The role of free-living pathogenic amoeba in the transmission of leprosy: a proof of principle.
The routes, methods and mechanisms of transmission of leprosy are poorly understood. However, some of the pieces of the leprosy transmission puzzle have been partially defined and support reasonable hypotheses. For example, it seems likely that the enormous numbers of leprosy bacilli expelled into the environment in the nasal discharges of lepromatous patients (1) is one source of infection and Desikan has demonstrated detectable viability of M. leprae in nasal discharges. (2) There is also evidence to support excretion of bacilli from skin lesions. (3) Other experimental evidence supports the entry of bacilli into a new host via one of two (or both) portals; invasion and subsequent infection though the nasal mucosa (4) or abraded or punctured skin. (5)
Regardless of the hypothetical route of transmission, there remains an enigma. How does M. leprae, an obligate intracellular pathogen that is so fastidious, it cannot be cultured after 130 + years of effort, remain viable and infectious in a rather inhospitable environmental niche between hosts? In the present hypothesis we explored whether M. leprae could be taken up by free-living pathogenic amoebae in the soil or water and survive, sheltered intracellularly in these protozoa serving, essentially as 'feral macrophages'.
There is ample precedence for this hypothesis. A number of studies report that microorganisms can survive endosymbiotically in free-living pathogenic amoebae. (6) In 1980 an association between Acanthamoeba and Legionella pneumophila (7) was reported by Rowbotham who suggested that infected amoebae were the source of Legionaires Disease. Subsequently L. pneumophila was shown to resist phagosome-lysosome fusion and multiplies in A. castellanii. (8) A number of other organisms have been shown to be endosymbionts in Acanthamoeba spp. including Pseudomonas, (9) Chlamydia, (10) Burkholderia (11) and Listeria monocytogenes. (12) Several reports describe infection of Acanthamoebae with environmental (13) or pathogenic mycobacteria such as M. avium-intracellularae, (14,15) Mycobacterium paratuberculosis, (16) M. bovis and BCG. (17)
Infection of amoebae with M. leprae was suggested by Jadin in 1975 who demonstrated the uptake of M. leprae by Acanthamoeba castellanii (18) and by Grange et al. (19) in 1987. Our findings extend these reports by exploiting our routine access to highly viable and purified nu/nu-derived M. leprae (20,21) coupled with in vitro and in vivo assays for M. leprae viability. We pose the question of whether the leprosy bacillus survives intracellularly in A. castellani.
Materials and Methods
A. CASTELLANII CULTURE
Frozen Acanthamoeba castellanii (Neff) culture was obtained from ATCC (Cat # 30010) and maintained in T75 flasks (Corning) by twice weekly passage at room temperature (26[degrees]C) in ATCC 712 medium (www.atcc.org product information sheet 30010). A. castellanii was also maintained in culture on a non-nutrient agar surface coated with killed Escherichia coli as described by Neff. (22) Briefly, 1.0 ml (1 x [10.sup.9]) irradiated E. coli ([10.sup.6] Rad [Sheppard Model 484 [sup.60]Co irradiator]) was spread evenly on 80 mm Petri plates of non-nutrient agar (Difco). An A. castellanii suspension (5 x [10.sup.6] amoebae in 0.1 ml) was then spotted at the centre of the plate and the cultures incubated at 33[degrees]C. Over a 24-48 hour period the amoebae ingested the E. coli, spread radially and multiplied.
NUDE MOUSE DERIVED M. LEPRAE
The Thai-53 isolate of Mycobacterium leprae was maintained in the foot pads of athymic nu/nu mice infected for 4-6 months, and then harvested as described previously, (20) washed by centrifugation, resuspended in RPMI-1640 (Gibco) + 10% (v/v) fetal calf serum [(FCS) Gibco] and enumerated by direct count according to Shepard's method. (23) M. leprae suspensions were purified by NaOH treatment as described previously. Briefly, 1 x [10.sup.9] fresh M. leprae were suspended in 1.0 ml of 0.1N NaOH (Sigma) and incubated for 3 minutes at room temperature, after which the bacteria were washed three times in Hanks balanced salt solution and finally resuspended in the appropriate media. Freshly harvested viable bacilli were always employed in experiments within 2 hours of harvest.
