Cortisol Measurement in Koala (Phascolarctos cinereus) Fur

Summary

We present a protocol to determine the optimal extraction solvent to measure cortisol from koala fur. The solvents used in this protocol are methanol, ethanol and isopropanol. Determining an optimal extraction solvent will aid in reliably measuring fur to determine the impact of chronic stress on koalas.

Abstract

Optimal methods of hormone extraction used to measure stress in animals across sample types are not always the same. Australia's iconic marsupial species, the koala (Phascolarctos cinereus), faces prolonged exposure to anthropogenic-induced stressors and assessment of chronic stress in wild populations is urgently warranted. One of the most effective ways to measure chronic stress is through analyzing the glucocorticoid hormone cortisol in hair or fur, as it supports physiological and behavioral responses. This laboratory validation study aims to test current techniques to validate an optimal hormone extraction method to be used as a non-invasive measure of cortisol in koala fur. It is recognized that using non-invasive techniques to measure stress hormones is preferred over traditional, invasive techniques due to their ideal practical and ethical standpoints. Additionally, it is comparatively easier to acquire fur from koalas than it is to acquire samples of their blood. This study used samples of koala fur acquired from the Adelaide Koala and Wildlife Hospital to run a number of hormone extraction techniques in an attempt to validate an optimal cortisol extraction method. Results showed that 100% methanol provided the most optimal solvent extraction compared to 100% ethanol or 100% isopropanol based on parallelism results. In conclusion, this method of cortisol extraction from koala fur provided a reliable non-invasive assay that could be used to study chronic stress in koalas.

Introduction

Australian ecosystems sustain human life through the provision of services including food and fiber among many other dynamic interactions¹. Ironically, it is human activity that operates as the dominant driver of ecosystem disruption through biodiversity change². Habitat fragmentation, known as the process of dividing large continuous habitats into small patches of land, isolated from each other, is the major anthropogenic biodiversity change threatening Australian ecosystems². Habitat fragmentation modifies the structure and diversity of species composition in any given area, thus reducing the area of habitat necessary for these species to maintain viable populations². The result of this is increased competition between species for resources including food, fuel, fiber, and water³. The destruction of Australian ecosystems through biodiversity change is having catastrophic consequences on many Australian native species¹.

Australia's most iconic marsupial species, the koala (Phascolarctos cinereus), depends on Australian ecosystems remaining healthy for their survival⁴. The introduction of the European Settlement caused a rapid decline in Australian populations of koalas, as they were slaughtered for their pelts in pursuit of profit in a large export trade⁵. This practice was banned in the 1980's and populations of koalas were then able to stabilize⁵. However, exponential growth of the human population has resulted in this species competing for much of their habitat, and their survival is again under threat⁶. According to the International Union for the Conservation of Nature (IUCN), all populations of Australian koalas are listed as vulnerable to extinction with a decreasing population trend⁷. This listing is attributed to the uncertainty around relevant population parameters and marked variation in population trends for this species⁷. As the most iconic and endemic animals, koalas largely benefit the Australian economy through tourism (NSW Office of Environment and Heritage 2018). An estimation suggests that koala related tourism has generated approximately 9,000 jobs and contributes between $1.1 and $2.5 billion to the economy (NSW Office of Environment and Heritage 2018). The removal of any one species has the potential to be catastrophic, and can be seen in the steady decline of native Australian wildlife⁶. Additionally, the Australia economy will feel the ramifications if populations of Australian koalas continue to decline at the rate they are⁶.

It is suggested that prevalence of death and disease in response to habitat fragmentation is the result of chronic stress⁸. Already, twenty-four marsupial species have been declared extinct in Australia due to habitat fragmentation, with koalas following a similar trend⁸. The complexity of habitat fragmentation and biological systems is synergistic but can be unpacked through analysis of the stress response⁶. Generally, any disturbance in an animals natural surroundings activates a complex cascade of neurohormonal events, known as a 'fight or flight' response^9,10. This response to stress is a process that begins in the brain where the hypothalamic-pituitary-adrenal (HPA) axis is activated¹¹. A component of the brain called the hypothalamus releases corticotrophin-releasing hormone (CRH), which then signals the anterior pituitary to release adrenocorticotrophic hormone (ACTH)¹¹. This in turn stimulates the glucocorticoid secretion from the adrenal medulla. The body circulates glucocorticoids through the blood, which diverts the storage of glucose from glycogen and mobilizes glucose from stored glycogen¹¹. This cascade of neurohormonal events is the response used by the animal to deal with unpredictable stimuli¹¹. However, when glucocorticoids are being released and remain elevated for a prolonged period of time, the animal is considered to be experiencing chronic stress^12,13. This process involves diverting energy away from other corporal bodily functions, as it is needed for ongoing glucocorticoid production¹³. As a result, chronic stress can prohibit growth, reproduction and immunity, all being key fitness traits required for survival¹⁴.

