Corpse management of the invasive Argentine ant inhibits growth of pathogenic fungi

Abstract

A dead conspecific poses a potential pathogen risk for social animals. We have discovered that Argentine ants (Linepithema humile) prevent spread of pathogenic fungi from corpses by depositing the dead to combined toilet and refuse areas and applying pygidial gland secretion on them. The presence of a corpse in a nest increases this secretion behaviour. We identified three fungi growing on Argentine ant corpses. Growth of the Argentine ant pathogen Aspergillus nomius and the plant pathogen Fusarium solani on corpses was inhibited as long as the ants were constantly attending them as the ant anal secretion only delayed germination of their spores. In contrast, the effect of the ant anal secretion on the human pathogen Aspergillus fumigatus was much stronger: it prevented spore germination and, accordingly, the fungus no longer grew on the treated corpses. The Argentine ants are one of the world’s worst invasive alien species as they cause ecological and economical damage in their new habitats. Our discovery points at a novel method to limit Argentine ant colonies through their natural fungal pathogens.

Introduction

Social immune system is a term used to describe co-operative behaviour of social animals to reduce vulnerability to disease transmission that arises from living in a genetically homogenous closely interacting group1. For example, management of corpses, faeces, and food waste is part of the social immune system to improve nest hygiene. Corpse-induced behavioural responses in insects include corpse removal from the nest, burial, cannibalism, avoidance, and combinations of these2,3. Undertaking responses depend also on disease and developmental state of the cadaver as well as nesting and feeding habits of the insect4. Corpse management aims to prevent growth and spread of pathogens and parasites: for example, it has been shown in a laboratory experiment that a single fungal infected cadaver can be fatal to the whole ant colony5. In some highly socially organised insects corpse management has been suggested to be separate from the other basic cleaning activities, such as disposing faeces and food remains. For example, some ant species remove corpses from nest more quickly and farther away than other objects6,7, foreign corpses are treated differently to nestmates’ corpses8, and faeces and corpses are deposited into separate areas9.

The Argentine ant is listed in the International Union for Conservation of Nature’s 100 world’s worst invasive alien species, because it has spread from South America to all over the world during the past 160 years and is able to harm ecosystems by displacing native species10,11,12. The success of the invasive Argentine ants has been attributed mostly to their lack of territoriality as the ants mix freely between nests and can hence form extensive supercolonies spanning thousands of kilometers13,14. Whereas introduced Argentine ants from two different continents may show no hostility15, the native South American Argentine ants that form much smaller16 and short-lived17 colonies display aggression among colonies18. The unicolonial social structure enables high population densities19, which together with low genetic diversity20 and relative few immune genes21 may predispose the invasive Argentine ants to pathogens. Thus, hygiene behaviour is expected to be especially important for their survival.

Argentine ants deposit food waste and dead bodies onto refuse piles22 yet their defecating behaviour has not been studied. We discovered that Argentine ants defecate and secrete pygidial gland content onto the corpses at the refuse piles and that this behaviour inhibits growth of pathogenic fungi.

Results

The Argentine ants deposit corpses and faeces on the same area

We plated 20 ants to plaster-bottom petri dishes and fed them with blue-coloured sugar mix. After four days we measured the sizes of the blue stained areas they left on the plaster. We repeated the experiment 20 times. The ants had clearly a preferred toilet area at the periphery of the plate as indicated by the large blue stained areas (1–2 toilets per plate, size >0.001 stained/whole area, that is, the proportion of stained area from the whole surface are of the plate), although several tiny patches were also visible (total number of blue patches per plate: mean = 9, SD = 8.6) (Fig. 1a).

Figure 1
figure1

The Argentine ants have combined toilet and refuse pile areas. (a) Argentine ants defecate on dedicated toilet areas. Worker ants were plated on plaster-bottom petri dishes (N = 20) and they were given blue-coloured sugar solution for food. Plates were photographed four days after and the area of each blue patch was measured and blotted for each plate (colony). The false-colour image of a presentative plate shows toilet area in red. (b) The Argentine ants deposit corpses on the toilet areas. Ants were plated on plaster-bottom petri dishes (N = 20) and were given blue-coloured sugar solution for food and the next day one ant was killed and the corpse was immediately placed back to the middle of the nest plate. Three days later the plates were photographed and the stained areas were measured and the location of the corpse was recorded and blotted for each plate (colony). In a blot the yellow circles denote toilet patches and red circles are toilet patches with a corpse in them. In colonies #10, 11, 12, 16, and 20 the corpse was chopped into two pieces and deposited into two different toilet areas. In colony #7 the corpse was outside of toilet areas and it is marked with red circle at zero area. In the presentative false-colour image, the toilet areas are in red and a white arrow indicates the location of the corpse. (c) The presence of a corpse in a nest induces anal secretion. Total area of all the blue patches were calculated for each nest without (yellow, CTRL) and with a corpse (red, CORPSE). (d) Large blue patches (>0.001 stained/whole area) with a corpse (red, N = 22) were significantly larger than patches without a corpse (yellow, N = 33). In the box plots, the black line represents median value, values inside the box cover first and third quartile (interquartile) range, the whisker show values up to 1.5 times the interquartile range, and grey circles are individual values beyond the whisker range (outliers).

