Vampyrum spectrum (Phyllostomidae) movement and prey revealed by radio-telemetry and DNA metabarcoding

Abstract

The spectral bat (Vampyrum spectrum), the largest bat species in the Americas, is considered Near Threatened by the International Union for Conservation of Nature and is listed as a species of special concern or endangered in several countries throughout its range. Although the species is known as carnivorous, data on basic ecology, including habitat selection and primary diet items, are limited owing to its relative rarity and difficulty in capturing the species. Leveraging advances in DNA metabarcoding and using radio-telemetry, we present novel information on the diet and movement of V. spectrum based on locations of a radio-collared individual and fecal samples collected from its communal roost (three individuals) in the Lowland Dry Forest of southern Nicaragua. Using a non-invasive approach, we explored the diet of the species with genetic markers designed to capture a range of arthropods and vertebrate targets from fecal samples. We identified 27 species of vertebrate prey which included birds, rodents, and other bat species. Our evidence suggested that V. spectrum can forage on a variety of species, from those associated with mature forests to forest edge-dwellers. Characteristics of the roost and our telemetry data underscore the importance of large trees for roosting in mature forest patches for the species. These data can inform conservation efforts for preserving both the habitat and the prey items in remnants of mature forest required by Vampyrum spectrum to survive in landscape mosaics.

About the Authors:

José Gabriel Martínez-Fonseca

Roles Conceptualization, Data curation, Formal analysis, Supervision, Writing – original draft, Writing – review & editing

* E-mail: [email protected]

Affiliations Bat Ecology & Genetics Lab, School of Forestry, Northern Arizona University, Flagstaff, Arizona, United States of America, Pathogen and Microbiome Institute, Northern Arizona University, Flagstaff, Arizona, United States of America

ORCID logo https://orcid.org/0000-0002-3181-2525

Rebecca Mau

Roles Formal analysis

Affiliation: Pathogen and Microbiome Institute, Northern Arizona University, Flagstaff, Arizona, United States of America

Faith M. Walker

Roles Conceptualization, Formal analysis, Project administration, Supervision, Writing – review & editing

Affiliations Bat Ecology & Genetics Lab, School of Forestry, Northern Arizona University, Flagstaff, Arizona, United States of America, Pathogen and Microbiome Institute, Northern Arizona University, Flagstaff, Arizona, United States of America

Arnulfo Medina-Fitoria

Roles Writing – original draft, Writing – review & editing

Affiliation: Asociación mastozoológica de Nicaragua (AMAN), Ticuantepe, Nicaragua

Kei Yasuda

Roles Data curation, Supervision, Writing – review & editing

Affiliation: Independent field research assistant, Eugene, Oregon, United States of America

Carol L. Chambers

Roles Conceptualization, Data curation, Project administration, Supervision, Writing – original draft, Writing – review & editing

Affiliation: Bat Ecology & Genetics Lab, School of Forestry, Northern Arizona University, Flagstaff, Arizona, United States of America

Introduction

With a mass of up to 235 g, the spectral bat (Vampyrum spectrum) is the largest bat species on the American continents [1, 2]. This species belongs to the subfamily Phyllostominae, the leaf-nosed bats (Phyllostomidae), which inhabit forests with relatively low anthropogenic disturbance [3–7]. The International Union for Conservation of Nature (IUCN) has designated the species as Near Threatened with a decreasing population trend throughout its range [8]. The species is considered at risk of extinction in several countries, including Bolivia, Mexico, and Nicaragua [9, 10]. In Nicaragua, V. spectrum was first recorded in 1910 and currently only a handful of capture sites are known, mainly in the Pacific and the southeastern regions of the country [11, 12]. Despite its widespread distribution on the continent, the basic ecology of the species is largely unknown [13].

Based on roost descriptions from Costa Rica, Mexico, Trinidad and Tobago, the species selects large hollow tree trunks in primary forests [2, 7]. Foraging and activity outside the roost seems to be irregular and might correspond to resource availability [2]. Mammals and birds constitute much of the diet of the species [13, 14]. Several studies recorded predation of rodents and other bat species based on prey remains (e.g., bones, wing and tail parts) at the bottom of roosts and trials with captive animals [15–17]. Feathers found at a communal roost entrance suggest the predation and transport of at least 18 bird species ranging from the 150 g White-tipped Dove (Leptotila verreauxy) to the 20 g Banded Wren (Thryothorus pleurosticus) [2]. In some cases, examination of stomach contents revealed the bones of bats, passerine birds, and arboreal rodents [13, 18, 19]. Visual examination of stomach contents and remains at roosts have obvious constraints on the ability to recognize diet items and often implies that collection of live specimens is necessary (e.g., [13]). With genetic approaches, one can identify items that have been partially or wholly digested (i.e., non-identifiable from stomach contents), exist in scarce quantities, or were eaten in a previous meal [20]. In recent years, advances in genetic techniques have facilitated the study of diet using fecal samples from a diversity of animal species including bats (e.g., [21, 22]). In Panama, metabarcoding techniques confirmed that Trachops cirrhosus fed not only on a diversity of frogs but also small mammals and reptiles [23]. However, in the Neotropics, DNA techniques for bat diet determination is a novel area for research.

