Environmental DNA (eDNA) is the trace genetic material that all animals and plants leave behind in their environment in the form of skin cells, mucous, faeces, etc. For aquatic species, eDNA can be extracted from water samples and screened for the presence of the target species using specific DNA markers. The main advantages of the method are that detection is not dependent on seeing or hearing the animals – greatly reducing sampling costs – and it is able to detect low numbers of individuals (e.g. rare species or early incursions of invasive species). This means that monitoring programs can be conducted rapidly, at lower cost and across a large range of locations, and field sampling can be undertaken by non-specialists including Indigenous rangers and citizen scientists. The goal of this research was to develop and utilise eDNA techniques to improve monitoring of key species in northern Australia.
Fieldwork is expensive and laborious, especially in remote northern Australia. Traditional sampling equipment may be expensive and require expert training to operate or be difficult or impossible to deploy. Our eDNA methods overcome these challenges as they do not require specialised training or equipment and can be conducted rapidly. As a result, sampling can be more frequent and widespread, providing much more data on the occurrence of aquatic plants and animals and leading to more effective management of key threatened or invasive species.
This project had two specific objectives: develop eDNA assays for species of management concern in northern Australia and trial improved field methods for eDNA sampling in remote locations. For the first objective, we selected key exotic species (cane toads, cabomba, spotted tilapia, Mozambique tilapia, snakehead fish, yellow crazy ants) and threatened species (largetooth sawfish, three Elseya turtle species, three rainforest frog species). We refined field sampling methods to make them easier, involving the simple filling of small tubes, containing a DNA preservative, with water. Previous eDNA field protocols involved filtering water through filter papers, which were then preserved in alcohol. This method involves either carrying filtration equipment to sampling sites, or collecting water and keeping it at low temperature before filtering. These procedures are logistically very difficult at remote sites or sites with high sediment loads (which clog filters) and multiple field filtering increases risk of contamination. Additionally, the logistics of keeping water samples cold after collection can limit the ability to preserve eDNA in water. Finally, alcohol can easily evaporate at the high ambient temperatures found in northern Australia and may be prohibited in some communities.
The DNA preservative strategy we developed enables field sampling by simply filling a tube or bottle containing the DNA preservative. We proved that this method was time- and cost-effective, and even more robust than filtering large volumes of water. For example, we were able to detect eDNA from a small remnant population of an endangered rainforest frog 20 km downstream from where they live. In addition, we detected Irwin’s turtle eDNA in the lower Burdekin River, at sites where they had not been seen for >30 years. This field method also increased engagement with Indigenous ranger groups and other non-specialists for sample collection. Given that Indigenous rangers work on their Country year-round, simple and effective field methods allow them to include eDNA sample collection in their usual schedule of activities. The ‘user-friendly’ field methods allowed fieldwork to be undertaken by collaborators in the Torres Strait Islands, north Queensland, the Northern Territory and Western Australia.
Threatened rainforest frogs such as the armoured mistfrog (top) and invasive species including cane toads (bottom) can be detected using eDNA techniques developed during this research. Top photo: Conrad Hoskin. Bottom photo: Northern Australia Environmental Resources Hub.
In the Torres Strait Islands, Indigenous rangers collected samples at permanent waterbodies in key islands that are at risk of cane toad and pest fish incursions. Similarly, three Indigenous ranger groups from Western Australia’s Kimberley region – the Balanggarra Rangers (Adolphus Island), the Nyikina Mangala Rangers (Fitzroy Crossing, mid-west Kimberley) and the Paruku Rangers (Lake Gregory, south-east Kimberley) – collected water samples to screen for cane toads. For threatened species, one Indigenous ranger group (Anindilyakwa Land and Sea Rangers, Groote Eylandt) and one community group (Mimal Land Management, central Arnhem Land) in the Northern Territory collected samples for detection of largetooth sawfish eDNA at areas where there was anecdotal evidence of the species’ presence. In Queensland, Traditional Owners from the Urannah Properties Association aided and participated in sample collection for detection of Irwin’s turtle whose core habitats are under threat from a large dam proposal.
