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Leishmania mexicana mexicana: quantitative analysis of the intracellular cycle

Published online by Cambridge University Press:  06 April 2009

P. S. Doyle
Affiliation:
Laboratory of Parasitic Diseases, National Institute of Allergy and Infectious Diseases, National Institutes of Health, Bethesda, Maryland 20892, USA
J. C. Engel
Affiliation:
Laboratory of Parasitic Diseases, National Institute of Allergy and Infectious Diseases, National Institutes of Health, Bethesda, Maryland 20892, USA
A. A. Gam
Affiliation:
Laboratory of Parasitic Diseases, National Institute of Allergy and Infectious Diseases, National Institutes of Health, Bethesda, Maryland 20892, USA
J. A. Dvorak
Affiliation:
Laboratory of Parasitic Diseases, National Institute of Allergy and Infectious Diseases, National Institutes of Health, Bethesda, Maryland 20892, USA

Summary

The complete intracellular cycle of the Leishmania mexicana mexicana G. S. strain was quantified in human macrophages and in the mouse IC-21 macrophage line utilizing a culture system that allows the direct observation of individual intracellular parasites. A wide range of pre-replicative lag periods exists, implying that promastigotes may be in any phase of their DNA synthetic cycle when phagocytosed by the macrophage. Amastigotes replicated 2–3 times, after which the host cell died and liberated amastigotes that were taken up by other macrophages and continued to replicate. The mean amastigote population-doubling time in human macrophages (17.5 h) was not statistically different from promastigotes growing in axenic culture (16.4 h), but was nearly 2-fold less than amastigotes growing in mouse-derived IC-21 macrophages (33.7 h). These observations are markedly different from cover-glass culture assays of Leishmania-macrophage interactions and provide an unambiguous description of the intracellular cycle of Leishmania mexicana mexicana.

