Measuring and reducing biofilm in mosquito rearing containers

doi:10.21203/rs.2.22664/v2

Download PDF

Short report

Measuring and reducing biofilm in mosquito rearing containers

https://doi.org/10.21203/rs.2.22664/v2

This work is licensed under a CC BY 4.0 License

Journal Publication

published 02 Sep, 2020

Read the published version in Parasites & Vectors →

You are reading this latest preprint version

Background: Mosquito rearing containers contain organic-rich water that nourishes numerous bacteria, some of which are capable of forming biofilms. Biofilm is broadly an extracellular polymeric matrix (EPS) in which living bacteria occur, and the accumulation of biofilm is possible during routine stock-keeping as most of these containers are re-used. Whether biofilm has an effect on the mosquito rearing is not a question that has been investigated, nor have measures to reduce biofilm in this context been systematically studied.

Methods: We measured biofilm accumulation in standard rearing containers by staining with crystal violet and determining the OD using a spectrophotometer. We also treated rearing containers with 0.1% sodium hypochlorite to determine its effectiveness in reducing biofilm abundance. Lastly, we performed an analysis of the relationship between the occurrence of biofilm and the likelihood of microbial blooms that were associated with larval death during trials of larval diets.

Results: We observed that soaking rearing containers overnight in 0.1% sodium hypochlorite greatly reduced biofilm, but we observed no relationship between the use of containers that had not been treated with bleach and subsequent microbial blooms.

Conclusions: Larva rearing leaves detectable biofilm. While we were unable to correlate microbial blooms with the presence of biofilm, as a precaution, we recommend that plastic containers that are re-used be treated with 0.1% sodium hypochlorite bleached occasionally.

Parasitology

mosquito rearing

biofilm

bacteria

aquaculture

pathogens

By far the most common containers used for rearing mosquito larvae are plastic or metal trays. These are usually re-used and may be cleaned in a number of ways including with detergent or water alone, and they are sometimes treated with bleach or autoclaved after washing. In our experience, many insectary staff are reluctant to use detergents for fear of contaminating the containers with any residue that might harm larvae, but we are aware of no systematic efforts to determine how likely this is.

Because mosquito rearing is not aseptic, introduction of pathogens is always a possibility. In fish aquaculture, which has similar characteristics, when even non-pathogenic opportunistic bacteria become excessively abundant, death can occur [1]. In mosquito larval culture substantial bacterial growth is usually evidenced by extremely turbid water, a foul odor and can result in complete larval death in the container. We will refer to this event simply as a ‘microbial bloom’. The usual method to avoid this is to prevent excess amounts of food and to maintain a larval density that keeps the amount of food per larva in the container from becoming excessive, however this results in a chronic state of food restriction [2].

Biofilm occurs on surfaces that are exposed to biological material in aqueous liquids. They consist of bacteria embedded in a matrix—the extracellular polymeric substances (EPS) –that many bacteria secrete consisting of polysaccharides, lipids, nucleic acids and proteins [3, 4]. The EPS itself is a complex microhabitat that protects and promotes the persistence of the bacteria that reside in it and contribute to its structure. It is difficult to remove, being resistant to desiccation, ultraviolet light and detergents [5].

While biofilms occur in diverse environments such as industrial equipment, human health products and soil, in the context of mosquito rearing, aquaculture provides an analogous source of experience in managing issues associated with biofilm formation. Indeed, previous studies have reported the potential for harm that biofilms present in aquaculture systems; King et al. [1] found fish and human pathogens present in biofilms in aquaculture facilities. Although most of the fish pathogens identified were opportunistic and non-detrimental, three were known to cause significant disease in marine fish populations. Furthermore, Skjermo et al. [6] described the negative effect of microbial growth on the early stages of marine larvae. High larval densities, decay from dead larvae, and low water exchange contributed to intense biofilm formation that ultimately led to increased mortality or inferior adults. Such conditions are reminiscent of typical mosquito larva rearing conditions.

Biofilms can be extremely difficult to remove and physical measures alone—scrubbing or high-pressure spraying—are not completely effective, often leaving largely invisible source colonies of contaminating bacteria. The use of chemicals, such as sodium hypochlorite, has been shown to significantly reduce the presence of biofilm depending on the substrate [5]. We therefore chose this widely available and inexpensive chemical to determine its effect on biofilm presence and amount in mosquito rearing containers.

