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High-Throughput Carbon Substrate Profiling of Mycobacterium ulcerans Suggests Potential Environmental Reservoirs

High-Throughput Carbon Substrate Profiling of Mycobacterium ulcerans Suggests Potential Environmental Reservoirs

  • Dezemon Zingue, 
  • Amar Bouam, 
  • Muriel Militello, 
  • Michel Drancourt
PLOS
x

Abstract

Background

Mycobacterium ulcerans is a close derivative of Mycobacterium marinum and the agent of Buruli ulcer in some tropical countries. Epidemiological and environmental studies pointed towards stagnant water ecosystems as potential sources of M. ulcerans, yet the ultimate reservoirs remain elusive. We hypothesized that carbon substrate determination may help elucidating the spectrum of potential reservoirs.

Methodology/Principal findings

In a first step, high-throughput phenotype microarray Biolog was used to profile carbon substrates in one M. marinum and five M. ulcerans strains. A total of 131/190 (69%) carbon substrates were metabolized by at least one M. ulcerans strain, including 28/190 (15%) carbon substrates metabolized by all five M. ulcerans strains of which 21 substrates were also metabolized by M. marinum. In a second step, 131 carbon substrates were investigated, through a bibliographical search, for their known environmental sources including plants, fruits and vegetables, bacteria, algae, fungi, nematodes, mollusks, mammals, insects and the inanimate environment. This analysis yielded significant association of M. ulcerans with bacteria (p = 0.000), fungi (p = 0.001), algae (p = 0.003) and mollusks (p = 0.007). In a third step, the Medline database was cross-searched for bacteria, fungi, mollusks and algae as potential sources of carbon substrates metabolized by all tested M. ulcerans; it indicated that 57% of M. ulcerans substrates were associated with bacteria, 18% with alga, 11% with mollusks and 7% with fungi.

Conclusions

This first report of high-throughput carbon substrate utilization by M. ulcerans would help designing media to isolate and grow this pathogen. Furthermore, the presented data suggest that potential M. ulcerans environmental reservoirs might be related to micro-habitats where bacteria, fungi, algae and mollusks are abundant. This should be followed by targeted investigations in Buruli ulcer endemic regions.

Author Summary

Buruli ulcer is a neglected tropical disease which has been reported in over 33 countries, mainly located in tropical and subtropical regions. It is caused by Mycobacterium ulcerans, an environmental pathogen associated to slow-moving water. The sources and reservoirs of M. ulcerans remain elusive and are still to be discovered. In a first attempt to address this issue we used high-throughput carbon substrate profiling of M. ulcerans. The reported results show that some nutrients, naturally available in organisms present in M. ulcerans’ environment, are metabolized by this microorganism. This carbon substrate determination should help improve the culture of M. ulcerans as well as suggest potential environmental reservoirs in Buruli ulcer endemic regions.

Introduction

Mycobacterium ulcerans is the etiologic agent of Buruli ulcer, a disabling infection of the cutaneous and subcutaneous tissues [13]. M. ulcerans has been discovered in Bairnsdale, Australia, where Buruli ulcer was initially described [4,5]. Buruli ulcer is a World Health Organization notifiable infection and has been reported at least once by 33 countries located in the rural tropical regions of Africa and South America, in addition to Australia and Japan [6,7]. Over the past ten years, 83.6% (80.89–86.30) of cases were declared by eight West African countries [8]. In these highly endemic regions, the exact reservoirs of M. ulcerans remain elusive [6, 911]. However, epidemiological studies conducted in West African countries all indicated a significant association between the prevalence of Buruli ulcer and the contact of populations with stagnant water sources [1217] through routine activities such as washing, swimming, fishing and farming [18,19]. A significant progress was recently made by narrowing the possible sources down to contacts with rice fields in Côte d’Ivoire which are sources of stagnant water [16,18,20,21]. Parallel environmental investigations of stagnant water [20,22], water insects [2325], fishes [26,27] and aquatic mammals [12] showed the presence of PCR-amplified M. ulcerans insertion sequences (IS) IS2404, IS2606 and KR-B gene. Furthermore, M. ulcerans partial DNA coding sequences were also recovered from the soil in the vicinity of stagnant water [20,22,26,28,29]. This finding was strengthened by an experimental study confirming a four-month survival of M. ulcerans in soil [30]. M. ulcerans DNA has been also detected in water plants [28,31] and in Thryonhuomys swinderianus (agouti), a small mammal causing damages to rice fields and in close contacts with rural populations in West Africa [20].