Type
Research Article
Copyright
Copyright © Cambridge University Press 1989

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References

Axline, S. G. (1970). Functional biochemistry of the macrophage. Seminars in Haematology 7, 142–60.Google ScholarPubMed
Axline, S. G. & Cohn, Z. A. (1970). In vitro induction of lysosomal enzymes by phagocytosis. Journal of Experimental Medicine 131, 1239–60.CrossRefGoogle ScholarPubMed
Berman, J. D., Dwyer, D. M. & Wyler, D. J. (1979). Multiplication of Leishmania in human macrophages in vitro. Infection and Immunity 26, 375–9.CrossRefGoogle ScholarPubMed
Berman, J. D., Fioretti, T. B. & Dwyer, D. M. (1981). In vivo and in vitro localization of Leishmania within macrophage phagolysosomes: use of colloidal gold as a lysosomal label. Journal of Protozoology 28, 239–42.CrossRefGoogle ScholarPubMed
Berman, J. & Neva, F. A. (1981). Effects of temperature on multiplication of Leishmania amastigotes within human monocyte-derived macrophages in vitro. American Journal of Tropical Medicine and Hygiene 30, 318–21.CrossRefGoogle ScholarPubMed
Biegel, D., Topper, G. & Rabinovitch, M. (1983). Leishmania mexicana: temperature sensitivity of isolated amastigotes infecting macrophages in culture. Experimental Parasitology 56, 289–97.CrossRefGoogle ScholarPubMed
Black, C. M., Beaman, B. L., Donovan, R. M. & Goldstein, E. (1983). Effect of virulent and less virulent strains of Nocardia asteroides on acid-phosphatase activity in alveolar and peritoneal macrophages maintained in vitro. Journal of Infectious Diseases 148, 117–24.CrossRefGoogle ScholarPubMed
Boné, G. J. & Steinert, M. (1956). Isotopes incorporated in the nucleic acids of Trypanosoma mega. Nature, London 178, 308–9.CrossRefGoogle ScholarPubMed
Bryceson, A. D. M. (1969). Diffuse cutaneous leishmaniasis in Ethiopia. I. The clinical and histological features of the disease. Transactions of the Royal Society of Tropical Medicine and Hygiene 63, 708–37.CrossRefGoogle ScholarPubMed
Cohn, Z. A. (1968). The structure and function of monocytes and macrophages. Advances in Immunology 9, 163214.CrossRefGoogle ScholarPubMed
Cooper, S. (1982). The continuum model: application to G1 arrest and Go. In Cell Growth (ed. Nicolini, C.) New York and London: Plenum Press. pp. 305–14.Google Scholar
Croft, S. L., Neal, R. A., Pendergast, W. & Chan, J. H. (1987). The activity of alkyl phosphorylcholines and related derivatives against Leishmania donovani. Biochemical Pharmacology 36, 2633–6.CrossRefGoogle ScholarPubMed
Dvorak, J. A. & Howe, C. L. (1979). Toxoplasma gondii vertebrate cell interactions. II. The intracellular reproductive phase. Journal of Protozoology 26, 114–17.CrossRefGoogle ScholarPubMed
Dvorak, J. A. & Stotler, W. F. (1971). A controlledenvironment culture system for high resolution light microscopy. Experimental Cell Research 68, 144–8.CrossRefGoogle ScholarPubMed
Finley, R. W. & Dvorak, J. A. (1987). Trypanosoma cruzi: analysis of the population dynamics of heterogeneous mixtures. Journal of Protozoology 34, 409–15.CrossRefGoogle ScholarPubMed
Hadjuck, S. L., Kitchin, P. A., Marini, J. C. & Englund, P. T. (1983). Structure and replication of kinetoplast DNA. In Molecular Biology of Host-Parasite Interactions, Proceedings of a UCLA Symposium on Molecular and Cellular Biology (ed. Agabian, N. & Eisen, H.), New York: A. R. Liss, Inc. pp. 197204.Google Scholar
Heinzel, F. P., Sadick, M. D. & Locksley, R. M. (1988). Leishmania major: analysis of lymphocyte and macrophage cellular phenotypes during infection of susceptible and resistant mice. Experiment Parasitology 65, 258–68.CrossRefGoogle ScholarPubMed
Mauel, J. & Defendi, V. (1971). Activation and transformation of mouse peritoneal macrophages by simian virus 40. Journal of Experimental Medicine 134, 335–50.CrossRefGoogle ScholarPubMed
Nakagawara, A., Nathan, C. F. & Cohn, Z. A. (1981). Hydrogen peroxide metabolism in human monocytes during differentiation in vitro. Journal of Clinical Investigation 68, 1243–52.CrossRefGoogle ScholarPubMed
Petersen, E. A., Neva, F. A., Oster, C. N. & Bogaert-Diaz, H. (1982). Specific inhibition of lymphocyteproliferation responses by adherent suppressor cells in diffuse cutaneous leishmaniasis. New England Journal of Medicine 306, 387–90.CrossRefGoogle ScholarPubMed
Sacks, D. L., Barral, A. & Neva, F. A. (1983). Thermosensitivity patterns of Old vs. New World cutaneous strains of Leishmania growing within mouse peritoneal macrophages in vitro. American Journal of Tropical Medicine and Hygiene 32, 300–4.CrossRefGoogle ScholarPubMed
Scott, p. A., James, S. & Sher, A. (1985). The respiratory burst is not required for killing of intracellular and extracellular parasites by a lymphokine-activated macrophage cell line. European Journal of Immunology 15, 553–8.CrossRefGoogle Scholar
Scott, P. A., Sacks, D. & Sher, A. (1983). Resistance to macrophage-mediated killing as a factor influencing the pathogenesis of chronic cutaneous leishmaniasis. Journal of Immunology 131, 966–71.CrossRefGoogle ScholarPubMed
Scott, P. A. & Sher, A. (1986). A spectrum of susceptibility of Leishmanial strains to intracellular killing by murine macrophages. Journal of Immunology 136, 1461–6.CrossRefGoogle ScholarPubMed
Shnur, L. F., Walton, B. C. & Bogaert-Diaz, H. (1983). On the identity of the parasite causing diffuse cutaneous leishmaniasis in the Dominican Republic. Transactions of the Royal Society of Tropical Medicine and Hygiene 77, 756–62.CrossRefGoogle Scholar
Simpson, L. (1972). The kinetoplasts of hemoflagellates. International Review of Cytology 32, 139207.CrossRefGoogle Scholar
Vickerman, K. & Preston, T. M. (1976). Comparative cell biology of the kinetoplastid flagellates. In Biology of the Kinetoplastida, Vol.1 (ed. Lumsden, W. H. & Evans, D. A.), London: Academic Press. pp. 3588.Google Scholar