We report the results of a simple method to detect biofilm in mosquito rearing containers and the effect of bleaching on removing biofilm. The preliminary results of the relationship between rearing larvae in untreated used larval containers compared to new containers is also reported. The likelihood of microbial blooms, a correlate of biofilm that might cause substantial or total mortality of rearing stock, was investigated. We also analyzed the effect of larval food type, form and concentration and whether the development of biofilm varies between the mosquito species Aedes aegypti and Anopheles gambiae. We will generally refer to the residual substances on the submerged surfaces of rearing trays and dishes as ‘biofilm.’

Effects of mosquito species, food type and quantity

The rearing methods and experimental material that were analyzed in the observations reported here have been published previously [4]. Briefly, 80 L1 An. gambiae ‘G3’ or Ae. aegypti ‘New Orleans’ strain larvae were reared in 150 mm Petri dishes containing approximately 100 ml of standard rearing water consisting of 0.3 g of pond salts (API, McLean, VA USA) per liter of type II purified water. After pupation, the containers that were to be reused were scrubbed with a wet sponge, rinsed in type II water and thoroughly air-dried. Alternatively, new containers were used. Four diets were used; two of these were custom formulations of a diet specifically designed for mosquitoes [9]. This diet consists of a 2:2:1 ratio (by weight) of bovine liver powder, tuna meal and Vanderzant vitamin mix. One formulation was prepared at CDC in Atlanta, GA using ‘Now’ brand liver powder (Bloomingdale, IL USA), tuna meal (AA Baits, Rock Ferry, Birkenhead, UK) and Vanderzant vitamin mix (Bio-Serv, Flemington, NJ, USA). The other formulation of the Damiens diet was prepared by Frontier Scientific Services (Newark, DE USA) using defatted, desiccated liver powder (product no. 1320; Frontier Scientific Services), Vanderzant vitamin mix (product no. F8045, Frontier Scientific Services) and the same lot of tuna meal as was used at CDC. The other two diets were commercially available fish foods; TetraMin Plus Flakes (Tetra GmbH, Melle, Germany) and Doctors Foster and Smith Koi Staple diet (Rhinelander, WI USA). Koi pellets were ground in a Miracle Model MR-300 Electric Grain and Flour Mill (Danbury, CT USA) followed by sieving and saving the particles that passed a 600 m standard sieve. The TetraMin was ground in a Black and Decker ‘SmartGrind’ coffee grinder (Beachwood, OH USA) to a consistency that passed through a 600 m sieve. These diet types will be identified as CDC, Frontier, TetraMin, and Koi respectively. Diet was fed at two concentrations, 1.6 or 3.2% on alternate days. We also fed one diet, Koi, as a pellet, the form in which it is supplied, or as a powder. Two pellets (equivalent to 52 mg/dish/day) were fed on alternate days. For details, consult the previously mentioned paper [4]. There were three dishes for each species, food and concentration.

Estimating Biofilm Abundance

A quantitative estimate of the amount of biofilm was made in situ by staining with crystal violet (Product no. C0775-25G, Millipore Sigma, Billerica, MA USA), essentially by the method of O’Toole [10]. A 0.1% solution of crystal violet was prepared and 10mL were added to each Petri dish. Dishes were stained with gentle agitation for 15 min and then rinsed 3 times with type II water and air-dried overnight. The bound crystal violet was eluted by adding 20mL of 30% acetic acid and incubated at room temperature for 15 min. The OD₅₉₀, which is the maximum absorbance of crystal violet, was then measured using a general-purpose UV/VIS spectrophotometer (720 series, Beckman Coulter, Atlanta, GA USA) in 1 cm light path polystyrene cuvettes. We confirmed that maximal absorbance was 590nm in the 30% acetic acid solution rather than 550 nm as described by O’Toole. Background absorbance was measured on eluant from new dishes and subtracted from the absorbance values of all samples. The spectrophotometer was zeroed against a blank containing 30% acetic acid after approximately every 5 measurements to be certain there was no drift in observations.