As it was earlier shown that black garden ants (Lasius niger) have separate toilet area and waste pile to where the corpses were laid9, we studied next where Argentine ants put their dead. We modified the previous experiment by killing one of the ants a day after plating them, placing it immediately back to middle of the plate, and recording its location three days later. The experiment was repeated 20 times. We found that the corpses were in the large (>0.001 stained/whole area, 1–2 per plate) toilet areas and not at random locations (Fisher exact test p-value < 0,00001) (Fig. 1b). We saw the same effect with ants fed with fluorescence dye sugar mix instead of blue dye (see Supplementary Fig. 1).

When the ants were given a corpse they produced larger total area of blue patches than when there was no corpse in a plate (N = 40, Mann-Whitney U = 99, p = 0.006, Fig. 1c). However, when only the larger blue areas were considered (>0.001 stained/whole area, N = 55), there was no difference in their sizes between the colonies that were given a corpse (Fig. 1a) or not (Fig. 1b) (Mann-Whitney U = 326, p = 0.408). Yet the large blue patches with a corpse (N = 22) were significantly larger than patches without a corpse (N = 33) (Mann-Whitney U = 515, P = 0.009, Fig. 1d). These results suggest that in the presence of a corpse, ants increase defecation and/or secretion of anal gland products, specifically to the area where the corpse is (see Supplementary video 5 and Supplementary videos 1–4 for prior corpse processing behaviour).

Placing corpses to toilets inhibits fungal growth on them

We noticed that when the ants are starving (were given only water) or fed with neonicotinoid neurotoxin (Imidacloprid) they did not pile or process the corpses and these unmanaged corpses started to grow fungi in a few days (see Supplementary Fig. 2). These observations indicated that fungal growth is inhibited from the corpses placed at the toilet areas. To test this idea we plated 22 ants on plaster-bottom petri dishes and a day after we killed two of them: the first corpse was placed to an empty new plate and the second corpse was put back to the nest plate. The corpse in the nest plate was kept with the living ants for six days after which the ants were removed. We recorded how many days after the ants were killed would fungus visibly grow on the corpses. The experiment was repeated 40 times. When a corpse was alone it started to grow fungus, on average, three days after death, whereas corpses in the nests did not grow fungi as long as there were living ants present (Fig. 2a). When the ants were removed, the corpses in the nests started to grow fungus in one day even if the corpses were in the toilet areas. Inhibition of fungal growth on corpses in the nests and alone was significantly different (inhibition shown with survival analysis with number of days until fungal growth from the corpses: Cox’s proportional hazard model, hazard ratio HR = 0.40, p = 0.002, see Supplementary Fig. 3). The overall percentage of fungi growing corpses remained somewhat lower in the nests (47.5%) than in the empty plates (57.5%), yet the difference is not statistically significant (Chi2 with Yates correction = 0.4511, p-value = 0.5018).

Figure 2
figure2

The Argentine ant anal secretion inhibits mould growth. (a) Worker ants were plated on plaster-bottom petri dishes (N = 40 plates) and were given sugar solution for food. The next day two of the ants were killed and the first corpse was put on an empty plaster-bottom petri dish and the second back to the nest plate. After six days, ants were removed from the nest plate (red arrow) and the appearance of visible fungal growth was recorded for six more days. The blot shows the percentage of corpses visibly growing fungi for lone corpses (black, Alone) and corpses in the nests (yellow, Nest). (b) F. solani, A. nomius, and A. fumigatus were identified from the corpses. The bars show how many corpses were visibly growing each fungus in lone (black, at six days) or nest (yellow, at 12 days) conditions. Effect of the isolated Argentine ant gaster-liquid on spore germination was measured for (c) F. solani, (d) A. nomius, and (e) A. fumigatus. Gaster-liguid was collected from ants that had two corpses (red) or none (yellow) in a nest. Spores were plated on nutrient agar plates and 1 µl of gaster-liquid, 10% sugar solution (green), or fungicide Amphotericin B (black) was added to three spots on a plate and percentages of germinated spores were recorded every hour for 12 hours. Grey dashed lines indicate the time points for statistical analysis. The experiment was repeated three times (N = 9, variation is ± SE). (f) Gaster-liquid prevented germination of A. fumigatus spores and after 24 hours no-growth zones (mm of diameter) were measured for the gaster-liguid (corpse: red bar, no-corpse: yellow bar), 10 % sugar, and Amphotericin B (black bar) treated spots (N = 9, variation is ± SE). (g) Pygidial gland but not gut-derived secretion inhibited A. fumigatus growth. Gut and pygidial gland content were collected separately and used in A. fumigatus spore germination test. No-growth zone was measured 24 hours after the application of the samples. The experiment was repeated three times using two different isolations (N = 6, variation is ± SE). (h) Gut secretion liquid had twice as much of food-derived fluorescein than pygidial gland secretion. Three separate isolations from 10 ants were measured (N = 3, variation is ± SE).

Fungal identification

The corpses were growing three visibly different fungi, which were identified by internal transcribed spacer (ITS) sequencing to be Aspergillus nomius (yellow conidia, Fig. 3a), Aspergillus fumigatus (blue conidia, Fig. 3b), and Fusarium solani (completely white appearance, Fig. 3c). Interestingly, frequencies of the three fungi growing on corpses were dependent on whether the corpses were alone or in the nest (Fig. 2b, Freeman-Halton Fisher exact test p-value = 0.003152). The corpses treated with anal secretion by their nestmates never grew A. fumigatus but still readily grew A. nomius and F. solani, whereas all three fungi grew in corpses that were alone.