Moreover, this compelling amount of information concerning the presence of M. ulcerans DNA-related sequences found in the environment has been strengthened by the isolation of five wild strains from those sources [3,32,33].

Here, we propose that a characterization of the metabolic profile of M. ulcerans may give clues to better define its natural environment including its environmental reservoirs. In this perspective, we used the Biolog Phenotype MicroArray (Biolog Inc., Hayward, CA) for high-throughput carbon substrate profiling of M. ulcerans. Indeed, Biolog Phenotype MicroArray was previously used to classify and characterize heterotrophic microbial communities from different natural habitats according to their sole-carbon-source utilization profiles [34]. Accordingly, this approach previously unraveled the phenotypic patterns of some Mycobacterium tuberculosis complex mycobacteria [35] and Mycobacterium avium subsp. paratuberculosis [36]. It is used here in the context of unique carbon metabolisms such as chitinase exhibited by M. ulcerans [37].

Materials and Methods

M. ulcerans strains

This experimental study investigated M. ulcerans strain CU001 (a gift from Pr V. Jarlier, Paris, France), a clinical isolate representative of the West African epidemic, M. ulcerans ATCC 19423 isolated in Australia, M. ulcerans ATCC 33728 isolated in Japan, M. ulcerans ATCC 25900 isolated in the USA and Mycobacterium buruli ATCC 25894 isolated in Uganda [38]. These strains were manipulated into a BLS3 laboratory and a clinical isolate of Mycobacterium marinum was isolated in our laboratory [39]. All strains were cultured at 30°C in Middlebrook 7H10 agar medium supplemented with 10% (v/v) oleic acid/albumin/dextrose/catalase (OADC) (Becton Dickinson, Sparks, MD, USA) and 0.5% (v/v) glycerol in a microaerophilic atmosphere for one week for M. marinum and four weeks for M. ulcerans.

Biolog Phenotype microarray

The Biolog Phenotype MicroArray (Biolog Inc.), which consists of 96-well microtiter plates containing each a defined medium that incorporates a unique carbon source (plates PM1 and PM2A for 190 different carbon sources) plus a dye indicator of cell respiration was used, according to the previously reported standard Biolog Inc. protocol [40,41]. M. ulcerans and M. marinum colonies were removed from Middlebrook 7H10 medium using a cotton swab previously dipped in 0.1% Tween 80 (WGK Germany, Sigma Aldrich). Mycobacteria were taken with the wet swab off the agar plate culture by gently sweeping on the surface of the culture and then rubbed against the wall of a dry glass tube containing glass beads. The cells were then suspended in GN/GP-IF-0a (Biolog inoculating fluid n°133), the suspension was vigorously vortexed, passed three times through a 29-gauge needle in order to separate aggregates and adjusted to 81% transmittance using a turbidimeter (Biolog Inc). The PM-additive solutions for each plate were prepared according to Table 1. The inoculating fluid (Table 2) consisted of 20 mL of IF-0a GN/GP (1.2 x), 0.24 mL of dye mix G (100x) and 2.0 mL of PM additive (12x) added to the M. ulcerans or M. marinum suspension in IF-0a GN/GP (1.76 mL). Each PM plate was then inoculated in duplicate with 100 μL of inoculating fluid. The PM plates were incubated in the OmniLog PM System (Biolog Inc.) which measures the growth of mycobacteria every fifteen minutes for eight days at 30°C. In each well the substrate was reduced to a purple color which was directly proportional to the growth of the mycobacteria. The intensity of the purple color was recorded as dye reduction value, which was then plotted as area under the curve (AUC) by Biolog's parametric software. Negative control wells containing non-inoculated additive solutions in each PM1 and PM2 plates were run at the same time as a quality control element. The threshold separating the wells which exhibited a positive reaction from those with a negative reaction was set for each plate according to the value of the area under the curve (AUC) of the negative control Well (NCW). We defined moderately positive growing wells (MPW) and highly positive growing wells (HPW) as follows: MPW is when the AUC value of the well is equal to or lower than 1.25 times the AUC value of the negative control well, and HPW is when the AUC value of the well is equal to or higher than 1.50 times the AUC value of the negative control. PM plates were further examined visually at the end of each incubation period to ensure an independent verification of the results.