The goals of this study were to identify the diet of V. spectrum and to describe roost and movement in the Lowland Dry Forest (LDF) of the Pacific coast of Nicaragua. We used habitat information for prey species identified in the diet of V. spectrum to infer forest conditions used by this predator while foraging and commuting. Additionally, we discuss management and conservation implications of our findings for this species.

Methods

Study site

Our study site encompassed the > 2000 ha Escameca Grande Private Reserve and surrounding forested lands in Rivas Department, Pacific of Nicaragua (11°12’33” N, 85°44’2” W). The Rivas Isthmus (~70 km long, 40–18 km wide) separates the Pacific Ocean and the south coast of Lake Nicaragua and includes a mosaic of pastures, seasonal and permanent crops, and remnants of mature and secondary growth of deciduous LDF [24–26]. The area experiences strong seasonality with well-marked rainy (mid-May to the end of November) and dry (remainder of year) seasons. Annual precipitation varies from 1400 to 2000 mm with areas near the Lake Nicaragua receiving higher precipitation. Terrain in the isthmus is rougher near the Pacific coast (elev. ≤400 m) with a low-elevation plain near the lake shore (elev. ~40 m) [27].

Live capture and telemetry

We used single and triple high mist nets (Avinet Research Supplies, USA) to capture bats along flyways and over water [28]. Nets were open at ~1750 h and closed at ~0030 h. Bats were handled under Nicaraguan permit of the Ministerio de Ambiente y Recursos Naturales (MARENA) No.015-122011, with the approval of the Northern Arizona University Institutional Animal Care and Use Committee (15–006) and under guidelines of the American Society of Mammologists [29]. To identify species, we used a field key and descriptions by Reid [1], Medina-Fitoria [30], and nomenclature according to Martínez-Fonseca et al. [12]. Standard morphometric measurements (mass, forearm length, sex, reproductive status) were collected from each individual.

We used two methods for attaching the radio transmitters to maximize the chances of at least one transmitter staying on the bat long enough to track the bat to roost sites. In previous attempts, we attached transmitters to large bats (e.g., Phylloderma stenops, Phyllostomus hastatus) that fell off or bats removed in ≤ 2 nights. We applied two radio transmitter models (BD2 [0.9 g], BD2C [1.1 g], Holohil Systems Ltd., Canada) to an individual to locate day roost. One transmitter was a custom-made collar designed to release after ~3 weeks and the second was designed to be attached between the scapula using a non-toxic medical glue (Torbot Liquid Bonding Cement, Torbot Group Inc., USA). We radio tracked using a close approach method [31] with a receiver (R1000, Communication Specialist Inc., USA) and two-element Yagi antenna (RA-23K, Telonics Inc., USA). We recorded all locations in geographic coordinate system WGS84 with a precision of <3 m using a handheld Global Positioning System device (Garmin 64map, Garmin Ltd., Switzerland). To confirm locations of the roost cavities, we climbed trees identified as potential roosts (based on telemetry signal) and visually inspected cavities. To record exit and entry time of the radio tagged animal from the roost, a team member monitored the signal and position of the animal with a receiver as frequently as possible at night (from 1730 h to 0630 h). To avoid disturbing the animals and affecting their behavior, observations were made at >30 m from the base of the roost tree.

Fecal DNA collection and analysis

For diet analysis, we collected 10 subsamples of fecal material upon initial discovery of the roost (Sample A). Additionally, six subsamples of fresh pellets (Sample B; defecated after discovery of the roost) were collected by placing a clear plastic sheet at the bottom of the roost and retrieving the freshly deposited guano the following day. Samples were taken from directly under the bats and constituted several guano pellets of about 2.5 ml in total volume. We only collected fresh samples one night to avoid disturbance to animals and reduce interference with their normal activity patterns.

Fecal samples were stored in 15 mL conical tubes containing 7 mL RNAlater solution (Thermo Fisher Scientific Inc., USA). Once transported to the USA, fecal samples were stored at -20°C in the Bat Ecology and Genetics lab at Northern Arizona University (https://www.nau.edu/sff). We extracted DNA from homogenized samples using a QIAamp Fast DNA Stool Mini Kit (Qiagen Inc., USA) following manufacturer instructions. We performed initial PCRs using four primers that targeted identification of a range of vertebrates and arthropods: ANML [32], 12S [33], 18S [34] and SFF [35, 36]. Each primer set was run on replicates of the 16 samples on its own plate with non-template (NTC) and positive control (PTC) for a total of 72 wells across four plates. We followed the corresponding PCR protocols and cycling conditions for each primer and used an Applied Biosystems SimpliAmp thermocycler (Thermo Fisher Scientific Inc., USA).