Figure 3
figure3

A. nomius is an Argentine ant pathogen. Presentative photographs of Argentine ant corpses growing (a) A. nomius, (b) A. fumigatus, and (c) F. solani. Effect of A. nomius spores on ant survival was tested by applying spores onto the ant thorax. (d) Survival of infected (A. nomius, N = 30) and control (CTRL, N = 30) ants were recorded for 14 days. Difference in survival between the treatments was calculated using the Cox’s proportional hazard model. The corpses were surface sterilized the day they died and visible appearance of fungal growth on corpses was recorded for at least 7 days. (e) All A. nomius infected (N = 22) corpses grew A. nomius whereas over half of the control corpses (N = 9) grew no fungus at all.

Argentine ant pygidial gland secretion inhibits fungal spore germination

To tests whether Argentine ant anal secretion inhibits fungal spore germination, we collected gut and gland contents by gently squeezing the ant’s gaster. Because in the previous experiment we saw that the presence of a corpse increased the secretion behaviour, we isolated gaster-liquids from ants that either had no corpse or had two corpses in the nest. We used fungicide Amphotericin B as a negative and 10% sucrose solution and no-treatment as positive controls. We plated F. solani, A. nomius, and A. fumigatus spores onto nutrient agar plates and added 1 µl of the gaster-liquid samples and controls to the plates. We were not able to use the common disc diffusion assay as the amount of liquid extracted from the ants was not sufficient. Percentage of germinated spores was recorded for each fungus every hour until the germination percentage at the control samples reached plateau (Fig. 2c–e). We repeated the experiment three times and had triplicates of each treatment (gaster-liquids and controls) on each plate. Additionally, the area of inhibition was measured for A. fumigatus samples 24 hours post-plating (Fig. 2f). The gaster-liquid delayed the start of the germination of F. solani and A. nomius spores by about two hours. As the germination rate of spores treated with gaster-liquid collected from ants housed with or without corpses was similar, these samples were combined as the “gaster-liquid” treatment. This also suggests that the production of the effective substance in the gaster-liguid is not induced by the presence of a corpse. Additionally, the two positive controls (sugar and no-treatment) were combined for the analysis (Fig. 2c,d, see Supplementary Table 1). Spore germination rates of these two groups were compared at the time point when the positive control samples had reached a plateau. For F. solani, spore germination percentage was significantly lower for the spores treated with gaster-liquid (7 hours post-plating, p < 0.001, 24% and 91% for gaster-liquid and control, respectively). Similarly, for A. nomius, spore germination percentage was lower  for the gaster-liquid treated spores (8 hours post-plating, p < 0.001, 34% and 88% for gaster-liquid and control, respectively) (Table 1). The germination of A. fumigatus was completely inhibited by the gaster-liquid since we detected no germinated spores during the 8 hour observation period when about 70% of spores had germinated in the controls (Fig. 2e). After 24 hours we saw a no-growth zone where the gaster-liguid was applied indicating that the effect was permanent (Fig. 2f). On average, 250 ng of Amphotericin B produced 10 mm and gaster-liquid 2.7 mm diameter no-growth zone.

Table 1 GLM results showing the effect of gaster-liquid treatment (in comparison to control samples) on the spore germination of F. solani and A. nomius.

Since the collected gaster-liquid consist mainly of the content of rectum and the pygidial gland, we decided to collect the two secretions separately and test them against A. fumigatus spores using a growth inhibition test (Fig. 2g). We used the same controls as above: sugar and Amphotericin B. Gut liquids did not inhibit fungal spore germination at all (no-growth zone of 0 mm) whereas pygidial gland content produced similar effect with original gaster-liquid (no-growth zone of 3.1 mm).

Since pygidial gland secretion, not gut liquids (i.e., faeces), inhibited the fungal germination, we examined the distribution of food-derived fluorescence dye into gut and pygidial gland in order to see whether increase in application of pygidial gland secretion could contribute to plaster staining in the behavioral experiment (Fig. 1c,d). Although significantly more fluorescein was in the gut secretion than in pygidial gland (student’s t-test p-value = 0.0137), the amount was only 2.5 times higher and thus also the pygidial gland secretion would be visible in dye feeding experiments and would contribute  to the size of the stained areas.

A. nomius kills Argentine ants

We tested by trial experiments the sensitivity of the ants to the three fungi we identified (see Supplementary Fig. 4). Because the preliminary results suggested that A. nomius was the most effective in killing the ants, we tested its effect on the ant survival by topical application of A. nomius spores (Fig. 3d). We used 0.1% tween as a control treatment. We followed survival of the ants in individual plates for 14 days. A. nomius treatment increased mortality significantly in comparison to control treatment (lowered survival probability shown with Cox’s proportional hazard model, N = 60, HR = 3.541, 95% Cl for HR 1.618–7.747, z = 3.165, and p = 0.00155). We surface sterilised the corpses on the day of their death and over half of the control corpses did not grow fungus during the seven day observation period (Fig. 3e). However, all the A. nomius infected corpses showed A. nomius growth, on average, in 1.36 days suggesting that their death was due to A. nomius infection.