We also engaged with government agencies, such as Biosecurity Queensland, the Queensland Department of Natural Resources, Mines and Energy and the Northern Territory Department of Environment and Natural Resources for eDNA sample collection for detection of tilapia and snakeheads (both pest fish), Irwin’s turtle and the invasive aquatic plant Cabomba caroliniana, respectively. The results of these case studies have assisted managers, Indigenous ranger groups and Traditional Owners to manage these species on their land and in their waterways in northern Australia.
Cooper, M. K., Villacorta-Rath, C., Burrows, D., Jerry, D. R., Carr, L., Barnett, A., Huveneers, C., & Simpfendorfer, C. A. (2021). Practical eDNA sampling methods inferred from particle size distribution and comparison of capture techniques for a Critically Endangered elasmobranch. Environmental DNA, 00, 1– 13. https://doi.org/10.1002/edn3.279
Villacorta-Rath C, Hoskin CJ, Strugnell JM, Burrows D. 2021. Long distance (>20 km) downstream detection of endangered stream frogs suggests an important role for eDNA in surveying for remnant amphibian populations. PeerJ 9:e12013 https://doi.org/10.7717/peerj.12013
The Northern Australia Environmental Resources Hub addressed key research questions to come up with practical, on-ground solutions to some of the north’s most complex environmental challenges. A transdisciplinary research approach has been at the heart of the hub. Integrating key research users – policy-makers and land managers including Traditional Owners and ranger groups – into the co-design of research projects has led to rapid uptake of research outcomes into land management practices and decision-making. The hub has produced this wrap-up video outlining these impacts from the perspectives of research users.
Trujillo-González, A., Villacorta-Rath, C., White, N. E., Furlan, E. M., Sykes, M., Grossel, G., Divi, U., & Gleeson, D. (2021). Considerations for future environmental DNA accreditation and proficiency testing schemes. Environmental DNA. https://doi.org/10.1002/edn3.243
Kwong, S.L.T., Villacorta-Rath, C., Doyle, J. et al. Quantifying shedding and degradation rates of environmental DNA (eDNA) from Pacific crown-of-thorns seastar (Acanthaster cf. solaris). Mar Biol 168, 85 (2021). https://doi.org/10.1007/s00227-021-03896-x
Cooper, M.K., Huerlimann, R, Edmunds, RC, Budd, A.M., Le Port A., Kyne, P.M., Jerry, D.R., Simpfendorfer, C.A. 2021. Improved detection sensitivity using an optimal eDNA preservation and extraction workflow and its application to threatened sawfishes. Aquatic Conserv: Mar Freshw Ecosyst. 2021; 1– 18. https://doi.org/10.1002/aqc.3591
Edmunds R.C., Burrows D. 2020. Got Glycogen?: Development and Multispecies Validation of the Novel Preserve, Precipitate, Lyse, Precipitate, Purify (PPLPP) Workflow for Environmental DNA Extraction from Longmire's Preserved Water Samples. J Biomol Tech. 2020 Dec;31(4):125-150. doi: 10.7171/jbt.20-3104-003. PMID: 33100918; PMCID: PMC7566611.
Villacorta‐Rath, C, Adekunle, AI, Edmunds, RC, Strugnell, JM, Schwarzkopf, L, & Burrows, D. (2020). Can environmental DNA be used to detect first arrivals of the cane toad, Rhinella marina, into novel locations?. Environmental DNA. 2020; 00: 1– 12. https://doi.org/10.1002/edn3.114
Huerlimann, R., Cooper, M.K., Edmunds, R.C., Villacorta‐Rath, C., Le Port, A., Robson, H.L.A., Strugnell, J.M., Burrows, D. and Jerry, D.R. (2020), Enhancing tropical conservation and ecology research with aquatic environmental DNA methods: an introduction for non‐environmental DNA specialists. Anim Conserv. doi:10.1111/acv.12583
The project was led by Professor Damien Burrows from James Cook University (JCU). He was assisted by other researchers at JCU, The University of Western Australia, Charles Darwin University, Griffith University and CSIRO.
Damien Burrows, James Cook University
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