We removed PCR primer by-products with a 1 × bead cleanup using AMPure XP beads (Beckman Coulter Inc., USA). Indexing barcodes [37] were added with the KAPA HiFi (KAPA Biosystems Inc., USA) master mix. We quantified DNA concentrations using KAPA Library Quantification Kit (KAPA Biosystems, USA) and pooled equimolar samples for sequencing on a MiSeqGA2x with a V3 600 cycle kit (Illumina Inc., USA). All samples from all maker sets were combined in the same run.

We processed sequencing data using the QIIME2 pipeline [38]. Primers were trimmed off sequences using cutadapt [39] and paired-end reads were trimmed, denoised, joined, dereplicated, and chimera filtered using the DADA2 [40] command in QIIME2 (qiime dada2 denoise-paired). Amplicon Sequence Variants (ASVs) from the primers targeting the 12S rRNA gene were trimmed to 150bp during the DADA2 step, 18S rRNA amplicons were trimmed to 100bp, amplicons from the ANML primers targeting the COI gene were trimmed to 110bp, and amplicons from the SFF primers were trimmed to 130bp and 115bp for the forward and reverse reads, respectively. To increase confidence in diet item sequences, we required the ASV to be present in at least 3 samples and filtered out any ASVs that did not meet this requirement. We assigned taxonomy using the NCBI’s Basic Local Alignment Search Tool (BLAST) and database (https://blast.ncbi.nlm.nih.gov/). Since many species of vertebrates with recent taxonomical splits in Nicaragua do not have reference sequences in GenBank, we assigned IDs to sister species known to occur in our study area. For ranges in mass and ecological data of vertebrate species in V. spectrum fecal samples, we used Reid [1], Chavarría-Duriaux et al. [41], and Billerman et al. [42].

Results

Roost and activity patterns

On 3 March 2017, at 0000 h, we caught a post-lactating female V. spectrum (mass = 160 g, FA = 116 mm, E = 40 mm, RF = 28 mm) at ground level in the bottom shelf of a single 12 m x 2.7 m mist net. The net was located across a dry riverbed of a small tributary of the Escameca Grande River, San Juan del Sur (11°11’31" N, 85°46’6" W, 47 m). Other species captured at the same site included Artibeus jamaicensis, A. lituratus, A. phaeotis, Micronycteris microtis, Carollia perspicillata, C. subrufa, Glossophaga commissarisi, Phyllostomus discolor, Sturnira parvidens, Saccopteryx bilineata, and Tonatia bakeri.

The animal was released at the capture site following attachment of two transmitters once we ensured appropriate collar fit. Both radio transmitters combined accounted for <5% of the mass of the bat before release. We radio tracked the animal the following day to the roost area located 720 m east of the capture location. The density of standing trees, their foliage, and the fact that the bat was enclosed in the interior of a live tree affected signal radiation and, therefore, reception to ~250 m. Because of personnel and climbing equipment constraints, identifying the specific roost tree was delayed to 14 March, when a member of our team was able to climb and identify the roost entrance 12.5 m above ground in a guayabón tree (Terminalia oblonga). The roost tree was 66.5 cm diameter at breast height and 27 m tall. The roost tree contained other cavities and was located 15 m from the riverbed of the Escameca Grande.

Once the roost entrance in the tree was identified, we confirmed presence of V. spectrum inside the roost, and collect 10 subsamples “A “and came back the next day to collect six more fecal subsamples “B”. The roost cavity had a “boot” shape, with an entrance of about 20 cm in diameter that expanded to 30 cm inside. The ceiling of the roost was about 1.2 m above the entrance (Fig 1A). We observed three individual V. spectrum of approximately the same size inside (family unit). The transmitter collar was not visible because of the position (close proximity) of the three individuals (Fig 1B). The bats were observed at the upper area of the cavity and did not move during our observations. White-tipped dove (Leptotila verreauxi) feathers were recognizable at the bottom of the roost atop a guano pile, and we assumed them to be remnants of a prey item (Fig 1C). The guano pile itself was 10 cm deep, relatively flat due to decomposition of the older depositions, and filled the base of the roost except for the entrance. Recent depositions were of a lighter color than the older, more decomposed ones. Additionally, spine-like hairs of Salvin´s pocket mice (Liomys salvini) were recognizable in the fresh and old guano. We found no indication that other species (e.g., bat, arboreal mammals, or birds) used the cavity concurrently with the V. spectrum.

[Figure omitted. See PDF.]

Fig 1. Roosting Vampyrum spectrum.

Wide angle view of the roost of a radio-tagged post-lactating female (A), close-up of the three individuals roosting presumed to be a family unit (B), and entrance to the tree cavity (C), Rivas, Nicaragua, March 2017.

https://doi.org/10.1371/journal.pone.0265968.g001

Activity monitoring of the radio-tagged individual was conducted opportunistically (based on transportation and personnel availability) during 11 non-consecutive nights between 14 March to 15 April 2017. The bat left the roost once per night during each of the observation nights. The bat spent 37 to 280 minutes out of the roost each night (mean and SE: 127 ± 20.8 minutes; Table 1). The limited range of the transmitter signal in the forest environment and limited road access in the area made impossible to track the bat during foraging at night. On 16 March, the transmitter that was glued to the back of the V. spectrum was found 160 m away from the riverbed of the Escameca Grande River, 1.6 km southwest from the original capture location and 2.7 km from the roost. The area enclosed by the roost, capture site, and dropped transmitter locality was 16.3 ha (Fig 2). The transmitter in the collar stayed attached to the animal until the signal was too unreliable to monitor and vanished (probably due to battery failure) on 16 April 2017.