STAINING OF M. LEPRAE WITH THE VITAL RED STAIN PKH26
For confocal microscopy studies, freshly harvested and 0.1N NaOH treated M. leprae were stained with fluorescent red PKH26 dye (Sigma) following a published protocol. (24) Briefly, M. leprae were stained for 2 minutes at room temperature with a 1:250 dilution of PKH26 dye. The suspension was washed three times in appropriate medium. The numbers of bacteria were recounted following staining by Shepard's direct count method. (23)
INFECTION OF A. CASTELLANII WITH LIVE M. LEPRAE
Monolayers of A. castellanii cultures in T75 flasks (Corning) containing 15 ml of ATCC 712 media were infected with viable M. leprae at an MOI of 20:1 and incubated overnight at 26[degrees]C. Extracellular M. leprae were removed by decanting the media and washing 3 times with phosphate buffered saline (PBS). For some experiments infected amoebae were removed by vigorous shaking after chilling the cultures at 4[degrees]C. For other experiments intracellular M. leprae were released from amoebae by lysis with 0.1N NaOH (Sigma) at 24, 48, 72 and 96 hour post infection, and the M. leprae processed for radiorespirometry, viability staining and inoculation into nu/nu mouse foot pads.
STAINING OF INFECTED A. CASTELLANII TROPHOZOITES
Briefly, A. castellanii cultures were stained with carbol fucshin for 20 minutes at room temperature. After washing with acid alcohol the slides were counter stained with methyl green.
A Leica SP2 confocal microscope was used to ascertain internalisation of live M. leprae by A. castellanii trophozoites. Serial optical sections of the infected amoeba were taken at 0.2 nm using 514 nm excitation laser and 560 [+ or -] 20 nm emission filters.
Metabolism of suspensions of control and amoeba-derived M. leprae was measured by evaluating the oxidation of [sup.14]C-palmitic acid to [sup.14]C[O.sub.2] by RR as described previously.  Briefly, 1 x [10.sup.7] M. leprae were suspended in 4.0 ml of acidified Middlebrook 7H12 BACTEC PZA media (Becton Dickinson) in a 5 ml glass vial with loosened cap which, in turn was inserted into a wide mouth liquid scintillation vial lined with filter paper impregnated with NaOH, 2,5-diphenyloxazole (Sigma) and Concentrate I (Kodak). When read daily, captured [sup.14]C[O.sub.2], determines the rate of [sup.14]C-palmitic acid oxidation. In the present study the 7th day cumulative counts per minute (CPM) are reported. This measure of metabolic activity by suspensions of M. leprae correlates highly with viability as demonstrated by growth in the mouse foot pad. (20)
FLUORESCENT VIABILITY STAINING (VS) OF M. LEPRAE
The membrane integrity of amoeba-derived M. leprae was evaluated with a LIVE/DEAD BacLight Bacterial Viability Kit[R] (Molecular Probes) as described previously. (21) Briefly, M. leprae were washed in normal saline and incubated for 15 minutes at room temperature with Syto9 and propidium iodide (PI). The bacteria were washed again and resuspended in 10% (v/v) glycerol in normal saline. The dead and live bacteria were enumerated by direct counting of fluorescent green and red bacilli using appropriate single bandpass filters. The excitation/emission maxima are 480 nm/500 nm for Syto9 and 490 nm/635 nm for PI. This VS method measures the cell wall integrity of individual bacilli and correlates highly, both with RR and growth in the mouse foot pad. (21)
NUDE MOUSE FOOT PAD GROWTH OF M. LEPRAE
Athymic nu/nu mice, four in each group, were inoculated on the plantar surface of both hind feet with 5 x [10.sup.6] M. leprae harvested 72 hour post infection from A. castellanii or control M. leprae incubated in parallel at 26[degrees]C. At 4- and 7-months both hind foot pads were harvested from each of two mice, processed and the number of AFB enumerated using Shepard's technique. (23)
The data are shown as means [+ or -] standard deviation (SD) from a representative of three to four experiments. The raw data were subjected to Student's t test to determine whether the observed differences between the means were significant. P < 0.05 was taken as significant.