Environmental sources of substrates metabolized by all tested M. ulcerans strains

In order to find the potential environmental origin of the carbon substrates metabolized by M. ulcerans, we used the PubMed database to obtain information on the environmental sources for each of the 190 carbon substrates present in the PM1and PM2 plates. The environmental sources were organized in 10 categories (plants, fruits and vegetables, bacteria, algae, fungi, nematodes, mollusks, mammals, insects and the inanimate environment). The Chi-square test was used to compare the proportion of each category for substrates not metabolized by M. ulcerans versus substrates metabolized by all tested M. ulcerans strains; a P value < 0.05 was used as the criterion for statistical significance. We then used the PubMed database to match each substrate, used as a key-word, with all environmental sources significantly associated with substrates metabolized by all tested M. ulcerans strains, used as the second key-word (e.g., D-glucosamine and fungi). We calculated the number of hits obtained in this research and compared it to the number of hits obtained by searching only for the key word corresponding to the environmental sources (e.g., fungi).

Results

Carbone substrate profiling in M. marinum and M. ulcerans

The negative control wells remained negative in all the PMs plates, and results obtained with the five M. ulcerans strains and the M. marinum strain were duplicated. A total of 131/190 (69%) carbon substrates were metabolized by at least one of the five M. ulcerans strains, including 28/190 (15%) carbon substrates common to the five M. ulcerans strains and 16/190 (8%) carbon substrates metabolized by only one M. ulcerans strain (Table 3). A total of 21/28 (75%) substrates metabolized by all tested M. ulcerans strains were also metabolized by M. marinum (Table 3). In detail, 17/95 (18%) carbon sources in PM1 plates were metabolized by all M. ulcerans strains and comprised D-glucose-6-phosphate, D-ribose, L-asparagine, uridine, D-fructose-6-phosphate, adenosine, inosine, acetoacetic acid, methyl pyruvate, L-malic acid, D-psicose, L-lyxose, glucuronamide, pyruvic acid, L-galactonic acid-g-lactone, D-galacturonic acid and phenylethylamine. Six of these substrates exhibited a strong positive reaction (D-ribose, L-malic acid, L-lyxose, glucuronamide, pyruvic acid and D-galacturonic acid). Then, 11/95 (11.5%) carbon sources in PM2 plates metabolized by all M. ulcerans strains comprised D-raffinose, butyric acid, D-glucosamine, α-keto-valeric acid, 5-keto-D-gluconic acid, oxalomalic acid, sorbic acid, L-isoleucine, L-lysine, putrescine and dihydroxyacetone. Five of these substrates exhibited a strong positive reaction (D-glucosamine, 5-keto-D-gluconic acid, oxalomalic acid, sorbic acid and dihydroxyacetone). A total of 21/28 carbon substrates were also metabolized by M. marinum leaving D-galacturonic acid, uridine, methyl pyruvate, α-keto-valeric acid, L-isoleucine, L-lysine and putrescine as the only substrates specific to M. ulcerans (Table 3).