[Figure omitted. See PDF.]

Fig 2. Telemetry locations post-lactating female spectral bat (Vampyrym spectrum) in Escameca Grande Private Reserve, Rivas Department, Nicaragua.

Capture, roost, and dropped transmitter. The area of the minimum convex polygon is 16.3 ha. The red dot in the inset map shows the general study location in the southeastern Pacific coast of Nicaragua. Basemap layer from ArcGIS Online maps under a CC BY license, with permission from Esri, original Copyright 2018 Esri (Basemaps supported by Esri, DigitalGlobe, GeoEye, Earthstar Geographics, CNES/Airbus Ds, USDA, AEX, Getmapping, Aerogrid, IGN, IGP, swisstopo, and the GIS User Community).

https://doi.org/10.1371/journal.pone.0265968.g002

[Figure omitted. See PDF.]

Table 1. Activity log (exit and return times) of a post-lactating female Vampyrum spectrum in the Lowland Dry Forest of the southeastern Pacific coast of Nicaragua.

https://doi.org/10.1371/journal.pone.0265968.t001

Diet

We detected 27 species of terrestrial vertebrates in fecal samples representing birds and mammals, including the host species (Table 2). Sample B contained fewer vertebrate species (n = 5) compared to the Sample A (n = 25). Birds constituted the largest group, with 12 native and one non-native bird species. Maximum mass of prey ranged from 32 g (Tyrannus savanna) to 170 g (Megascops cooperi). We also detected domestic chicken (Gallus gallus; which range from 35–65 g in chicks to 1–2.5 kg adults).

[Figure omitted. See PDF.]

Table 2. Vertebrate species identified in fecal samples collected from a Vampyrum spectrum roost using four genetic markers (ANML, SFF, 12S, 18S), Rivas department, Nicaragua 2017.

https://doi.org/10.1371/journal.pone.0265968.t002

Bats represented the second largest group in species richness for V. spectrum diet. We detected 11 species of bats excluding the host DNA. Maximum mass for bat species ranged from 5 g (Rhogeessa bickami) to 59 g (Eumops underwoodi) and species encompassed nine genera. The third group of diet items contained three terrestrial rodents Liomys salvini (65 g), Sigmodon hispidus (130 g), and Sphiggurus mexicanus (~2600 g). Liomys salvini was the only species consistently detected across all 16 subsamples and four genetic markers. Several invertebrate, bacterial, and fungal groups were detected by the ANML, SFF, and 12S primers.

Arthropod groups detected included Arachnida, Blattodea, Coleoptera, Diptera, Hymenoptera, and Lepidoptera. Bonato et al. [13] reported arthropods in the diet of V. spectrum but did not clarify how they discriminated items consumed by the prey, an issue documented by Sheppard et al. [43]. There is also a likelihood that many invertebrate items originated from organisms living in the guano, or the tree. Additionally, the incompleteness of sequence libraries for Central American arthropods limits the confidence of identification of potential diet items at this time. Here, we focused our reporting and discussion on the vertebrates we identified. As reference libraries become more complete a future re-analysis of the data and provide informative results, therefore, all raw sequences from all markers were submitted to NCBI SRA (submission ID SUB10749581, BioProject ID PRJNA785628, accession numbers SAMN23572418-51).

Discussion

Considering the diversity of prey species and variation in foraging duration, we believe that V. spectrum forage opportunistically on vertebrates that included both habitat specialists and generalists. All species that we identified in the fecal samples of V. spectrum were known to occur in the study area [1, 12, 41]. Twenty-five of the vertebrate species detected in the fecal samples fall within the mass range of previously documented prey and we considered them diet items for V. spectrum [2, 7, 13, 17–19]. The SFF marker, which is optimized for identifying bat species from fecal samples [35, 36], followed by the 12S marker [33], provided the greatest diversity of identifiable vertebrate taxa with 10 species confirmed by both markers. The ANML primer [32] detected fewer vertebrate taxa; however, it was the only one that detected Megascops cooperi. This highlights the importance of using a multiple set of markers to maximize the detection of prey items.

Birds may represent an energetically cost-effective and abundant food source for V. spectrum. Species like Campylorhynchus capistratus, Coccyzus minor, Crotophaga sulcirostris, and Zenaida asiatica were already reported as part of the diet [2]. Excluding M. cooperi and Antrostomus carolinensis, all birds detected in the samples were diurnal species which might suggest that they were captured while at rest and required less energy to obtain. In addition, bird species detected are known to have diverse habitat associations. In Nicaragua, species like the mangrove cuckoo (C. minor) are mostly tied to the proximities of wetlands, riparian forests, and estuaries, while Northarchus macrorhynchus, Piaya cayana, and Campylorhynchus rufinucha are common on forest edges, secondary growth, and urbanized areas [41]. However, because the habitat descriptions of these birds corresponded to diurnal observations and not nocturnal roosts, they might not reflect the actual environment in which they were captured [44].