UPTAKE OF M. LEPRAE BY A. CASTELLANII
As shown by acid fast staining of infected amoebae in Figure 1A and confocal microscopy of fluorescent stained M. leprae in Figure 1B, the amoebae were able to efficiently ingest live M. leprae after overnight incubation at a MOI of 20:1. Greater than 90% of amoebae were infected (Figure 1A). Ingestion of live M. leprae did not show any apparent adverse effect on the amoeba as they divided normally over several days (data not shown) and did not form cysts.
CULTURE OF A. CASTELLANII ON A SURFACE CONSISTING OF E. COLI OR M. LEPRAE
Figure 2B shows progress of spreading A. castellanii culture at 33[degrees]C on non-nutrient agar coated with irradiated E. coli, while amoeba did not advance on either non-nutrient agar alone (2A) or on non-nutrient agar coated with irradiated M. leprae (2C).
Similar findings were seen at an incubation temperature of 37[degrees]C while the radial advance of amoebae on the E. coli plates was markedly reduced at 26[degrees]C (data not shown). These results indicate that A. castellanii was not able to thrive solely on irradiated M. leprae as it could efficiently on irradiated E. coli.
[FIGURE 1 OMITTED]
IN VITRO TESTS FOR VIABILITY OF M. LEPRAE ISOLATED FROM INFECTED A. CASTELLANII
Both RR and VS results show negligible loss of viability in M. leprae ingested by amoebae even after 96 hour (RR P = 0.802, VS P = 0.783) (Figure 3A and 3B).
It was difficult to perform the assays beyond 96 hours due to the multiplication of the amoebae and the consequent dilution of the infected population. In a representative experiment where 90% of the amoebae were infected at 0 hours, 49% were infected at 24 hours, 15% at 72 hours and < 5% at 96 hours.
[FIGURE 2 OMITTED]
[FIGURE 3 OMITTED]
GROWTH IN THE NUDE MOUSE FOOT PAD OF M. LEPRAE ISOLATED FROM A. CASTELLANII
M. leprae harvested from A. castellanii 72 hours after ingestion were used to inoculate both hind foot pads of athymic nu/nu mice. In both groups foot pads were visibly enlarged at 4 months. At 4 and 7 months post inoculation the growth in the nude mouse foot pad of M. leprae harvested from A. castellanii 72 hour post-infection was indistinguishable from (P = 0.894) that of the control (Figure 4).
Our laboratory has devoted considerable effort to defining the biophysical optima of M. leprae, (20) quantifying 'viability' in vitro in this uncultivable organism (25,21) and developing routine access (weekly) to large numbers of fresh viable M. leprae from the foot pads of athymic (nu/nu) mice. (21,24) These techniques and this valuable research resource were critical to carrying out the present study.
[FIGURE 4 OMITTED]
We chose for the present studies Acanthamoebae castellanii as a putative amoebic 'host cell' for M. leprae because these protozoa have been shown to harbour and support the growth of a number of other bacteria, including environmental mycobacteria; (13) and there is ample precedence for Acanthamoeba being a host cell for several pathogenic mycobacteria; M. avium-intraclllularae, (14) M. paratuberculosis, (16) BCG (17) and M. bovis. (17) Acanthamoeba may play a role in transmission of mycobacterial infection to man. (14)
The present studies demonstrated the avid uptake of M. leprae by A. castellanii in a dose dependant manner. Even with a high MOI where virtually all of the amoebae phagocytosed M. leprae, there appeared to be no ill effect on the multiplication of the infected protozoa (data not shown). Time course observations (data not shown) revealed that with time (24-48 hours) individual intracellular bacilli, distributed throughout the cytoplasm at 0 hours, appeared to be packaged by the host amoeba into a single large vacuole.