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Table 3. Carbone substrates metabolized by at least one of the five tested M. ulcerans strains compared with carbon substrates metabolized by Mycobacterium marinum on Biolog PM1 & PM2 plates.

https://doi.org/10.1371/journal.pntd.0005303.t003

Environmental sources for substrates metabolized by all tested M. ulcerans strains

Comparing the potential environmental sources in search of substrates metabolized by all tested M. ulcerans strains versus non-metabolized substrates, we found a significant association between M. ulcerans metabolized substrates and bacteria (p = 0.000), fungi (p = 0.001), algae (p = 0.003) and mollusks (p = 0.007). The differences were not significant for plants (p = 0.535), fruits and vegetables (p = 0.870), mammals (p = 0.064), insects (p = 0.234) and the inanimate environment (p = 0.477). No carbon source was found to be associated with nematodes. Further MedLine research incorporating bacteria, fungi, algae and mollusks as keywords disclosed that 16/28 (57%) metabolized substrates were associated with bacteria, 5/28 (18%) were associated with alga, 3/28 (11%) were associated with mollusks and 2/28 with fungi. Discarding bacteria because of a potential bias since Biolog was designed for the study of bacterial metabolism, 15/28 (54%) metabolized substrates were associated with fungi whereas 6/28 (21%) were associated with the algae and 6/28 (21%) with mollusks (Table 4).

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Table 4. Cross-search of the Medline database (May, 2016) for fungi, mollusks and algae as potential sources of carbon substrates; and substrates metabolized by all tested M. ulcerans strains.

The total number of hits for fungi, mollusks and algae is indicated into brackets. Each cell contains the number of cross-hits and green cells indicate the higher relative hit for each carbon source.

https://doi.org/10.1371/journal.pntd.0005303.t004

Discussion

We determined that five different strains of M. ulcerans could use 28 different substrates as sources of carbon. These results were authenticated by the negativity of the negative controls introduced in every plate and the reproduction of data over two replicates. Moreover, stringent criteria were used to ensure the predictive value of the positive results. However, only seven of these 28 substrates were found to be specifically used by M. ulcerans and not by the phylogenetically closest species M. marinum. Three of these seven carbon sources indeed contain indispensable amino-acids.

The carbon sources here determined for M. ulcerans may by incorporated in culture media in the perspective of enhancing the isolation and culture of this pathogen. Indeed, M. ulcerans is a slow-growing mycobacterium and the availability of an improved method for its culture would improve the diagnosis of Buruli ulcer patients and the quest for environmental reservoirs [32]. As an example, it has been shown that the incorporation of chitin into the Middlebrook 7H9 broth enhances the growth of M. ulcerans [37]. Accordingly, our study points towards a possible association of M. ulcerans with fungi as a potential source of chitin, a polysaccharide possibly degraded by M. ulcerans’ genome-encoded chitinase [42]. Likewise, the other carbon sources here disclosed should be tested for their potential to increase the cultivation of M. ulcerans.

Moreover, our analyses suggested that M. ulcerans may have found some sources of carbon in microbial communities including alive and dead bacteria, fungi and algae. As for bacteria, it has been previously reported that M. ulcerans was isolated in environments where 17 other mycobacteria species were also isolated, including M. fortuitum as a constant co-inhabitant [3, 32, 33]. These results suggest cross-feeding between various bacterial complexes including mycobacteria, for the acquisition of carbon. Likewise, green algae extracts have been shown to halve the in vitro doubling time of M. ulcerans and promote the formation of biofilm [31]. We observed that M. ulcerans metabolizes D-galacturonic acid, the main component of pectin contained in the primary cell walls of terrestrial plants, and putrescine, a foul-smelling chemical derived from the decomposition of dead plants, which indicates that M. ulcerans may live in assemblages of dead aquatic plants. This finding is reinforced by the observation that M. ulcerans’s genome encodes five putative cutinases. Cutinases are mainly produced by phytopathogenic fungi to hydrolyze cutin (a main component of the cuticle which covers the aerial surfaces of plants) during plant colonization process [43].