Discussion

Argentine ants start carrying dead nestmates to refuse piles when cuticular “life-associated” chemicals, dolichodial and iridomyrmecin, have disappeared22. These volatiles are secreted from pygidial gland and Argentine ants use them also as defensive compounds23 and trail pheromones24. Argentine ants have four distinct anal endocrine glands: Pavan’s, Dufour’s, venom, and pygidial gland25, from which the pygidial gland is the largest25. Iridomyrmecin is major product of pygidial gland23 and it has been shown to be weakly antibacterial26. Beetle pygidial gland secretion has been described to inhibit fungal growth27,28,29. However, fungicidal properties of ant pygidial gland chemicals have not been reported before.

Ants generally inhibit fungal and bacterial growth on their surface by self- and allo-grooming30,31, metapleural32 and poison gland secretion33, and symbiotic bacteria34,35. Interestingly, Argentine ants, unlike many other ant species, were found to lack antibacterial substances on their surfaces36. Moreover, Linephitema melleum, a congener of Argentine ant, has been shown to spread antibiotic metapleural secretion only on themselves and not on nestmates, brood, or queens as some other ant species do37. Thus, if Argentine ants have to rely on grooming to keep bacteria and fungal spores away, then contamination risk from corpses is high. Furthermore, since Argentine ants are predators38,39 they bring other insect species into the nest, which is an additional source of pathogenic fungi. Hence, as the Argentine ant pygidial gland secretion has anti-fungal properties, combining the refuse pile and toilet area provides simultaneous sanitation of food waste, corpses, and faeces. Other corpse and waste management associated processes, such as, chopping up the corpses, eating them, and collecting other nest materials on the refuse piles will also inhibit fungal growth3,40,41.

In nature ants have refuse piles inside or/and outside the nest and some species have dedicated workers to manage the waste42,43,44. Eurhopalothrix heliscata (Myrmicinae) builds a waste chamber inside the nest, yet in an artificial nest they deposit waste on a corner of a foraging area45 like Argentine ants22. The red ants (Myrmica rubra) dispose corpses outside the nest but when they are placed into confined artificial nest they scatter corpses around the area2. Thus, although our experimental set-up was artificial, the results will likely reflect ants’ natural behaviour.

We identified three fungi growing from the dead Argentine ants: F. solani belongs to a species complex best known as plant pathogens46, A. nomius is an aflatoxin-producing entomopathogen47,48,49,50, and A. fumigatus is one of the most common pathogenic fungus in immune compromised humans51. All these opportunistic fungi are widespread in nature and especially Aspergillus spp. are commonly associated with social insects and their nests52,53,54,55. According to our results, A. fumigatus was the most sensitive to the effects of Argentine ant pygidial gland secretion as the gland secretion prevented the spore germination and the fungus never grew on the bodies at the refuse piles. The inhibitory effect of the pygidial gland secretion on Argentine ant pathogen A. nomius and plant pathogen F. solani was transient both in vivo and in vitro assays. Hence, inhibiting the growth of A. nomius and F. solani requires constant application of pygidial gland secretion on the corpses. Consistently, the presence of a corpse increased stained areas especially at the toilet/refuse piles where the corpse was, suggesting that corpse may have induced pygidial gland secretion behaviour. We cannot separate in our experiments faeces and pygidial gland-derived staining, since the food-derived dye was able to cross to pygidial gland content as well. However, as pygidial gland secretion has been shown to attract nestmates as a trail pheromone24 and defence substance23, its application on corpses could create virtuous cycle, whereby more ants gather to the site, which leads to increased pygidial gland secretion and thus more efficient fungal growth inhibition.

Argentine ants are notoriously difficult to eradicate due to their non-territoriality, large colony sizes, and existence of several queens per nest56. Our results suggest that Argentine ants secrete pygidial gland chemicals on toilet/refuse piles to inhibit growth of pathogenic fungi on corpses and other waste. If this behaviour is crucial for nest hygiene, it might open a mechanism to lower the population fitness of this destructive invasive pest by neutralising the anti-fungal component(s) of the pygidial gland secretion.

Methods

Ants

The Argentine ants were collected in April 2011 from the European Main supercolony in Catalonia, Spain57. The ants were kept in artificial nest in Sanyo climate chambers set to 14 hours of light in 27 °C and 10 hours of dark in 20 °C, and air moisture between 40–60%. Ants had water all the time and were fed two times per week with honey and cockroaches. For experiments ants were removed from the artificial nest to wetted plaster-bottom 9 cm diameter petri dishes and they were given (50 µl) 10% sucrose solution or 2.5% blue food colouring (Brilliant Blue FCF, Dr. Oetker) in 10% sucrose solution.

Behavioural experiments

For toilet localisation experiment, ants were removed after four days of plating and plates were photographed. For corpse management experiment, one of the ants was killed by squeezing with forceps one day after plating and placed immediately back to the middle of the nest plate. Three days after the plate was photographed. The Fisher exact test compared the observed (19 bodies in large toilets, 0 in small patches, and 1 outside toilets) and expected values based on probabilities of corpse being randomly either in or outside of a toilet area. The experiment was repeated 20 times.