Whereas the amoebae could survive and multiply on a simple diet of killed E.coli, (22) M. leprae alone did not appear to provide the necessary nutrients and were not digested or degraded. In fact, M. leprae survived for at least 4 days as shown by their metabolic activity (RR) and cell wall integrity (VS), in vitro assays for viability. (21) More importantly, viability after 3 days of infection of amoebae was undiminished when evaluated by inoculation into the foot pads of athymic (nu/nu) mice. We consider these findings as proof of principle supporting the hypothesis that A. castellanii and perhaps other soil or aquatic free-living pathogenic amoebae might perform as 'feral macrophages' by facilitating the survival of the leprosy bacillus in the environment when expelled from their human host.
An interesting corollary to this hypothesis would be the potential role of dormant encysted amoeba in protecting M. leprae during adverse environmental conditions such as desiccation, changes in temperature and pH. (26) In preliminary experiments with M. leprae-infected A. castellanii, where encystment was induced by raising NaCl concentration we observed, under phase microscopy, that as the trophozoites condensed in size and formed thickened cell walls they appeared to expel their particulate contents, including M. leprae (unpublished observation). However, a report by Steinert et al. employed electron microscopy to demonstrate the presence of M. avium within the outer walls of the double walled Acanthamoeba cyst when infected trophozoites were encouraged to encyst. (15) Additional studies are being carried out with M. leprae.
Finally, the demonstration that M. leprae will survive in a pathogenic free-living amoeba will allow us to move this hypothesis forward and determine if M. leprae infected free-living pathogenic amoebae could play a role in the actual transmission of leprosy by facilitating the invasion of human tissue. First we will need to confirm these in vitro findings in other members of the genus Acanthamoeba, A. culbertsoni, and A. polyphaga, both of which have already been shown to support the growth of pathogenic mycobacteria. (27) Various species of Acanthamoeba, A. castellani, A. culbertsoni and A. polyphaga are the agents of human diseases (27) including Granulomatous Amoebic Encephalitis (GAE) a slowly progressive CNS infection, cutaneous acanthamoebiasis (CA), and amoebic keratitis (AK). GAE and CA are diseases seen in immunosuppressed patients while (AK) is a sight-threatening corneal disease that can occur in immunocompetent individuals and is acquired from contact lens cases or cleaning solutions. The route of infection for GAE and CA are not clearly understood but the nasal passages and/or cutaneous lesions are considered likely routes. (27)
In preparation for the next (in vivo) stage in these studies we will also be concerned with Naeglaria fowleri, a notorious human pathogen. (28) N. fowleri is the causative agent of primary amoebic meningoencephalitis, (PAM) a rare but rapidly fatal human disease. (28) N. fowleri is found in warm fresh water ponds and lakes worldwide, inadequately chlorinated swimming pools, and moist soil. (28) The portal of entry for humans appears to be the nasal mucosa with subsequent invasion of the olfactory nerve plexus and rapid travel ( (24) hours) of the amoebae up the olfactory nerves, through the cribiform plate and into olfactory bulb and spread to other areas of the CNS. (29)
The crux of this second hypothesis is that the vast majority of infections with free-living pathogenic amoebae are of no consequence; that human disease is an extremely rare outcome. Hundreds of millions have likely been exposed to N. fowleri by diving, swimming or splashing in infected fresh water, yet there are less than (200) recorded cases of the rapidly fatal fulminate PAM, suggesting a high level of resistance or that infection is usually asymptomatic. (30) Mice immunised with killed N. fowleri are highly resistant to a lethal intravenous challenge with amoebae (31) and serologic studies in endemic areas show a high prevalence of protective antibodies in humans suggesting exposure without disease. (32) One estimate of the probability of contracting PAM, once exposed to Naegleria is 1 in 100 million exposures. (30)
The earliest response of the host to amoebae consists of an influx of polymorphonuclear neutrophils to the site of infection, followed by an influx of macrophages (33) which have been shown in vitro to have a deleterious effect on target amoebae. (34) This is the exact sequence of events, culminating in uptake of M. leprae by its preferred host cell, the macrophage that would complete the hypothesis for a role of free-living amoebae in facilitating leprosy transmission. We intend to exploit already described mouse models for N. fowleri (29,31,35-36) and Acanthomoeba sp. (34) infection to determine if M. leprae infected amoebae transport the bacilli through the nasal mucosa or through intact or abraded skin.
