Southeastern Naturalist
197
E.J. Burge and S.D. King
22001155 SOUTHEASTERN NATURALIST 1V4o(1l.) :1149,7 N–2o1. 21
Parasites of the Carolina Bay Lake-Endemic Fundulus
waccamensis (Waccamaw Killifish)
Erin J. Burge1,* and Stanley D. King2
Abstract - Lake Waccamaw, NC, is an unusual Carolina bay home to endemic and rare species.
Parasites of the lake-endemic Fundulus waccamensis (Waccamaw Killifish) have not
been described previously. In 2011, we collected Waccamaw Killifish (n = 101) by seining
and dip netting from 3 sites over 3 seasons (spring, summer, and fall) to investigate the
identity, prevalence, and intensity of the parasite-component community. We found 13 taxa
of parasites, all of which were new host records, and total prevalence of parasitism = 95%.
Infected hosts contained 2.3 ± 1.0 (mean ± SD) parasite species, with the component community
composed of 6 ecto- and 7 endoparasites. The most prevalent (70.3%) and highest
mean intensity (17.3 metacercariae per host) infections were associated with the generalist
trematode Posthodiplostomum minimum.
Introduction
Lake Waccamaw, Columbus County, NC, is the largest extant, permanently
flooded Carolina bay lake (Frey 1949, 1950). Carolina bays are elliptical geological
features arranged on a northwest–southeast axis along the Atlantic coastal plain of
the US from Delaware to northern Florida. They are widely recognized as ecologically
important and biodiverse habitats (Sharitz 2003). The modern Lake Waccamaw
is estimated to have formed between 15,000 and 32,000 years BP (Stager and Cahoon
1987) and comprises the headwaters of the Waccamaw River, which drains into the
Atlantic Ocean at Winyah Bay, SC. Lake Waccamaw has an unusual water chemistry
that diverges from most other Carolina bay lakes in having near-neutral pH, and
high alkalinity, calcium concentration, and primary productivity (Cahoon et al. 1990,
Frey 1949, Stager and Cahoon 1987). The lake is the only one of its type that supports
a rich endemic fauna of invertebrates and fishes (Casterlin et al. 1984, Dillon
et al. 2013, Frey, 1951, Fuller 1977, Glover and Floyd 2004, Hubbs and Raney 1946,
Porter 1985, Stager and Cahoon 1987). During the late 20th century, Lake Waccamaw
experienced significant increases in nutrient concentrations attributed to lakeside development
and changing land-use patterns within the watershed, leading to increased
eutrophication and raising concerns about the sustainability of its endemic biota
(Casterlin et al. 1984, Heise and Jones 2010, Lindquist and Yarbrough 1982, Shute
et al. 2000). Biotic changes in recent years include the invasion and establishment
of Labidesthes sicculus (Cope) (Brook Silverside; Moser et al. 1998), the introduction
of the noxious submersed aquatic plant Hydrilla verticillata (L.f.) Royle (Indian
1Department of Marine Science, Coastal Carolina University, Marine Science, PO Box
261954, Conway, SC 29528-6054. 2Department of Biology, Dalhousie University, Department
of Biology, 1355 Oxford Street, Halifax, NS, Canada, B3H 4J1. *Corresponding author
- eburge@coastal.edu.
Manuscript Editor: Hayden Mattingly
Southeastern Naturalist
E.J. Burge and S.D. King
2015 Vol. 14, No. 1
198
Stargrass; Heise and Jones 2013), and population declines of endemic mussels (Heise
and Jones 2010).
Lake Waccamaw is home to several endemic invertebrates, including the caddisfly
Nectopsyche waccamawensis Glover & Floyd (Waccamaw White Miller; see
Glover and Floyd 2004), an undescribed Floridobia sp. gastropod, (Waccamaw
Siltsnail; see Dillon et al. 2013), and the 2 endemic unionid freshwater mussels,
Elliptio waccamawensis (Lea) (Waccamaw Spike) and Lampsilis fullerkati (Johnson)
(Waccamaw Fatmucket) (Porter 1985). Like nearly all unionids, these mussels
produce glochidia, a parasitic larval stage that infects skin and gill tissues of host
fishes (Kat 1984). The fishes hosting glochidia of endemic unionids have not yet
been identified (Porter and Horn 1980).