For fungus growing experiment 22 ants were plated and a day after plating two ants were tweezed to death, one was placed directly to a new wetted plaster-bottom petri dish, and the other corpse was placed back to middle of the nest plate. After six days, ants were removed from the nest plate. Fungal growth on bodies was inspected for 12 days (time until fungal growth was used in the survival analysis testing for the inhibitory effect of ant gaster-liquids, see Fig. 3 in Supplemental material). The experiment was repeated 40 times.

Fungi

Fungi were isolated from ant corpses and subcultured on potato dextrose agarose (PDA) plates. Axenic cultures of each species were used for the experiments and species-level identification. Fungal cultures were maintained at the same conditions as the ants. Spores were collected by submerging fungus growing on a PDA plate into 10 ml of sterile distilled water containing 0.1% Tween-20 (v/v) to release the spores. The spore suspensions were filtered through one layer of Miracloth (EMD Millipore, cat. no. 475855, pore size of 22–25 µm). For the experiments, freshly-collected spore suspensions were counted and adjusted for specific spore concentration (1 × 106–2 × 107 spores/ml). Suspensions were stored at 4 °C and used in the experiments during the same day.

Identification of ant associated fungi

Fungal samples were collected into 15 µl of sterile water, boiled for 5 min, and then used as a template for PCR. To identify the fungi, region of the fungal rRNA gene repeat, Internal Transcribed Spacer (ITS2), was amplified using fungal specific primers fITS758 and ITS459. PCR was performed in 20 µl final volume, containing 1X Phusion HF Buffer, 200 µM of dNTPs, 0.5 µM of both primers, and 0.02U/µl of Phusion high-fidelity DNA polymerase (ThermoFisher). The following PCR protocol was used: 98 °C for 3 min, followed by 35 cycles of 98 °C for 10 s, 57 °C for 15 s, and 72 °C for 30 s, with a final elongation of 72 °C for 7 min. For each of the three fungal species, two representative samples were sequenced: one collected directly from a dead ant’s surface, and another from an axenic subculture from PDA plates. PCR products were sequenced with fITS7 and ITS4 primers at Eurofins. The fungi were identified by Blastn search of the National Center for Biotechnology Information database.

Spore germination assay

Spores were counted and diluted into 1 × 107/ml for F. solani, 2 × 107/ml for A. nomius, and 3.5 × 107/ml for A. fumigatus. Spore solutions (100 µl) were plated on nutrient broth agar plates (Scienova) and incubated at 30 °C for either two or four hours before test solutions were added (due to different germination speeds of the fungi). On each fungal spore plate, 1 µl of the gaster-dilutions, Amphotericin B (250 µg/ml), or 10% sucrose solution was applied to three separate spots (i.e., three replicates). Spore germination, i.e., existence of visible germ tube, was recorded every hour for the next 8 hours, each time examining 100 spores under light microscope. 24 hours from the plating the diameter of no-growth zone was measured for A. fumigatus plates. Experiments were repeated three times.

The effect of the treatment (gaster-liquid or positive control) on the spore germination percentage was tested using Generalized Linear Model (GLM, with Gaussian distribution) using R, controlling for the variation among plates with using the plate information as a factor in the analysis. The gaster-liquid treatment comprised of samples from ants of nest plates with or without a corpse present, and positive controls were combined samples of sucrose treatment and control without any treatment. Spore germination was compared at the time point when the positive control samples had reached a plateau, i.e. 7 and 9 hours after the plating the spores for F. solani and A. nomius, respectively.

Anal-liquid collection

A day before the collection 50 ants were plated per plaster plate with 10% sucrose solution for feed. In half of the nests two ants were killed and placed to the nest two to six hours before the liquid collection. Liquid was collected from ants by squeezing their gaster into drop (2 µl) of sterile water. Gaster-liquid from about 200 ants (in total about 2 µl) was collected into a 20 µl of water and frozen at −20 °C until use. We standardised the amount of gaster-liquid collected at separate times by measuring absorbance at wavelength of 275 nm.

To collect gut and pygidial gland contents separately, ant gaster was squeezed and when gut (ventral opening) and/or pygidial gland (dorsal opening) secretion droplets were visibly separable under microscope they were collected to separate drops (1 µl) of sterile water by touching the surface of the water drop with the secretion droplet. Argentine ant gaster has been shown to contain several gland openings ventrally (i.e., Pavan’s, Dufour’s, and venom)25 and thus we cannot rule out contents from these glands in the gut fraction.

Fluorescein distribution measurements

Ants were plated on plaster-bottom petri dishes and given 10 µg/ml fluorescein (Fluka) in 10% sucrose solution to feed. After two days gut and pygidial gland secretions were squeezed from 10 ants and diluted into 50 µl of water. Isolation was repeated three times. Fluorescein concentration in the samples were measured with plate reader (485 nm excitation/520 nm emission, Victor PerkinElmer) and the amount of fluorescein was calculated from linear standard curve.

Ant survival experiments

Effect of exposure to A. nomius spores on ant survival by surface application was studied by pipetting a 1 µl drop of either 1.6 × 107/ml A. nomius spores or 0.1% Tween-20 onto the ant thorax. A day before the experiment, 60 ants were plated onto their own plaster-bottom petri dishes with 50 µl of 10% sucrose solution. 30 ants were treated with the spore solution and 30 ants with the control solution. Survival of the ants were recorded for 14 days and each day the dead were removed from the nest plate, surface sterilized60, and fungal growth from the corpses was recorded until the end of the experiment or at least 7 days.