Cleaning method

The effect of overnight bleaching on biofilm abundance was also determined. Thirty, previously-used dishes (without knowledge of the specific food type or amount used) were allocated into two equal groups of 15; one group was treated overnight in a solution of 0.1% sodium hypochlorite prepared from an 8.5% sodium hypochlorite solution of concentrated Chloroxâ (Oakland, CA USA) bleach diluted in type II water. This formulation of bleach contained no fragrances or sodium hydroxide which are found in some household bleach solutions. After bleach treatment, the dishes were thoroughly rinsed three times in type II water and fully air-dried. The OD₅₉₀ was determined as above.

Food form

To explore whether the form in which the food was provided might affect the amount of biofilm that formed, we established an orthogonal set of six dishes for each species, half of which were provided with two Koi pellets and half were provided a 1.6% Koi slurry. Dishes were treated with crystal violet as mentioned above, and the OD₅₉₀was determined. As a side note, we observed that Aedes aegypti are active feeders that disintegrated the pellets rapidly whereas the pellets remained largely intact for up to 2 days when placed in dishes containing An. gambiae which we thought might affect the amount of biofilm. It should be kept in mind that the weight of Koi food when fed as a pellet was greater than when fed as a slurry.

Analyses

Statistical analyses were performed using R version 3.5.1 “Feather Spray” [11]. As OD₅₉₀, the measure of biofilm abundance, was a continuous variable, an ANOVA was used. The OD₅₉₀ data were strongly skewed and had a single outlier, these data were Ln-transformed for tractability in the analyses. The transformed values of the response variable (optical density) led to substantially improved model fit in all cases. As model fit was good, in no case was there evidence of particular influence by the outlier apparent in the un-transformed data.

Full models were fit with all main effects and interactions and the importance of terms was assessed by stepwise simplification. As the data are low replication, p<0.01 was used as a threshold for assessing the significance of interactions to avoid over-interpretation; p<0.05 was used for main effects. The occurrence (presence/absence) of total larval mortality which indicated microbial blooms as a function of whether the dish was previously used or new was analyzed by Fisher’s Exact Probability test. The effect of bleaching on the residual biofilm abundance was estimated by adjusted t-test to allow for the substantially different variance observed between the bleached and unbleached groups.

Effects of mosquito species, food type and quantity

There was no evidence of interactions between the species of mosquito being reared, the quantity or the type of food found in these data (p>0.01 in all cases) affecting the measured abundance of biofilm. No three-way interaction was detected between the main effects (F=1.75, d.f.=32,35,p=0.18) nor between food type and the dose it was given at (F=0.73, d.f.=35,38, p=0.54) or between food type and the mosquito species (F=1.57, d.f.=38,41, p=0.21). The hint of interaction suggesting that the biofilm abundance was higher at lower dose for An. gambiae did not pass our threshold for interactions and was potentially affected by the single outlier in the data (F=7.07, d.f.=41,42, p=0.012). Within the main effects, there was also no evidence of variation in biofilm abundance attributable to the species being reared (Mean _{+/- SE} Ln(OD₅₉₀) Ae. aegypti 4.6 _{+/- 0.14}, An. gambiae 4.77 _{+/- 0.02}, F=0.59, d.f.=42,43, p=0.48). There was, however, significant variation detected as a function of food type with Frontier and Tetramin leading to slightly lower biofilm abundance than the CDC & Koi formulations (F=3.84, d.f.=43,46, p=0.016, Figure 1). The level of food received was also found to affect the biofilm (F=7.81, d.f.=43,44, p=0.008), though this was in a counter-intuitive way with a higher biofilm being observed at the lower food level (1.6 % w/v = 4.9_{+/- 0.17}; 3.2 % w/v = 4.38_{+/- 0.16}, Figure 1).

In all, we observed 12 occurrences of microbial bloom as indicated by foul odor and extreme turbidity that preceded complete larval mortality. The likelihood of this happening was, however, independent of whether dishes had been used previously or were new (Fisher’s Exact test p=0.68).

Estimating Biofilm Abundance and Cleaning Method

Biofilm was readily seen in used dishes after staining with crystal violet (Figure 2). The residual biofilm abundance on plates was also observed in solution after elution. Bleaching greatly reduced residual biofilm (t=14.06, d.f.=23.05, p<0.001): the mean, untransformed OD₅₉₀ of the bleached group was 38.07 _{+/- 3.82} compared to 397.40 _{+/- 49.54} for the unbleached group.