Unlike birds, all mammal species detected in the fecal samples of V. spectrum are predominantly nocturnal or are more active at dusk [1]. Bat species represented most of the mammal species detected in our samples and represented a range of masses, foraging guilds, and habitat associations. Species like Micronycteris microtis, M. minuta, M. schmidtorum, Pteronotus davyi, and Rhogeessa bickami are small insectivorous bats that either glean or catch their prey during flight [45–48]. Micronycteris species are often tied to mature, less-disturbed, forest conditions and are captured in small numbers in this area [26, 49]. Artibeus jamaicensis and Carollia perspicillata are frugivores, abundant along forest edges and within disturbed forests; they are also the two most abundant species in the area [26, 50–52]. The two vampire bats detected were exclusively hematophagous with Desmodus rotundus being the third most abundant species in the disturbed landscape matrix of our study area due the presence of cattle (Bos spp.; [26]). It is not clear how V. spectrum hunts and captures other bats [14, 19]. It is possible that the species can prey upon bats while they are at rest in foliage or a roost, but aerial hawking of other bat species has been observed. In Panama, V. spectrum was observed, while in flight, using one of its wings to strike and manipulate a flying Sturnira parvidens into its mouth (F. J. Bonaccorso, pers. comm.).

Liomys salvini might constitute the most common terrestrial mammal in the diet of V. spectrum and was detected in all our samples. This species of pocket mouse is abundant in mature and secondary forest in the LDF of Nicaragua and are often observed in our study area, supporting the idea that V. spectrum hunts opportunistically on available vertebrates species ([1]; Medina-Fitoria pers. comm.). Similarly sized rodents are also reported in stomach contents of V. spectrum from Panama [7, 19].

The only two species detected that did not matched mass ranges for previously described prey were S. mexicanus and domestic chicken [2, 7, 18]. Sphiggurus mexicanus is a common semiarboreal mammal species in the LDF of the Rivas Department and is often observed sharing roosts with bat species including Carollia perspicillata, Tonatia surophila, and Saccopteryx bilineata (A. Medina-Fitoria and J. G. Martínez-Fonseca pers. obs.). The detection of porcupine DNA was possibly from an individual searching for a tree cavity as a potential rest site. The DNA from domestic chicken could indicate that V. spectrum preyed on young birds (a village where chickens were common was <600 m from the roost). Both vampire species that we detected fed on blood from domestic birds and cattle [53, 54]. Although we did not detect cattle in our samples, Walker et al. [35] genetically identified cattle from D. rotundus feces, so it is not unrealistic to conclude that domestic birds could be either prey of V. spectrum or reflect diet of vampire bats that we detected.

Other “false vampire” bat species like Macroderma gigas, Megaderma lyra, and M. spasma from Australia and Asia prey on amphibians and reptiles [55–57]. However, we did not detect these despite using 12S and 18S markers which other studies have successfully used for barcoding these taxa (e.g., [58–60]). Additionally, our study was conducted during the dry season which could negatively impact the availability of these prey items for V. spectrum.

The lower diversity of diet items in Sample B compared to Sample A likely reflected that the latter represented accumulation of fecal material over a longer period, and thus more prey species. Walker et al. [35] successfully sequenced DNA in six-month-old bat fecal samples in Belize, and found that dry conditions can help preserve DNA for longer periods of time. The dry season, during which our study was conducted, might have helped reduce degradation of DNA in the feces for weeks or months.

The spatial data obtained from our radio tagged V. spectrum indicated that it used tall riparian forest areas of the LDF of Nicaragua. The sites for the roost, capture, and dropped transmitter matched assumptions of the species’ preference for medium to large patches of mature, tall canopy forests that are relatively undisturbed [2, 8, 18, 19]. This corresponded with the previous knowledge of the species in other forest types but the distance between two of our localities was 2.4 km, implying that the home range of the species is considerably greater than the 3.2 ha previously reported [2]. Both hunting and resting space (large, tall trees, and dense canopy) and safe roost sites (needed for the long period of care that V. spectrum provide for their offspring) could represent limiting factors in managed environments. The habitat required for the protection of this species should encompass its home range as well as habitat for its diverse prey [61]. Given that prey included mature forest associated species, forest management should be a focus for conservation of this species. Similar patterns for association of roost and foraging habitats in mature forest habitats have been described in other bat species like M. microtis and Pipistrellus subflavus and other taxa (e.g., birds; [26, 49, 50, 62–65]). Mature and riparian forest might also be needed for other clutter-flying adapted bat species to commute and forage in a mosaic of agricultural and forested land [25, 66]. In this work, we showed that the combination of DNA metabarcoding and telemetry techniques can improve our understanding of the ecology and community interactions of a rare carnivorous bat species. Novel ecological data on diet, roosts, and habitat use of V. spectrum provided additional support for habitat management and conservation efforts of large mature forest patches (> 2000 ha) like Escameca Grande and overall species diversity in the landscape as important components of the spectral bat habitat requirements.