Differences in the survival of ants (days until death) treated with A. nomius spore solution and control solution was analyzed using survival analysis (the Cox’s proportional hazard model: surviving individuals were included in the analysis, but scored as separate from the dead ants), with the R package Survival61 (treatment was coded as 1 = ctrl and 2 = A. nomius spores).

Pictures and videos

Pictures were taken with Nikon D3300 camera with AF-P Nikkor 18–55 mm objective or with Olympus OMD EM1 camera with M. Zuiko Digital ED 60 mm f2.8 macro objective. Picture and video analysis and processing were done with Olympus viewer software, iMovie, ImageJ (Fiji), and Corel PaintShopt Pro X9.

Statistical analysis

Statistical analysis was done with R v.3.5.0 and IBM SPSS Statistics 24.

Data Availability

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

References

  1. 1.

    Cremer, S., Armitage, S. A. O. & Schmid-Hempel, P. Social Immunity. Current Biology 17, R693–R702 (2007).

  2. 2.

    Diez, L., Lejeune, P. & Detrain, C. Keep the nest clean: Survival advantages of corpse removal in ants. Biol. Lett. 10, 20140306 (2014).

  3. 3.

    Sun, Q. & Zhou, X. Corpse management in social insects. International Journal of Biological Sciences 9, 313–321 (2013).

  4. 4.

    Sun, Q., Haynes, K. F. & Zhou, X. Managing the risks and rewards of death in eusocial insects. Philosophical Transactions of the Royal Society B: Biological Sciences 373, 20170258 (2018).

  5. 5.

    Loreto, R. G. & Hughes, D. P. Disease in the society: Infectious cadavers result in collapse of ant sub-colonies. PLoS One 11, e0160820 (2016).

  6. 6.

    Skidmore, B. A. & Heithaus, E. R. Lipid cues for seed-carrying by ants in Hepatica americana. J. Chem. Ecol. 14, 2185–2196 (1988).

  7. 7.

    Wilson, E. O., Durlach, N. I. & Roth, L. M. Chemical Releaser of Necrophoric Behavior in Ants. Psyche (New York) 65, 108–114 (1958).

  8. 8.

    Maák, I. et al. Cues or meaningless objects? Differential responses of the ant Formica cinerea to corpses of competitors and enslavers. Anim. Behav. 91, 53–59 (2014).

  9. 9.

    Czaczkes, T. J., Heinze, J. & Ruther, J. Nest etiquette-where ants go when nature calls. PLoS One 10, e0118376 (2015).

  10. 10.

    Suarez, A. V. & Tsutsui, N. D. The evolutionary consequences of biological invasions. Molecular Ecology 17, 351–360 (2008).

  11. 11.

    Wetterer, J. K., Wild, A. L., Suarez, A. V., Roura-Pascual, N. & Espadaler, X. Worldwide spread of the Argentine ant, Linepithema humile (Hymenoptera: Formicidae). Myrmecological News 12, 187–194 (2009).

  12. 12.

    Lowe, S., Browne, M., Boudjelas, S. & De Poorter, M. 100 of the world’s worst invasive alien species. A selection from the Global Invasive Species Database. Invasive Species Spec. Gr. a Spec. Gr. Species Surviv. Comm. World Conserv. Union 12 (2000).

  13. 13.

    Chapman, R. E. & Bourke, A. F. G. The influence of sociality on the conservation biology of social insects. Ecol. Lett. 4, 650–662 (2001).

  14. 14.

    Giraud, T., Pedersen, J. S. & Keller, L. Evolution of supercolonies: The Argentine ants of southern. Europe. Proc. Natl. Acad. Sci. 99, 6075–6079 (2002).

  15. 15.

    Van Wilgenburg, E., Torres, C. W. & Tsutsui, N. D. The global expansion of a single ant supercolony. Evol. Appl. 3, 136–143 (2010).

  16. 16.

    Suarez, A. V., Tsutsui, N. D., Holway, D. A. & Case, T. J. Behavioral and genetic differentiation between native and introduced populations of the Argentine ant. Biol. Invasions 1, 43–53 (1999).

  17. 17.

    Vogel, V., Pedersen, J. S., D’Ettorre, P., Lehmann, L. & Keller, L. Dynamics and genetic structure of argentine ant supercolonies in their native range. Evolution (N. Y). 63, 1627–1639 (2009).

  18. 18.

    Tsutsui, N. D. & Case, T. J. Population genetics and colony structure of the Argentine ant (Linepithema humile) in its native and introduced ranges. Evolution 55, 976–85 (2001).

  19. 19.

    Holway, D. A., Lach, L., Suarez, A. V., Tsutsui, N. D. & Case, T. J. The Causes and Consequences of Ant Invasions. Annu. Rev. Ecol. Syst. 33, 181–233 (2002).

  20. 20.

    Tsutsui, N. D., Suarez, A. V., Holway, D. A. & Case, T. J. Reduced genetic variation and the success of an invasive species. Proc. Natl. Acad. Sci. 97, 5948–5953 (2000).

  21. 21.

    Smith, C. D. et al. Draft genome of the globally widespread and invasive Argentine ant (Linepithema humile). Proc. Natl. Acad. Sci. 108, 5673–5678 (2011).