Green algae are among the main food of freshwater mollusks pointed out in our study; mollusks are herbivores like other species of the freshwater snail family [44]. The principal genera of mollusks met in freshwater in West Africa are Bulinus, Planorbis, Pila, Lanistes, Melania, Bithynia, Lymnaea, Biomphalaria, Mutela, Aspatharia and Sphaerium [23,45]. Previous molecular investigations reported the detection of specific M. ulcerans DNA sequences in Bulinus spp. [23,46], in Planorbis spp. [23] and in mollusks of different Gastropoda order, Bivalvia order and Basommatophora order [26]. Furthermore, the experimental infection of Pomacea canaliculata (Ampullariidae) and Planorbis planorbis (Planorbidae) by plants contaminated by M. ulcerans- showed through optic microscopy digestive tract observation that snails remained infected by viable mycobacteria up to 25 days [23]. Small mollusks are also known to be a prey for water bugs which are involved in the transmission of M. ulcerans in Buruli ulcer endemic regions [3]. In West Africa, approximately 76% of the population lives next to rivers, lakes, and other water bodies contaminated with intermediate hosts such as snails [47].

In conclusion, our study is suggesting paths to improve culture media for the enhanced isolation of M. ulcerans by mimicking the natural ecosystem of M. ulcerans which is probably living in microbial communities with other bacteria, fungi and algae. These data support the recent hypothesis that mollusks could be part of a larger food chain including several hosts giving appropriate shelters to M. ulcerans, as recently reported [48]. Small mollusks should be further investigated using culture-based appropriate methods in the search for M. ulcerans.

Acknowledgments

The authors acknowledge Pablo Gluschankof for his fruitful discussion of the manuscript’s content.

Author Contributions

  1. Conceptualization: MD.
  2. Methodology: DZ AB.
  3. Software: MM.
  4. Validation: DZ AB MM.
  5. Writing – original draft: DZ AB MD.