Supporting information

S1 File.

https://doi.org/10.1371/journal.pone.0265968.s001

(DOCX)

Acknowledgments

We thank M. F. Chávez-Velásquez, M. Fernández-Mena, L. E. Gutiérrez-López, C. Hood, B. Noble, M. Parker, and A. Sohikian for field assistance and sample collection and transportation. We also thank Paso Pacífico and personnel C. Bonilla, H. Espinosa-Acevedo, and R. S. Castellón from the Ministerio del Ambiente y Recursos Naturales de Nicaragua (MARENA) for fieldwork logistics and research permits. We thank F. J. Bonaccorso, A. Dikeman, J. Foster, P. Fulé, S. Hershauer, J. Lyman, D. Sanchez, C. Sobek, T. Theimer, J. Upton, and E. Westeen for their training in lab techniques, sample preparation, bioinformatic analysis, and manuscript revision.

Citation: Martínez-Fonseca JG, Mau R, Walker FM, Medina-Fitoria A, Yasuda K, Chambers CL (2022) Vampyrum spectrum (Phyllostomidae) movement and prey revealed by radio-telemetry and DNA metabarcoding. PLoS ONE 17(4): e0265968. https://doi.org/10.1371/journal.pone.0265968

References

1. Reid FA. A field guide to the Mammals of Southeast Mexico and Central America. 2nd ed. New York: Oxford University Press; 2009.

2. Vehrencamp SL, Stiles FG, Bradbury JW. Observations on the Foraging Behavior and Avian Prey of the Neotropical Carnivorous Bat. J Mammal. 1977;58: 469–478.

3. Bonaccorso FJ. Foraging and reproductive ecology in a Panamanian bat community. Bull Florida State Museum. 1979;24: 359–408.

4. Cisneros LM, Fagan ME, Willig MR. Season-specific and guild-specific effects of anthropogenic landscape modification on metacommunity structure of tropical bats. J Anim Ecol. 2015;84: 373–385. pmid:25283305

5. Fenton MB, Acharya L, Audet D, Hickey MBC, Merriman C, Obrist MK, et al. Phyllostomid bats (Chiroptera: Phyllostomidae) as indicators of habitat disruption in the Neotropics. Biotropica. 1992;24: 440–446.

6. Meyer CFJ, Kalko EK V. Assemblage-level responses of phyllostomid bats to tropical forest fragmentation: land-bridge islands as a model system. J Biogeogr. 2008;35: 1711–1726.

7. Navarro L. D, Wilson DE. Vampyrum spectrum. Mamm Species. 1982;184: 1–4.

8. Aguirre LF, Mantilla H, Miller B, Dávalos LM. Vampyrum spectrum. In: The IUCN Red List of Threatened Species 2008: e.T22843A9395576. [Internet]. 2008 [cited 5 Apr 2018]. http://dx.doi.org/10.2305/IUCN.UK.2008.RLTS.T22843A9395576.en

9. Vargas Espinoza A, Aguirre LF, Emmons L, Teran M. Distribución de Vampyrum spectrum en Bolivia y comentarios sobre su estado de conservación. Ecol en Boliv. 2004;39: 46–51.

10. Medina-Fitoria A, Saldaña O, Aguirre Y, Salazar M, Martínez JG. Artículos de revisión. Bol la Red Latinoam y del Caribe para la consevación los murciélagos. 2017;8: 12–20.

11. Medina-Fitoria A, Martínez-Fonseca JG. Cronología histórica de la quiropterología en nicaragua. Rev Mex Mastozoología, nueva época. 2019;2: 1–28.

12. Martínez-Fonseca JG, Medina-Fitoria A, Westeen EP, Chambers CL. Revised Checklist of the Bats (Mammalia: Chiroptera) of Nicaragua. Occas Pap Museum Texas Tech Univ. 2021; 1–33.

13. Bonato V, Facure KG, Uieda W. Food Habits of Bats of Subfamily Vampyrinae in Brazil. J Mammal. 2004;85: 708–713.

14. Greenhall AM. Notes on the Behavior of the False Vampire Bat. J Mammal. 1968;49: 337–340.

15. Wehekind L. Notes on some Trinidad bats. J Trinidad Tobago F Nat Club. 1956; 18–21.

16. Goodwin GG, Greenhall AM. A review of the bats of Trinidad and Tobago: Descriptions, Rabies infections, and ecology. Bull Am Museum Nat Hist. 1961;122: 191–301.

17. Ditmars RL. A Vampyrum spectrum is born. Bull New York Zool Soc. 1936;39: 162–163.

18. Casebeer RS, Linsky RB, Nelson CE. The Phyllostomid Bats, Ectophylla alba and Vampyrum spectrum, in Costa Rica. J Mammal. 1963;44: 186–189.

19. Peterson RL, Kirmse P. Notes on Vampyrum spectrum, the false vampire bat, in Panama. Can J Zool. 1969;47: 140–142.

20. Sobek CJ, Walker FM. Square salads: Exploring the diet of the southern hairy-nosed wombat (Lasiorhinus latifrons) via DNA metabarcoding. Aust Mammal. 2021;43: 104–109.