  22. 22.

    Choe, D.-H., Millar, J. G. & Rust, M. K. Chemical signals associated with life inhibit necrophoresis in Argentine ants. Proc. Natl. Acad. Sci. 106, 8251–8255 (2009).

  23. 23.

    Welzel, K. F., Lee, S. H., Dossey, A. T., Chauhan, K. R. & Choe, D. H. Verification of Argentine ant defensive compounds and their behavioral effects on heterospecific competitors and conspecific nestmates. Sci. Rep. 8, 1477 (2018).

  24. 24.

    Choe, D. H., Villafuerte, D. B. & Tsutsui, N. D. Trail Pheromone of the Argentine Ant, Linepithema humile (Mayr) (Hymenoptera: Formicidae). PLoS One 7, e45016 (2012).

  25. 25.

    Billen, J. Morphology and ultrastructure of the abdominal glands in Dolichoderine ants (Hymenoptera, Formicidae). Insectes Soc. 33, 278–295 (1986).

  26. 26.

    Pavan, M. & Nascimbene, A. Studi sugli antibiotici di origine animale. I. Su un principio antibiotico di Iridomyrmex pruinosus humilis Mayr. (nota prev.). Boll. Soc. Med. Chir. Pavia 62, 193–197 (1948).

  27. 27.

    Nenadić, M. et al. Antifungal activity of the pygidial gland secretion of Laemostenus punctatus (Coleoptera: Carabidae) against cave-dwelling micromycetes. Naturwissenschaften 104, 52 (2017).

  28. 28.

    Nenadić, M. et al. The pygidial gland secretion of the forest caterpillar hunter, Calosoma (Calosoma) sycophanta: the antimicrobial properties against human pathogens. Applied Microbiology and Biotechnology 101, 977–985 (2017).

  29. 29.

    Nenadić, M. et al. Antimicrobial activity of the pygidial gland secretion of three ground beetle species (Insecta: Coleoptera: Carabidae). Naturwissenschaften 103, 34 (2016).

  30. 30.

    Reber, A., Purcell, J., Buechel, S. D., Buri, P. & Chapuisat, M. The expression and impact of antifungal grooming in ants. J. Evol. Biol. 24, 954–964 (2011).

  31. 31.

    Theis, F. J., Ugelvig, L. V., Marr, C. & Cremer, S. Opposing effects of allogrooming on disease transmission in ant societies. Philos. Trans. R. Soc. B Biol. Sci. 370, 20140108 (2015).

  32. 32.

    Yek, S. H. & Mueller, U. G. The metapleural gland of ants. Biol. Rev. 86, 774–791 (2011).

  33. 33.

    Tragust, S. et al. Ants disinfect fungus-exposed brood by oral uptake and spread of their poison. Curr. Biol. 23, 76–82 (2013).

  34. 34.

    Heine, D. et al. Chemical warfare between leafcutter ant symbionts and a co-evolved pathogen. Nat. Commun. 9, 2208 (2018).

  35. 35.

    Dhodary, B., Schilg, M., Wirth, R. & Spiteller, D. Secondary Metabolites from Escovopsis weberi and Their Role in Attacking the Garden Fungus of Leaf-Cutting Ants. Chem. - A Eur. J. 24, 4445–4452 (2018).

  36. 36.

    Penick, C. A. et al. External immunity in ant societies: Sociality and colony size do not predict investment in antimicrobials. R. Soc. Open Sci. 5, 171332 (2018).

  37. 37.

    Fernández-Marín, H., Zimmerman, J. K., Rehner, S. A. & Wcislo, W. T. Active use of the metapleural glands by ants in controlling fungal infection. Proc. R. Soc. B Biol. Sci. 273, 1689–1695 (2006).

  38. 38.

    Tillberg, C. V., Holway, D. A., LeBrun, E. G. & Suarez, A. V. Trophic ecology of invasive Argentine ants in their native and introduced ranges. Proc. Natl. Acad. Sci. 104, 20856–20861 (2007).

  39. 39.

    Abril, S., Oliveras, J. & Gómez, C. Foraging activity and dietary spectrum of the Argentine ant (Hymenoptera: Formicidae) in invaded natural areas of the northeast Iberian Peninsula. Environ. Entomol. 36, 1166–1173 (2007).

  40. 40.

    Renucci, M., Tirard, A. & Provost, E. Complex undertaking behavior in Temnothorax lichtensteini ant colonies: From corpse-burying behavior to necrophoric behavior. Insectes Soc. 58, 9–16 (2011).

  41. 41.

    Tragust, S. et al. Ants disinfect fungus-exposed brood by oral uptake and spread of their poison. Curr. Biol. 23, 76–82 (2013).

  42. 42.

    Peeters, C., Hölldobler, B., Moffett, M. & Ali, T. M. M. ‘Wall-papering’ and elaborate nest architecture in the ponerine ant Harpegnathos saltator. Insectes Soc. 41, 211–218 (1994).

  43. 43.

    Hart, A. G. & Ratnieks, F. L. W. Task partitioning, division of labour and nest compartmentalisation collectively isolate hazardous waste in the leafcutting ant Atta cephalotes. Behav. Ecol. Sociobiol. 49, 387–392 (2001).

  44. 44.