Measuring an animal's glucocorticoid production is a common indicator used to determine whether or not the animal is experiencing physiological stress¹⁵. To do so, glucocorticoids can be measured in blood plasma, serum, saliva, urine or faeces¹⁶. However, evidence suggests that hair is a much more effective indicator of chronic stress, as opposed to the aforementioned¹⁶. This is because hair is thought to incorporate blood-borne hormones during its growth phase; it is relatively stable; and any cortisol detected in hair reflects physiological stress experienced over the period of hair growth, which can be weeks through to months¹⁶. Furthermore, any collection of cortisol should be non-invasive in order to minimise the stress associated with capture and handling¹⁶. However, any stress experienced during this event would not impact glucocorticoid levels in hair¹⁶. There have been many studies that explore the proficiency of using hair to measure long-term stress in a number of animals, and include studies on reindeer, grizzly bears, rhesus monkeys, muskoxen, and brown bears^{17,18,19,20,21}. Hair cortisol is usually extracted by first washing the sample to ensure sweat and sebum-derived cortisol deposited on the surface of the hair is not co-extracted with cortisol and then pulverizing the sample in a bead-beater²². After washing, the sample needs to be dried to ensure complete evaporation²². Finally, using a solvent, the sample can be extracted and reconstituted to facilitate the assay of cortisol²². The most common solvent used to extract cortisol from fur is methanol^21,23; however, there are some studies that use ethanol and isopropanol in their cortisol extraction techniques. For example, a study that used ethanol was successful for extracting cortisol from human amniotic fluid²⁴. Additionally, a study that used isopropanol was successful for extracting cortisol from human hair and nails^25,26. For this reason, this study tested all three solvents (methanol, ethanol, and isopropanol) to determine which was the most successful for extraction of cortisol from samples of koala fur.

The primary objective of this study was to use current techniques to validate an optimal hormone extraction technique to be used as a non-invasive measure of cortisol from koala fur. This was achieved by testing three extraction solvents (methanol, ethanol, and isopropanol). We hypothesized that methanol will be the optimal solvent used for extracting cortisol from koala fur because it is the recommended solvent of extraction by Arbor assay cortisol kits²⁷.     

Protocol

This project was performed under strict animal and human care guidelines. Animal ethics was granted by Western Sydney University (A12373). Additionally, a lab risk assessment and biosafety and radiation form were submitted and accepted by Western Sydney University to safely undertake this research (B12366).

NOTE: Koala fur samples for this project were obtained from the Adelaide Koala and Wildlife Hospital, located at 282 Anzac Highway, Plympton South Australia. Fur was taken from one koala which had been admitted to the hospital and euthanized due to their severe injuries. The deceased koala had been stored in a freezer within a body bag soon after death. After removing the deceased koala from the body bag, 1.2 g of fur was shaved from the nape of the neck using standard animal clippers. The fur was shaved as close as possible to the skin, so as to ensure the skin was not cut. Once shaved, the deceased koala was put back into the body bag and placed in the freezer. The fur was then placed in a pouch made of aluminum foil and stored below -20 °C. In transit, the fur was kept at ambient temperature, and on arrival to the laboratory, the fur was stored at -80 °C.

1. Koala fur cortisol extraction

1. Remove the fur from storage at -80 °C and allow time to thaw.
2. Weigh the fur on a laboratory analytical precision balance.
3. Place 60 mg of the fur into a pre-weighed and labelled 1.5 mL centrifuge tube and repeat until 18 tubes are filled.
   NOTE: 18 fur sub-samples were used for this validation study.
4. Add 1 mL of 100% high-performance liquid chromatography (HPLC) grade isopropanol to each tube using a pipette.
5. Vortex samples for 30 s.
6. Strain each sample using a 0.5 mm micro precision sieve so as to achieve separation of liquid and fur.
7. Discard the liquid into a waste container.
8. Place each fur sample into a labelled plastic weighing boat, then place into a vacuum desiccator, leave the fur to dry for 3 days.
9. Once completely dry, place each sample into a labelled 1.5 mL microcentrifuge tube.
10. Place each sample in a bead mill with 3 chrome steel beads (3.2 mm) and pulverize for 2 min at 30 shakes per second.
11. Pipette 1.5 mL of the first extraction technique (100% analytical grade ethanol) into 6 1.5 mL microcentrifuge tubes containing the fur sample.
12. Perform the same for 100% analytical grade methanol and 100% analytical grade isopropanol until eighteen 1.5 mL microcentrifuge tubes are filled.
13. Cap each 1.5 mL microcentrifuge tube and incubate at room temperature (RT) with constant pulsating using a shaker for 3 h.
14. Remove and strain samples using a 0.5 mm micro precision sieve.
15. Transfer the liquid into a new, labelled 1.5 mL microcentrifuge tube with a pipette while ensuring that the fur is discarded appropriately.
16. Completely dry solvent extract under a stream of N₂ vapor under a fume-cupboard.
17. Reconstitute the dried sample extract using 400 µL of assay buffer (composition provided in the commercial cortisol kit; see Table of Materials) and 100 µL of 100% analytical grade ethanol.
    NOTE: Sample extracts can be stored at -80 .