21. Heim O, Puisto AIE, Fukui D, Vesterinen EJ. Molecular evidence of bird-eating behavior in Nyctalus aviator. Acta Ethol. 2019;22: 223–226.

22. Ingala MR, Simmons NB, Wultsch C, Krampis K, Provost KL, Perkins SL. Molecular diet analysis of neotropical bats based on fecal DNA metabarcoding. Ecol Evol. 2021;11: 7474–7491. pmid:34188828

23. Jones PL, Divoll TJ, Dixon MM, Aparicio D, Cohen G, Mueller UG, et al. Sensory ecology of the frog-eating bat, Trachops cirrhosus, from DNA metabarcoding and behavior. Behav Ecol. 2021;31: 1420–1428.

24. Holdridge LR. Life zone ecology. San José, Costa Rica: Tropical Science Center; 1967. https://doi.org/10.1016/0010-406x(67)90766-9 pmid:6053641

25. Martínez-Fonseca JG, Chávez-Velásquez M, Williams-Guillen K, Chambers CL. Bats use live fences to move between tropical dry forest remnants. Biotropica. 2020;52.

26. Chambers CL, Cushman SA, Medina-Fitoria A, Martínez-Fonseca J, Chávez-Velásquez M. Influences of scale on bat habitat relationships in a forested landscape in Nicaragua. Landsc Ecol. 2016;31: 1299–1318.

27. Incer J. Geografía Ilustrada de Nicaragua. Managua, Nicaragua: Recalde; 1973.

28. Kunz TH, Kurta A. Capture methods and holding devices. Ecological and behavioral methods for the study of bats. Washington D. C.: Smithsonian Institution Press; 1988. pp. 1–29.

29. Sikes RS, Mammlogist and the AC and UC of the AS of. 2016 Guidelines of the American Society of Mammalogists for the use of wild mammals in research and education. J Mammal. 2016;97: 663–688. pmid:29692469

30. Medina-Fitoria A. Murciélagos de Nicaragua: Guía de campo. Managua, Nicaragua: Programa para la Conservación de los Murciélagos de Nicaragua (PCMN) y Ministerio del Ambiente y los Recursos Naturales (MARENA); 2014.

31. Kenward RE. A Manual for Wildlife Radio Tagging. Cambridge, Massachusetts: Academic Press; 2000.

32. Jusino MA, Banik MT, Palmer JM, Wray AK, Xiao L, Pelton E, et al. An improved method for utilizing high-throughput amplicon sequencing to determine the diets of insectivorous animals. Mol Ecol Resour. 2019;19: 176–190. pmid:30281913

33. Klymus KE, Richter CA, Thompson N, Hinck JE. Metabarcoding of environmental DNA samples to explore the use of uranium mine containment ponds as a water source for wildlife. Diversity. 2017;9: 1–18.

34. Kounosu A, Murase K, Yoshida A, Maruyama H, Kikuchi T. Improved 18S and 28S rDNA primer sets for NGS-based parasite detection. Sci Rep. 2019;9: 1–12. pmid:30626917

35. Walker FM, Tobin A, Simmons NB, Sobek CJ, Sanchez DE, Chambers CL, et al. A fecal sequel: Testing the limits of a genetic assay for bat species identification. PLoS One. 2019;14: 1–16. pmid:31725795

36. Walker FM, Williamson CHD, Sanchez DE, Sobek CJ, Chambers CL. Species from feces: Order-wide identification of chiroptera from guano and other non-invasive genetic samples. PLoS One. 2016;11: 1–22. pmid:27654850

37. Colman RE, Schupp JM, Hicks ND, Smith DE, Buchhagen JL, Valafar F, et al. Detection of low-level mixed-population drug resistance in Mycobacterium tuberculosis using high fidelity amplicon sequencing. PLoS One. 2015;10: 1–18. pmid:25970423

38. Bolyen E, Rideout JR, Dillon MR, Bokulich NA, Abnet CC, Al-Ghalith GA, et al. Reproducible, interactive, scalable and extensible microbiome data science using QIIME 2. Nat Biotechnol. 2019;37: 852–857. pmid:31341288

39. Martin M. Cutadapt removes adapter sequences from high-throughput sequencing reads. Embnet.journal. 2011;17: 10–12.

40. Callahan BJ, McMurdie PJ, Rosen MJ, Han AW, Johnson AJA, Holmes SP. DADA2: High-resolution sample inference from Illumina amplicon data. Nat Methods. 2016;13: 581–583. pmid:27214047

41. Chavarría-Duriaux L, Hille DC, Dean R. Birds of Nicaragua: A field guide. New York: Zona Tropical Press; 2018.

42. Billerman SM, Keeney BK, Rodewald PG, Schulenberg TS, editors. Birds of the World. Ithaca, NY: Cornell Laboratory of Ornithology; 2020. https://birdsoftheworld.org/bow/home

43. Sheppard SK, Bell J, Sunderland KD, Fenlon J, Skervin D, Symondson WOC. Detection of secondary predation by PCR analyses of the gut contents of invertebrate generalist predators. Mol Ecol. 2005;14: 4461–4468. pmid:16313606

44. Jirinec V, Varian CP, Smith CJ, Leu M. Mismatch between diurnal home ranges and roosting areas in the Wood Thrush (Hylocichla mustelina): Possible role of habitat and breeding stage. Auk. 2016;133: 1–12.