    Hart, A. G. & Ratnieks, F. L. W. Waste management in the leaf-cutting ant Atta colombica. Behav. Ecol. 13, 224–231 (2002).

  45. 45.

    Wilson, E. O. & Brown, W. L. Behavior of the cryptobiotic predaceous ant Eurhopalothrix heliscata, n. sp. (Hymenoptera: Formicidae: Basicerotini). Insectes Soc. 31, 408–428 (1984).

  46. 46.

    Coleman, J. J. The Fusarium solani species complex: Ubiquitous pathogens of agricultural importance. Mol. Plant Pathol. 17, 146–158 (2016).

  47. 47.

    Kurtzman, C. P., Horn, B. W. & Hesseltine, C. W. Aspergillus nomius, a new aflatoxin-producing species related to Aspergillus flavus and Aspergillus tamarii. Antonie Van Leeuwenhoek 53, 147–158 (1987).

  48. 48.

    Chouvenc, T., Su, N. Y. & Elliott, M. I. Antifungal activity of the termite alkaloid norharmane against the mycelial growth of Metarhizium anisopliae and Aspergillus nomius. J. Invertebr. Pathol. 99, 345–347 (2008).

  49. 49.

    Foley, K., Fazio, G., Jensen, A. B. & Hughes, W. O. H. The distribution of Aspergillus spp. opportunistic parasites in hives and their pathogenicity to honey bees. Vet. Microbiol. 169, 203–210 (2014).

  50. 50.

    Jaber, S., Mercier, A., Knio, K., Brun, S. & Kambris, Z. Isolation of fungi from dead arthropods and identification of a new mosquito natural pathogen. Parasites and Vectors 9, 491 (2016).

  51. 51.

    Kwon-Chung, K. J. & Sugui, J. A. Aspergillus fumigatus - What Makes the Species a Ubiquitous Human Fungal Pathogen? PLoS Pathog. 9, 1–4 (2013).

  52. 52.

    Schmid-Hempel, P. Parasites in social insects. Monographs in Behavior and Ecology 291–325 (Princeton University Press 1998).

  53. 53.

    Hughes, W. O. H., Thomsen, L., Eilenberg, J. & Boomsma, J. J. Diversity of entomopathogenic fungi near leaf-cutting ant nests in a neotropical forest, with particular reference to Metarhizium anisopliae var. anisopliae. J. Invertebr. Pathol. 85, 46–53 (2004).

  54. 54.

    Poulsen, M., Hughes, W. O. H. & Boomsma, J. J. Differential resistance and the importance of antibiotic production in Acromyrmex echinatior leaf-cutting ant castes towards the entomopathogenic fungus Aspergillus nomius. Insectes Soc. 53, 349–355 (2006).

  55. 55.

    Reber, A. & Chapuisat, M. Diversity, prevalence and virulence of fungal entomopathogens in colonies of the ant Formica selysi. Insectes Soc. 59, 2231–239 (2012).

  56. 56.

    Silverman, J. & Brightwell, R. J. The Argentine Ant: Challenges in Managing an Invasive Unicolonial Pest. Annu. Rev. Entomol. 53, 231–252 (2008).

  57. 57.

    Viljakainen, L., Holmberg, I., Abril, S. & Jurvansuu, J. Viruses of invasive argentine ants from the European main supercolony: Characterization, interactions and evolution. J. Gen. Virol. 99, (2018).

  58. 58.

    Ihrmark, K. et al. New primers to amplify the fungal ITS2 region - evaluation by 454-sequencing of artificial and natural communities. FEMS Microbiol. Ecol. 82, 666–677 (2012).

  59. 59.

    White, T. J., Bruns, T., Lee, S. & Taylor, J. Amplification and direct sequencing of fungal ribosomal rna genes for phylogenetics. In PCR Protocols 315–322 (Academic Press Inc. 1990).

  60. 60.

    Lacey, L. A. & Brooks, W. M. Initial handling and diagnosis of diseased insects. In Manual of Techniques in Insect Pathology (ed. Lacey, L. A.) 1–16 (London: Academic Press 1997).

  61. 61.

    Therneau, T. M. A Package for Survival Analysis in S. version 2.38. http://CRAN.R-project.org/package=survival (2015).

Download references

Acknowledgements

We thank Dr. Viljakainen (University of Oulu, Finland) and Prof. Cremer (IST Austria) for providing the Argentine ant laboratory colony.

Author information

J.K., J.J.K. and J.J. designed and executed the experiments. J.K. and J.J. analysed the results. J.J. prepared the figures and wrote the manuscript.

Correspondence to Jaana Jurvansuu.

Ethics declarations

Competing Interests

The authors declare no competing interests.

Additional information

Publisher’s note: Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Supplementary information

Supplementary data

Supplementary video 1

Supplementary video 2

Supplementary video 3

Supplementary video 4

Supplementary video 5

Rights and permissions

Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The images or other third party material in this article are included in the article’s Creative Commons license, unless indicated otherwise in a credit line to the material. If material is not included in the article’s Creative Commons license and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this license, visit http://creativecommons.org/licenses/by/4.0/.

Reprints and Permissions

About this article

Verify currency and authenticity via CrossMark

Comments

By submitting a comment you agree to abide by our Terms and Community Guidelines. If you find something abusive or that does not comply with our terms or guidelines please flag it as inappropriate.