Three endemic fishes are also described from Lake Waccamaw: Fundulus waccamensis
Hubbs & Raney (Waccamaw Killifish), Etheostoma perlongum (Hubbs
& Raney) (Waccamaw Darter), and Menidia extensa Hubbs & Raney (Waccamaw
Silverside) (Hubbs and Raney 1946). Additionally, Lake Waccamaw is home to
a population of an undescribed Noturus sp. (broadtail madtom) (Bennetts et al.
1999, Rohde et al. 2009) and a slightly divergent morphotype of Notropis petersoni
Fowler (Coastal Shiner; Krabbenhoft et al. 2009a)—a cyprinid originally described
as Notropis waccamanus (Hubbs and Raney 1946). A genetically distinct population
of Elassoma boehlkei Rohde & Arndt (Carolina Pygmy Sunfish) has sporadic,
low-density occurrence in the canals and creeks adjacent to Lake Waccamaw and in
a few other localities in the Waccamaw and Santee river basins of South Carolina
(Quattro et al. 2001, Rohde and Arndt 1987).
A lacustrine origin of Waccamaw Killifish and the other lake-endemic fishes
(Waccamaw Darter and Waccamaw Silverside) was hypothesized by Hubbs and
Raney (1946) to have resulted by differentiation from the geographically widespread
sister species Fundulus diaphanus (Lesueur) (Banded Killifish), Etheostoma olmstedi
Storer (Tesselated Darter), and Menidia beryllina (Cope) (Inland Silverside),
respectively. These 3 progenitors are all found in the vicinity of Lake Waccamaw,
but not in the lake itself (Hubbs and Raney 1946, Shute et al. 1981). In their original
descriptions of the endemic fish, Hubbs and Raney (1946) remarked that the 3 species
were “decidedly slenderer and more terete” compared to their widely distributed cognates
and that they differed in head morphology and meristic characters, including
higher lateral-scale counts and more vertebrae. Geometric morphometric analyses
were used by Krabbenhoft et al. (2009a) to conclude that all 3 endemics have elongated
and streamlined morphologies relative to their sister species. They speculated that
convergent evolution for a stream-lined morphology may be an adaptation for higher
sustained swimming speeds in Fundulus and Menidia, and a “less-benthic” lifestyle
in Etheostoma selected for in the clear, open waters of Lake Waccamaw. The Waccamaw
Killifish is considered vulnerable–endangered (IUCN 2013, Krabbenhoft
et al. 2009b) and a Federal species of concern (LeGrand et al. 2012) because of its
restricted distribution in Lake Waccamaw, proximate portions of the lake-inlet creek
and canal system, and in the immediate headwaters of the Waccamaw River (Hubbs
and Raney 1946, Shute et al. 1981). Its habitat is indirectly protected because of its
Southeastern Naturalist
199
E.J. Burge and S.D. King
2015 Vol. 14, No. 1
sympatry with M. extensa which is federally listed as threatened and also restricted to
Lake Waccamaw (USFWS 1987).
Parasites have been shown to pose major threats to species at risk (McCallum
and Dobson 1995). Some estimates suggest that parasites may outnumber freeliving
species (reviewed in Dobson et al. 2008) and that they are an understudied
and underappreciated component of global biodiversity (Brooks and Hoberg 2000).
The roles of parasites in aquatic ecosystems through impacting food webs (Kuris et
al. 2008, Lafferty et al. 2006, Sukhdeo 2012), modifying host behavior (Barber et al.
2000), and providing of ecosystem services (Dobson et al. 2008, Lafferty 2008) are
important factors in aquatic community ecology. Until this study, there had been
no published research or surveys on the parasites of any endemic fish of Lake Waccamaw.