References

  1. 1. Doig KD, Holt KE, Fyfe JAM, Lavender CJ, Eddyani M, Portaels F, et al. On the origin of Mycobacterium ulcerans, the causative agent of Buruli ulcer. BMC Genomics 2012; 13, 258. pmid:22712622
  2. 2. Josse R, Guedenon A, Darie H, Anagonou S, Portaels F, Meyers WM. [Mycobacterium ulcerans cutaneous infections: Buruli ulcers]. Medecine tropicale: revue du Corps de sante colonial 1995; 55(4), 363–373.
  3. 3. Portaels F, Meyers WM, Ablordey A, Castro AG, Chemlal K, de Rijk P, et al. First Cultivation and Characterization of Mycobacterium ulcerans from the Environment. PLoS Negl Trop Dis. 2008; 2(3), e178. pmid:18365032
  4. 4. Portaels F, Fonteyene PA, de Beenhouwer H, de Rijk P, Guedenon A, Hayman J, et al. Variability in 3' end of 16S rRNA sequence of Mycobacterium ulcerans is related to geographic origin of isolates. J Clin Microbiol. 1996; 34(4), 962–965. pmid:8815117
  5. 5. Maccallum P, Tolhurst JC, Buckle G, Sissons HA A new mycobacterial infection in man. J Pathol Bacteriol. 1948; 60(1), 93–122.
  6. 6. Johnson PD, Azuolas J, Lavender CJ, Wishart E, Stinear TP, Hayman JA, et al. Mycobacterium ulcerans in mosquitoes captured during outbreak of Buruli ulcer, southeastern Australia. Emerg Infect Dis. 2007; 13(11), 1653–1660. pmid:18217547
  7. 7. Stinear TP, Seemann T, Pidot S, Frigui W, Reysset G, Garnier T, et al. Reductive evolution and niche adaptation inferred from the genome of Mycobacterium ulcerans, the causative agent of Buruli ulcer. Genome Res. 2007; 17(2), 192–200. pmid:17210928
  8. 8. WHO. World: Distribution of buruli ulcer, 2014 WHO Annual meeting on Buruli ulcer 2015.
  9. 9. Benbow ME, Williamson H, Kimbirauskas R, McIntosh MD, Kolar R, Quaye C, et al. Aquatic invertebrates as unlikely vectors of Buruli ulcer disease. Emerg Infect Dis. 2008; 14(8), 1247–1254. pmid:18680648
  10. 10. Garchitorena A, Ngonghala CN, Texier G, Landier J, Eyangoh S, Bonds MH, et al. Environmental transmission of Mycobacterium ulcerans drives dynamics of Buruli ulcer in endemic regions of Cameroon. Sci Rep. 2015; 5, 18055. pmid:26658922
  11. 11. Kenu E, Nyarko KM, Seefeld L, Ganu V, Käser M, Lartey M, et al. Risk Factors for Buruli Ulcer in Ghana—A Case Control Study in the Suhum-Kraboa-Coaltar and Akuapem South Districts of the Eastern Region. PLoS Negl Trop Dis. 2014; 8(11), e3279. pmid:25411974
  12. 12. Narh CA, Mosi L, Quaye C, Dassi C, Konan DO, Tay SCK, et al. Source Tracking Mycobacterium ulcerans Infections in the Ashanti Region, Ghana. PLoS Negl Trop Dis. 2015; 9, e0003437. pmid:25612300
  13. 13. Addo P, Adu-Addai B, Quartey M, Abbas M, Okang I, Owusu E, et al. Clinical and Histopathological Presentation of Buruli Ulcer in Experimentally Infected Grasscutters (Thryonomys swinderianus). Intern J Trop Med. 2006; 3(2).
  14. 14. Mensah-Quainoo EK. A study of the magnitude and determinants of Buruli ulcer disease in the Ga District of Ghana. International Conference on Buruli ulcer Control and Research; 6–8 July 1998; Yamoussoukro, Cote d’Ivoire 1998.
  15. 15. Peraudin ML, Herrault A, Desbois JC Ulcère cutanée à Mycobacterium ulcerans (ulcère de Buruli). Annales de Pédiatrie 1980; 27(10), 687–692. pmid:7212557
  16. 16. Brou T, Broutin H, Elguero E, Asse H, Guegan JF Landscape diversity related to Buruli ulcer disease in Cote d'Ivoire. PLoS Negl Trop Dis. 2008; 2(7), 0000271.
  17. 17. Johnson RC, Makoutodé M, Sopoh GE, Elsen P, Gbovi J, Pouteau LH, et al. Buruli Ulcer Distribution in Benin. Emerg Infect Dis. 2005; 11(3), 500–501. pmid:15789490