Food Form

In these experiments, two factors were analyzed to determine their effect on the amount of biofilm in the dishes: the species of mosquito and whether the food was fed as a pellet or slurry; any interaction between the species and form of the food was also evaluated. There was no interaction identified and the effect of food form on biofilm amount did not vary with the species being reared (F=0.22, d.f.=8,9, p=0.65, Figure 3). Nor did the form, whether slurry or a pellet, affect this (F=1.90, d.f.=9,10, p=0.20). The biofilm did vary between species, however, and was substantially greater in the An. gambiae than in the Ae. aegypti dishes (F=26.44, d.f.=10,11, p<0.001).

Biofilm is a potential source of mosquito rearing difficulties, and even though autoclaving may kill the bacteria within the EPS, the biofilm matrix can persist, promoting subsequent biofilm formation. While we did not observe whether bleaching killed the bacteria within the biofilm, it greatly reduced the amount of detectable biofilm based on the crystal violet assay and it is reasonable to suppose that it also reduced the viability and persistence of associated bacteria. Among several chemical treatments tested, bleach has been observed to be one of the most effective methods to remove biofilm and is widely used for this purpose [5]. While we did not observe an association between microbial blooms and whether dishes had been used previously or not—which we interpret as correlating with more biofilm—it seems to be a reasonable precaution to treat rearing containers with bleach occasionally.

The data presented here should be interpreted cautiously. Even though the cleaning was considered well done, biofilm was still detectable in the crevices. Therefore, there is a relationship between the efforts of the individual cleaning the dishes and the amount that will persist, and even though biofilm was most evident in crevices, we also observed crystal violet staining generally across the flat surfaces of used dishes even where they appeared clean. The ability of the person cleaning the container to see obvious film may be the reason biofilm was lower in dishes that had contained An. gambiae fed at the 3.2% rate than in the 1.6%. In spite of more food being provided—and 3.2% is quite high—there was less residual biofilm. We speculate that because biofilm was easier to see at the higher food rate, it was also easier to detect and thoroughly remove. Because of the variability observed, it would be benefical to have a standard operating procedure in place to minimize inconsistencies in pan washing or to make bleach treatment a standard procedure.

The difference we observed in biofilm abundance between the species being reared may have its source in the feeding habits of these particular species. The voracious nature of Ae. aegypti could affect this in two ways: firstly, it may be that they consume the food so rapidly that biofilm formation is inhibited by lack of available nutrients, or secondly, they may also consume the biofilm itself by scraping and thus reduce it. These two points are not mutually exclusive, and both may act at the same time. The more delicate An. gambiae is known to have higher mortality under similar rearing conditions [2] and the nutrients made available through decomposition of larvae may themselves promote biofilm formation.

These simple observations provide insight into factors that affect biofilm formation in mosquito cultures. Simple bleach treatment seems to be a reasonable precaution to minimize it when using containers that will withstand this rather harsh oxidizer.

ANOVA: analysis of variance

EPS: extracellular polymeric substances

L1: stage 1 larvae

OD: optical density

Authors’ contributions

MQB designed the experiments, made observations and organized the data. CMH assisted performing the experiments and analyzing the biofilm. CMC performed the statistical analysis. All authors participated in drafting and revising the manuscript.

Author details

Division of Parasitic Diseases and Malaria, Centers for Disease Control and Prevention, Atlanta Georgia

Catherine M. Hunt & Mark Q. Benedict

Centre for Environmental Policy, Imperial College London, London, UK

C. Matilda Collins

Acknowledgments

The following reagents were obtained through the NIH Biodefense and Emerging Infections Research Resources Repository, NIAID, NIH: An. gambiae, ‘G3’ strain (MRA-12) and Ae aegypti ‘New Orleans’ strain (NR-49160).

The findings and conclusions in this report are those of the authors and do not necessarily represent the official position of the Centers for Disease Control and Prevention. Use of trade names is for identification only and does not imply endorsement by [the Centers for Disease Control and Prevention/the Agency for Toxic Substances and Disease Registry], the Public Health Service, or the U.S. Department of Health and Human Services.

Competing interests

The authors declare that they have no competing interests.