45. Vonhof MJ. Rhogeessa tumida. Mamm Species. 2000; 1–3.

46. López-González C. Micronycteris minuta. Mamm Species. 1998; 1–4.

47. Moras LM, e Gomes AM, Da Cunha Tavares V. Distribution and taxonomy of the common big-eared bat Micronycteris microtis (Chiroptera: Phyllostomidae) in South America. Mammalia. 2015;79: 439–447.

48. Adams JK. Pteronotus davyi. Mamm Species. 1989; 1–5.

49. Solari S, Camacho M. Micronycteris microtis. In: The IUCN Red List of Threatened Species 2019: e.T136424A21985267 [Internet]. 2019 [cited 30 Jun 2021]. http://dx.doi.org/IUCN.UK.2019-2.RLTS.T136424A21985267.en

50. Ávila-Gómez ES, Moreno CE, García-Morales R, Zuria I, Sánchez-Rojas G, Briones-Salas M. Deforestation thresholds for phyllostomid bat populations in tropical landscapes in the Huasteca region, Mexico. Trop Conserv Sci. 2015;8: 646–661.

51. Ortega J, Castro-Arellano I. Artibeus jamaicensis. Mamm Species. 2001; 1–9.

52. Cloutier D, Thomas WD. Carollia perspicillata. Mamm Species. 1992;417: 1–9.

53. Greenhall AM, Joermann G, Schmidt U. Desmodus rotundus. Mamm Species. 1983; 1–6.

54. Greenhall AM, Schutt WA. Diaemus youngi. Mamm Species. 1996; 1–7.

55. Claramunt AMA, White NE, Bunce M, O’Connell M, Bullen RD, Mawson PR. Determination of the diet of the ghost bat (Macroderma gigas) in the Pilbara region of Western Australia from dried prey remains and DNA metabarcoding. Aust J Zool. 2019;66: 195–200.

56. Ramanujam ME, Verzhutskii B. The prey of the greater false vampire bat Megaderma lyra E. Geoffroy at Kaliveli, Tamil Nadu. Zoos’ Print J. 2004;19: 1655–1656.

57. Balete SD. Food and roosting habits of lesser false vamplire bat, Megaderma spasma (Chiroptera: Megadermatidae), in Philippine lowland forest. Asia Life Sciences. 2010. pp. 111–129.

58. Alvares LE, Wuyts J, Van de Peer Y, Silva EP, Coutinho LL, Brison O, et al. The 18S rRNA from Odontophrynus americanus 2n and 4n (Amphibia, Anura) reveals unusual extra sequences in the variable region V2. Genome. 2004;47: 421–428. pmid:15190359

59. Ellepola G, Herath J, Manamendra-Arachchi K, Wijayathilaka N, Senevirathne G, Pethiyagoda R, et al. Molecular species delimitation of shrub frogs of the genus Pseudophilautus (Anura, Rhacophoridae). PLoS One. 2021;16: 1–18. pmid:34665841

60. Jeong TJ, Jun J, Han S, Kim HT, Oh K, Kwak M. DNA barcode reference data for the Korean herpetofauna and their applications. Mol Ecol Resour. 2013;13: 1019–1032. pmid:23311467

61. Arrizabalaga-Escudero A, Garin I, García-Mudarra JL, Alberdi A, Aihartza J, Goiti U. Trophic requirements beyond foraging habitats: The importance of prey source habitats in bat conservation. Biol Conserv. 2015;191: 512–519.

62. Blakey RV, Law BS, Kingsford RT, Stoklosa J, Tap P, Williamson K. Bat communities respond positively to large-scale thinning of forest regrowth. J Appl Ecol. 2016;53: 1694–1703.

63. Rocha R, Ovaskainen O, Lopez-Baucells A, Farneda FZ, Sampaio EM, Bobrowiec PED, et al. Secondary forest regeneration benefits old-growth specialist bats in a fragmented tropical landscape. Sci Rep. 2018;8: 3819. pmid:29491428

64. Perry RW, Jenkins JMA, Thill RE, Thompson FR. Long-term effects of different forest regeneration methods on mature forest birds. For Ecol Manage. 2018;408: 183–194.

65. Bakermans MH, Rodewald AD, Vitz AC. Influence of forest structure on density and nest success of mature forest birds in managed landscapes. J Wildl Manage. 2012;76: 1225–1234.

66. Bader E, Jung K, Kalko EKV, Page RA, Rodriguez R, Sattler T. Mobility explains the response of aerial insectivorous bats to anthropogenic habitat change in the Neotropics. Biol Conserv. 2015;186: 97–106.