drug screening and its use for discovery and evaluation of a new class of leishmanicidal quinolinium salts. Antimicrob Agents Chemother. 57 (7), 3003-3011 (2013).
  42. Sacks, D. L., Brodin, T. N., Turco, S. J. Developmental modification of the lipophosphoglycan from Leishmania major promastigotes during metacyclogenesis. Mol Biochem Parasitol. 42 (2), 225-233 (1990).
  43. Sacks, D. L. Leishmania-sand fly interactions controlling species-specific vector competence. Cell Microbiol. 3 (4), 189-196 (2001).
  44. McConville, M. J., Turco, S. J., Ferguson, M. A., Sacks, D. L. Developmental modification of lipophosphoglycan during the differentiation of Leishmania major promastigotes to an infectious stage. EMBO J. 11 (10), 3593-3600 (1992).
  45. Sacks, D. L., Hieny, S., Sher, A. Identification of cell surface carbohydrate and antigenic changes between noninfective and infective developmental stages of Leishmania major promastigotes. J Immunol. 135 (1), 564-569 (1985).
  46. Yao, C., Chen, Y., Sudan, B., Donelson, J. E., Wilson, M. E. Leishmania chagasi: homogenous metacyclic promastigotes isolated by buoyant density are highly virulent in a mouse model. Exp Parasitol. 118 (1), 129-133 (2008).
  47. Almeida Marques-da-Silva, E., et al. Extracellular nucleotide metabolism in Leishmania: influence of adenosine in the establishment of infection. Microbes Infect. 10 (8), 850-857 (2008).
  48. Moreira, D., et al. Impact of continuous axenic cultivation in Leishmania infantum virulence. PLoS Negl Trop Dis. 6 (1), e1469 (2012).
  49. Svensjo, E., et al. Interplay between parasite cysteine proteases and the host kinin system modulates microvascular leakage and macrophage infection by promastigotes of the Leishmania donovani complex. Microbes Infect. 8 (1), 206-220 (2006).

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