We gratefully acknowledge the excellent technical support of Baljit Randhawa and Greg McCormick. These studies were support by a grant from The German Leprosy Relief Association, Wurzburg, Germany.
(1) Davey TF, Rees RJW. The nasal discharge in leprosy: clinical and bacteriological aspects. Lep Rev, 1974; 45: 121-134.
(2) Desikan KV. Viability of Mycobacterium leprae outside the human body. Lepr Rev, 1977; 48: 231-235.
(3) Job CK, Jayakumar J, Kearney M, Gillis TP. Transmission of leprosy: A study of skin and nasal secretions of household contacts of leprosy patients using PCR. Am J Trop Med Hyg, 2008; in press.
(4) Chehl S, Job CK, Hastings RC. The nose: a site for the transmission of leprosy in nude mice. Am J Trop Med Hyg, 1985; 34: 1161-1166.
(5) Job CK, Harris EB, Allen JL, Hastings RC. Thorns in armadillo ears and noses and their role in the transmission of leprosy. Arch Pathol Lab Med, 1986; 110: 1025-1028.
(6) Barker J, Brown MRW. Trojan horses of the microbial world: protozoa and the survival of bacterial pathogens in the environment. Microbiology, 1994; 140: 1253-1259.
(7) Rowbotham TJ. Preliminary report on the pathogenicity of Legionella pneumophila for freshwater and soil amoeba. J Clin Pathol, 1980; 33: 1179-1183.
(8) Bozue JA, Johnson W. Interaction of Legionella pneumophila with Acanthamoeba castellanii: uptake by coiling phagocytosis and inhibition of phagosome-lysosome fusion. Infect Immun, 1996; 64: 668-673.
(9) Michel R, Burgha RDT, Bergmann H. Acanthamoeba, naturally intracellularly infected with Pseudomoinas aeruginosa after their isolation form a microbiologically contaminated drinking water system in a hospital. Zentbl Hyg Umweltmed, 1995; 196: 532-544.
(10) Essig A, Heinemann M, Simnacher U, Marre R. Infection of Acanthamoeba castellanii with Chlamydia pneumonia. Appl Envir Microbiol, 1997; 63: 1396-1399.
(11) Landers P, Kerr KG, Rowbotham TJ et al. Survival and growth of Burkholderia cepacia within the free-living amoeba Acanthamoeba polyphaga. Eur J Clin Microbiol, 2000; 19: 121-123.
(12) Ly TMC, Muller HE. Ingested Listeria monocytogenes survive and multiply in protozoa. J Med Microbiol, 1990; 33: 51-54.
(13) Adekambi T, Salah SB, Khlif M et al. Survival of environmental mycobacteria in Acanthamoeba polyphaga. Appl Envir Microbiol, 2006; 72: 5974-5981.
(14) Cirillo J, Falkow S, Tompkins L, Bermudez L. Interaction of Mycobacterium avium with environmental amoebae enhances virulence. Infect Immun, 1997; 65: 3759-3767.
(15) Steinert M, Birkness K, White E et al. Mycobacterium avium bacilli grow saprozoically in coculture with Acanthamoeba polyphaga and survive within cyst walls. Appl Envir Microbiol, 1998; 64: 2256-2261.
(16) Mura M, Bull T, Evans H et al. Replication and long term persistence of bovine and human strains of Mycobacterium avium subsp. paratuberculosis within Acanthamoeba polyphaga. Appl Envir Microbiol, 2006; 72: 854-859.
(17) Taylor SJ, Ahonen LJ, de Leij AM, Dale JW. Infection of Acanthamoeba castellanii with Mycobacterium bovis and M. bovis BCG and survival of M. bovis within the amoebae. Appl Envir Microbiol, 2003; 69: 4316-4319.