  18. 18. N’krumah RTAS, Koné B, Tiembre I, Cissé G, Pluschke G, Tanner M, et al. Socio-Environmental Factors Associated with the Risk of Contracting Buruli Ulcer in Tiassalé, South Côte d’Ivoire: A Case-Control Study. PLoS Negl Trop Dis. 2016; 10(1), e0004327. pmid:26745723
  19. 19. Aiga H, Amano T, Cairncross S, Domako JA, Nanas OK, Coleman S Assessing water-related risk factors for Buruli ulcer: a case-control study in Ghana. Am J Trop Med Hyg. 2004; 71(4), 387–392. pmid:15516631
  20. 20. Tian RB, Niamke S, Tissot-Dupont H, Drancourt M. Detection of Mycobacterium ulcerans DNA in the Environment, Ivory Coast. PLoS One 2016; 11(3): e0151567 pmid:26982581
  21. 21. Ahoua L, Guetta A, Ekanza E, Bouzid S, N’Guessan R, Dosso M Risk factors for Buruli ulcer in Côte d’Ivoire: Results of a cas-control study, August 2001. Afr J Biotechnol. 2009; 8, 536–546.
  22. 22. Vandelannoote K, Durnez L, Amissah D, Gryseels S, Dodoo A, Yeboah S, et al. Application of real-time PCR in Ghana, a Buruli ulcer-endemic country, confirms the presence of Mycobacterium ulcerans in the environment. FEMS Microbiol Lett. 2010; 304(2), 191–194. pmid:20146745
  23. 23. Marsollier L, Severin T, Aubry J, Merritt RW, Saint Andre JP, Legras P, et al. Aquatic snails, passive hosts of Mycobacterium ulcerans. Appl Environ Microbiol. 2004; 70(10), 6296–6298. pmid:15466578
  24. 24. Marsollier L, Robert R, Aubry J, Saint Andre JP, Kouakou H, Legras P, et al. Aquatic insects as a vector for Mycobacterium ulcerans. Appl Environ Microbiol. 2002; 68(9), 4623–4628. pmid:12200321
  25. 25. Konan KL, Doannio JM, Coulibaly NG, Ekaza E, Marion E, Asse H, et al. [Detection of the IS2404 insertion sequence and ketoreductase produced by Mycobacterium ulcerans in the aquatic Heteroptera in the health districts of Dabou and Tiassale in Cote d'Ivoire]. Med Sante Trop. 2015; 25(1), 44–51. pmid:25499000
  26. 26. Williamson HR, Benbow ME, Nguyen KD, Beachboard DC, Kimbirauskas RK, McIntosh MD, et al. Distribution of Mycobacterium ulcerans in buruli ulcer endemic and non-endemic aquatic sites in Ghana. PLoS Negl Trop Dis. 2008; 2(3), e205. pmid:18365034
  27. 27. Zogo B, Djenontin A, Carolan K, Babonneau J, Guegan J-F, Eyangoh S, et al. A Field Study in Benin to Investigate the Role of Mosquitoes and Other Flying Insects in the Ecology of Mycobacterium ulcerans. PLoS Negl Trop Dis. 2015; 9(7), e0003941. pmid:26196901
  28. 28. Amissah NA, Gryseels S, Tobias NJ, Ravadgar B, Suzuki M, Vandelannoote K, et al. Investigating the Role of Free-living Amoebae as a Reservoir for Mycobacterium ulcerans. PLoS Negl Trop Dis. 2014; 8(9), e3148. pmid:25188535
  29. 29. Williamson HR, Benbow ME, Campbell LP, Johnson CR, Sopoh G, Barogui Y, et al. Detection of Mycobacterium ulcerans in the Environment Predicts Prevalence of Buruli Ulcer in Benin. PLoS Negl Trop Dis. 2012; 6(1), e1506. pmid:22303498
  30. 30. Tian RD, Lepidi H, Nappez C, Drancourt M Experimental Survival of Mycobacterium ulcerans in Watery Soil, a Potential Source of Buruli Ulcer. Am J Trop Med Hyg. 2016; 94(1), 89–92. pmid:26526927
  31. 31. Marsollier L, Stinear T, Aubry J, Saint André JP, Robert R, Legras P, et al. Aquatic Plants Stimulate the Growth of and Biofilm Formation by Mycobacterium ulcerans in Axenic Culture and Harbor These Bacteria in the Environment. App Environm Microbiol. 2004; 70(2), 1097–1103.