Availability of data and materials

The datasets generated during and/or analyzed during the current study are available from the corresponding author on reasonable request.

Consent for publication

Not applicable.

Ethics approval and consent to participate

Not applicable.

Funding

Funding provided by Target Malaria, a project that receives core funding from the Bill & Melinda Gates Foundation and from the Open Philanthropy Project Fund, an advised fund of Silicon Valley Community Foundation.

Shayo F, Kidima W, Thomas A, Mahande A, Mazigo H, Kweka E. Exposure of malaria vector larval habitats to domestic pollutants escalate insecticides resistance: experimental proof. Int J Trop Insect Sci. 2020;40(1). https://doi.org/10.1007/s42690-020-00123-w.
Antonio-Nkondjio, C, Youmsi-Goupeyou, M, Kopya, E, Tene Fossog, B, Njiokou, F, Costantini, C, & Awono-Ambene, P. Exposure to disinfectants (soap or hydrogen peroxide) increases tolerance to permethrin in Anopheles gambiae populations from the city of Yaoundé, Cameroon. Malaria Journal, 13(1), 259–7. http://doi.org/10.1186/1475-2875-13-296
King RK, Flick GJ, Pierson MD, Smith SA, Boardman GD, Coale CW. Identification of Bacterial Pathogens in Biofilms of Recirculating Aquaculture Systems. J Aquat Food Prod Technol. 2004;13(1):125–33.
Benedict MQ, Hunt CM, Vella MG, Gonzalez KM, Dotson EM, Collins CM. Pragmatic selection of larval mosquito diets for insectary rearing of Anopheles gambiae and Aedes aegypti. BioRxiv 740142 [Preprint]. August 19, 2019 [cited 2019 Sept 30]. Available from: https://www.biorxiv.org/content/10.1101/740142v1.
Flemming H-C, Wingender J. The biofilm matrix. Nat Rev Microbiol [Internet]. 2010 Aug2;8(9):623–33. Available from: https://doi.org/10.1038/nrmicro2415
Wingender J, Neu TR, Flemming H-C. What are Bacterial Extracellular Polymeric Substances? In: Wingender J, Neu TR, Fleming H-C, editors. Microbial extracellular polymeric substances: characterization, structure, and function. Berlin: Springer; 1999. p. 1–19.
King RK, Flick GJ, Smith SA, Pierson MD, Boardman GD, Coale CW. Response of Bacterial Biofilms in Recirculating Aquaculture Systems to Various Sanitizers. J Appl Aquac. 2008;20(2):79–92.
Skjermo J, Vadstein O. Techniques for microbial control in the intensive rearing of marine larvae. Aquaculture. 1999;177(1):333–43. 5.
Damiens D, Benedict MQ, Wille M. An Inexpensive and Effective Larval Diet for Anopheles arabiensis (Diptera : Culicidae ): Eat Like a Horse , a Bird , or a Fish? J Med Entomol. 2012;49(5):1001–11.
O’Toole G. Microtiter Dish Biofilm Formation Assay. J Vis Exp. 2011;(47):10–1.
R Core Team. R: A language and environment for statistical computing. Vienna, Austria: R Foundation for Statistical Computing; 2018. https://www.R-project.org/.
Moriarty DJW. The role of microorganisms in aquaculture ponds. Aquaculture. 1997;151(1-4):333-349. doi:10.1016/S0044-8486(96)01487-1

graphicalabstarct.pdf

Download PDF

Journal Publication

published 02 Sep, 2020

Read the published version in Parasites & Vectors →

Editor assigned by journal
01 Jul, 2020
Submission checks completed at journal
30 Jun, 2020
Editor invited by journal
30 Jun, 2020

You are reading this latest preprint version

Measuring and reducing biofilm in mosquito rearing containers

Status:

Journal Publication

Version 2

Abstract

Figures

Background

Methods

Effects of mosquito species, food type and quantity

Estimating Biofilm Abundance

Cleaning method

Food form

Analyses

Results

Discussion

Conclusions

Abbreviations

Declarations

Authors’ contributions

Author details

Acknowledgments

Competing interests

Availability of data and materials

Consent for publication

Ethics approval and consent to participate

Funding

References

Supplementary Files

Status:

Journal Publication

Version 2