2. Internal controls

1. To make controls, make a pool of extracted samples with high hormone levels. To make this pool, select samples from animals with known exposure to stressor. For example, select samples from koalas that have been rescued from environmental trauma as they will generally display high cortisol hormone levels⁶.
   1. To make the extract pool, take 20 µL of extract from each sample (n = 10) until a total volume of 200 µL is obtained. The extract pool can be stored at -80 C until assays. Run the pool in each assay as low or high internal controls (see step 2.2).
2. For the assay, use the pool to make stocks for low and high controls that bind at 70% (C1) and 30% (C2), respectively. Obtain the dilution factor for the 30% and 70% binding points from the parallelism graph for the extract against the cortisol standard (Figure 1). Use the assay buffer for dilution of sample pool. For example, use 60 µL of the pool extract and 60 µL of assay buffer for 1:2 dilution.
   NOTE: For the methanol extract, the 30% binding point was at neat while 70% binding point was approximately 1:2 as per Figure 1. Thus, these provided the dilution factor for the internal controls (C1 and C2 respectively) for running within the assay.

3. Cortisol analysis in koala fur extracts

1. Use a commercial cortisol kit (Table of Materials) and set up the 96 well strip plate including the samples, controls, cortisol standards, non-specific binding wells, and maximum binding wells following the supplier’s instructions. Use the plate layout sheet provided in the kit booklet to list the positions of samples, controls, and standards on the plate map.
   NOTE: It is recommended that all samples, controls, and standards are run in duplicate to allow accuracy of results.
2. Prepare samples. Follow the fur hormone extraction (section 1) to obtain 100% methanol extracted koala fur.
3. Prepare reagents. Follow the procedure described in the commercial cortisol kit to prepare the reagents including (1) assay buffer, (2) wash Buffer, and (3) standards (compositions provided in the cortisol kit, Table of Materials).
4. As per the instructions provided in the cortisol kit, pipet 50 µL of samples or standards into wells in the plate. Pipet 75 µL and 50 µL of assay buffer into the non-specific binding (NSB) wells and the maximum binding (B0 or zero standard) wells, respectively.
5. Add 25 µL of the cortisol conjugate to each well using a repeater pipet. Then pipet 25 µL of the cortisol antibody into each well, except the NSB wells. Gently tap the sides of the plate to ensure that the reagents are well mixed.
6. Cover the plate with the plate sealer and shake at room temperature for 1 h (at slow speed) using an orbital shaker.
7. Remove the plate sealer and aspirate the well plate by washing each well with 300 µL of wash buffer 4 times.
8. Dry the plate by tapping the plate on clean absorbent towels.
9. Pipette 100 µL of tetramethylbenzadine (TMB) substrate (composition provided in the cortisol kit, Table of Materials) to each well.
10. Place the plate sealer on the well plate and incubate at RT for 30 min.
11. Pipette 50 µL of stop solution to each well.
12. Place the well plate in a plate reader capable of reading 450 nm.
13. To calculate the final hormone concentration, derive the final fur cortisol concentration in ng/mg of sample by multiplying the pg/mL hormone concentration with the final extract volume (0.5 mL) and dividing by the fur sample mass (60 mg).

Results

Assay detection of hormone metabolites of interest is determined using parallelism. Using a parallelism curve, the 50% binding point also determines the sample dilution factor on the standard curve (Figure 1). As shown in the parallelism graph (Figure 1), the 100% ethanol and 100% Isopropanol extracts did not provide parallel displacement against the cortisol standard. However, the 100% methanol extract provided parallel displacement against the cortisol standard. Dried extracts were run...

Discussion

There are a number of studies that use a range of techniques to detect cortisol in mammalian fur. This study presents results for the detection of cortisol in fur collected from a wild koala exposed to current anthropogenic stress. This ground-breaking study used fur to test which of the three commonly used solvents are best at extracting cortisol, a measure of chronic stress, from koala fur. Results showed that 100% methanol was the recommended solvent for cortisol extraction in this type of mammalian fur.

Materials

Name	Company	Catalog Number	Comments
Centrifuge Tubes	n/a	n/a	1.5 mL
Chrome Steel Beads	n/a	n/a	3.2 mm x 3
Cortisol Kit	Arbor Assays	K003-H1W	Manufactured in Michigan USA
DetectX Cortisol Enzyme Immunoassay Kit	Arbor Assays	K003-H5	Used first-time for cortisol testing in koala fur
Ethanol	n/a	n/a	HPLC Grade
Isopropanol	n/a	n/a	HPLC Grade
Methanol	n/a	n/a	HPLC Grade
Micro Pipette	n/a	n/a	n/a
Micro Precision Sieve	n/a	n/a	0.5 mm
Microplate Reader	Bio Radi	n/a	n/a
Microplate Washer	Bio Radi	n/a	n/a
Orbital Shaker	Bio Line	n/a	n/a
Plastic Weighing Boat	n/a	n/a	n/a
Plate Sealer	n/a	n/a	n/a
Precision Balance	n/a	n/a	n/a
Vortex Mixer	Eppendorf	n/a	n/a