  32. 32. Aboagye SY, Danso E, Ampah KA, Nakobu Z, Asare P, Otchere ID, et al. Isolation of Nontuberculous Mycobacteria from the Environment of Buruli Ulcer Endemic Communities in Ghana. App Environ Microbiol. 2016; 6, 2016.
  33. 33. Marsollier L, Aubry J, Saint-andré J, Robert R, Legras P, Manceau A. Ecology and transmission of Mycobacterium ulcerans. 2003;51:490–5.
  34. 34. Garland JAYL, Mills AL. Classification and Characterization of Heterotrophic Microbial Communities on the Basis of Patterns of Community-Level Sole-Carbon-Source Utilization. 1991;57(8):2351–9.
  35. 35. Khatri B, Fielder M, Jones G, Newell W, Abu-Oun M, Wheeler PR High Throughput Phenotypic Analysis of Mycobacterium tuberculosis and Mycobacterium bovis Strains' Metabolism Using Biolog Phenotype Microarrays. PLoS ONE 2013; 8(1), e52673. pmid:23326347
  36. 36. Chen J-W, Scaria J, Chang Y-F Phenotypic and Transcriptomic Response of Auxotrophic Mycobacterium avium subsp. paratuberculosis leuD Mutant under Environmental Stress. PLoS ONE 2012; 7(6), e37884. pmid:22675497
  37. 37. Sanhueza D, Chevillon C, Colwell R, Marion E, Marsollier L. Chitin promotes Mycobacterium ulcerans growth. J er. 2016;2010(October 2015):1–6.
  38. 38. Schoröder K. H. Investigation into the relatioship of M. ulcerans to M. burili and other mycobacteria. American review of resperatory disease 1975; 111, 559–562.
  39. 39. Bouricha M, Castan B, Duchene-Parisi E, Drancourt M Mycobacterium marinum infection following contact with reptiles: vivarium granuloma. Int J Infect Dis. 2014; 21, 17–18. pmid:24530276
  40. 40. Bochner BR Global phenotypic characterization of bacteria. Fems Microbiol Rev. 2009; 33(1), 191–205. pmid:19054113
  41. 41. Bochner BR, Gadzinski P, Panomitros E Phenotype MicroArrays for High-Throughput Phenotypic Testing and Assay of Gene Function. Genome Res. 2001; 11(7), 1246–1255. pmid:11435407
  42. 42. Stinear TP, Seemann T, Pidot S, Frigui W, Reysset G, Garnier T, et al. Reductive evolution and niche adaptation inferred from the genome of Mycobacterium ulcerans, the causative agent of Buruli ulcer. Genome Res. 2007;17(2):192–200. pmid:17210928
  43. 43. Côtes K, Bakala N’Goma JC, Dhouib R, Douchet I, Maurin D, Carrière F, et al. Lipolytic enzymes in Mycobacterium tuberculosis. Appl Microbiol Biotechnol. 2008;78(5):741–9. pmid:18309478
  44. 44. El-Assal FM, Shanab SMM, Abou-El-Hassan AA, Mahmoud KMA. Effect of some algal species on the snail intermediate hosts of schistosomiasis in Egypt II. Growth, infection and mortality rates. Egypt J Phycol. 2005; 6(1), 93–110.
  45. 45. Thiam N, Diallo A Intégration de la biodiversité d'eau douce dans le processus de développement en Afrique: Module de formation des formateurs sur Le suivi des Mollusques d’eau douce. Wetlands International Afrique [serial on the Internet]. 2010. https://cmsdata.iucn.org/downloads/module_mollusques_fr.pdf.
  46. 46. Kotlowski R, Martin A, Ablordey A, Chemlal K, Fonteyne P-A, Portaels F One-tube cell lysis and DNA extraction procedure for PCR-based detection of Mycobacterium ulcerans in aquatic insects, molluscs and fish. J Med Microbiol. 2004; 53(9), 927–933.
  47. 47. Hotez PJ, Kamath A Neglected Tropical Diseases in Sub-Saharan Africa: Review of Their Prevalence, Distribution, and Disease Burden. PLoS Negl Trop Dis. 2009, 3(8), e412. pmid:19707588
  48. 48. Morris AL, Guégan J, Andreou D, Marsollier L, Carolan K, Le Croller M, et al. Deforestation-driven food-web collapse linked to emerging tropical infectious disease, Mycobacterium ulcerans. 2016;1–7.