(18) Jadin JB. Amibes limax vecteurs possible de Mycobacteries et de M. leprae. Acta Leprol, 1975; 59: 57-67.
(19) Grange JM, Dewar CA, Powbotham TJ. Microbe dependence of Mycobacterium leprae: a possible intracellular relationship with protozoa. Int J Lepr, 1987; 55: 565-566.
(20) Truman RW, Krahenbuhl JL. Viable M. leprae as a research reagent. Int J Lepr, 2001; 69: 1-12.
(21) Lahiri R, Randhawa B, Krahenbuhl J. Application of a viability-staining method for Mycobacterium leprae derived from the athymic (nu/nu) mouse footpad. J Med Microbiol, 2005; 54: 235-242.
(22) Neff RJ. Mechanisms of purifying amoebae by migration on agar surfaces. J Protozool, 1958; 5: 226-231.
(23) Shepard CC, McRae RC. A method for counting acid fast bacteria. Int J Lepr, 1968; 36: 78-82.
(24) Lahiri R, Randhawa B, Krahenbuhl JL. Effects of Purification and Fluorescent Staining on Viability of Mycobacterium leprae. Int J Lepr, 2005; 73: 194-202.
(25) Franzblau SG. Oxidation of palmitic acid by Mycobacterium leprae in an axenic medium. J Clin Microbiol, 1988; 26: 18-21.
(26) Chagla AH, Griffiths AJ. Growth and encystations of Acanthamoeba castellanii. J Gen Microbiol, 1974; 85: 139-145.
(27) Marcianno-Cabral F, Puffenbarger R, Cabral GA. The increasing importance of Acanthamoeba infections. J Eukaryot Microbiol, 2000; 47: 29-36.
(28) John DT. Primary amebic meningoencephalitis and the biology of Naegleria fowleri. Ann Rev Microbiol, 1982; 36: 101-123.
(29) Jarolim KL, McCosh JK, Howard MJ, John DT. A light microscopic study of the migration of Naegleria fowleri from the nasal submucosa to the central nervous system during the early stages of primary amebic encephalitis in mice. J Parasitol, 2006; 86: 50-55.
(30) Matthews S, Ginzl D, Walsh D et al. Primary amebic meningoencephalitis--Arizona, Florida and Texas, 2007. MMWR, 2008; 57: 573-577.
(31) Grate I. Primary amebic meningoencephalitis: a silent killer. Can J Emerg Med, 2006; 8: 365-369.
(32) Chappell CL, Wright JA. Standardized method of measuring Acanthamoeba in sera from healthy human subjects. Clin Diag Lab Immunol, 2001; 8: 724-730.
(33) Ferrante A, Abell TJ. Conditioned medium for stiumulated mononuclear leukocytes augments human neutrophil- mediarted killing of a virulent Acanthamoeba sp. Infect Immun, 1986; 51: 607-617.
(34) Marcianno-Cabral F, Toney DM. The interaction of Acanthamoeba sp. with activated macrophages and with macrophage cell lines. J Eukaryot Microbiol, 1998; 45: 452-458.
(35) John DT, Weikm RR, Adams AC. Immunization of mice against Naegleria fowleri infection. Infect Immun, 1977; 16: 817-820.
(36) Soltow SM, Bremmer GM. Synergistic activity of azithromycin and amphoteracin B against Naegleria fowleri in vitro and in vivo in a mouse model of primary amebic meningoencephalitis. Anti Microb Agents Chemoth, 2007; 51: 23-27.
RAMANUJ LAHIRI & JAMES L. KRAHENBUHL
Laboratory Research Branch, National Hansen's Disease Programs, Health Resources Service Administration, Baton Rouge, LA 70803 USA
Accepted for publication 28 August 2008
Correspondence to: James L. Krahenbuhl, PhD, Director, National Hansen's Disease Programs, 1770 Physicians Park Dr., Baton Rouge, LA 70816, USA (Tel: 225-756-3776; Fax: 225-578-9856; e-mail: firstname.lastname@example.org)
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|Author:||Lahiri, Ramanuj; Krahenbuhl, James L.|
|Date:||Dec 1, 2008|
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