This information gap is somewhat surprising given the unique nature of the
lake, its degree of endemism in fishes and invertebrates, and the rich literature on the
parasite-component communities of other local littoral-zone fishes (e.g., Fundulus
spp.). In their review of parasites of 9 east-coast fundulids, Harris and Vogelbein
(2006) reported a speciose parasite fauna comprised of at least 93 taxa infecting
F. heteroclitus (L.) (Mummichog). Banded Killifish, the allopatric progenitor of
Waccamaw Killifish, also has a rich parasite fauna representing at least 3 protozoan
and 60 metazoan parasite species (Harris and Vogelbein 2006). King (2009) extended
the host records for both Mummichog and Banded Killifish to include 2 additional
gyrodactylids from the Canadian range: Fundulotrema foxi (Rawson) (see King
2009) and the new species Fundulotrema porterensis King & Cone (see King and
Cone 2009). Reported taxa of metazoan parasites from Fundulus spp. include representatives
from nearly every phylum and those with both one-host (monoxenous) and
multi-host (heteroxenous) life cycles. Fundulus spp. commonly host endoparasites
including nematodes, acanthocephalans, myxozoa, cestodes, and digenean trematodes
and ectoparasites from the monogenoid, ciliophoran, annelid, and crustacean
(copepods and brachiurids) groups.
Gyrodactylidae is a speciose group within the Monogenea that are common
ectoparasites of teleosts, with a few exceptional species infecting amphibians and
cephalopods (Bakke et al. 1992). Most gyrodactylids exhibit high host specificity
wherein species often infect only a single host or host genus. Fundulotrema, for example,
contains a group of 6 described species, 5 of which have only been reported
from species of Fundulus, and the 6th from a closely related cyprinodontid, Lucania
goodei Jordan (Bluefin Killifish). It has been suggested that gyrodactylids and other
highly host-specific parasites are more likely to co-speciate with their host due to
their phylogenetic conservatism in host choice (Huyse et al. 2003, Rohde 1993).
Considering this possibility, we might expect to find new species of parasites when
studying a recently diverged host that has yet to be examined for parasites.
In the current study, we undertook the first survey of the parasite-component community
of the Waccamaw Killifish. Our goals were to increase our understanding
of the biology and ecology of this endemic fish and to evaluate whether the unique
conditions in Lake Waccamaw have concealed undescribed species of parasites. Our
data will also serve as a baseline for future comparisons of biodiversity in light of
concerns regarding water quality and on-going biotic changes within the lake.
Southeastern Naturalist
E.J. Burge and S.D. King
2015 Vol. 14, No. 1
200
Methods
Field collections
We collected specimens from 3 different shoreline sites of Lake Waccamaw,
Columbus County, NC. We chose sites based on historical occurrences of Waccamaw
Killifish (Heise and Jones 2010; Shute et al. 1981, 1983, 2000), ease of
accessibility, and preliminary collections that indicated this species was abundant at
these locations. Characteristics of collection sites were largely representative of the
entire periphery of Lake Waccamaw and included a north-shore beach (34°19'01"N,
78°31'30"W; site 1a in Shute et al. 1981), the southwest corner of the lake at the
spillway (34°15'39"N, 78°31'22"W; site 1g in Shute et al. 1981), and a sandy beach
area on the south shore in Lake Waccamaw State Park (34°15'28"N, 78°30'57"W;
site 1f in Shute et al. 1981). More detailed site descriptions are available in Shute
et al. (1981). For background on the physical and chemical characteristics and biota
of Lake Waccamaw see Casterlin et al. (1984) and Frey (1949, 1950).
We collected specimens retained for parasitological examination (n = 101) in 2011
on 16 March (n = 4), 22 April (n = 22), 12 July (n = 20), 26 August (n = 10), 6 October
(n = 15), 27 October (n = 15), and 17 November (n = 15). Typically, we only retained
adults >45 mm (n = 93) for parasite dissections but in some months with limited sample
sizes, we used smaller individuals. We employed small seines (3.0 m × 0.91 m with
3-mm mesh and 6.1 m × 0.91 m with 6-mm mesh) and dip nets to capture fish in open
water. Immediately after capture, we euthanized fish with a fatal overdose of tricaine
methanesulfonate (MS-222; Sigma-Aldrich Company, St. Louis, MO). Each specimen
was identified to sex, measured for total length (TL) to the nearest 0.1 mm with
calipers, and transferred into 10% neutral-buffered formalin in individual glass vials
to ensure retention of loosely associated or motile ectoparasites.
Collections were permitted under the following licenses: North Carolina Wildlife
Resources Commission (NCWRC) Endangered Species Permit 10-ES00306,
NCWRC Scientific Fish Collecting License No. 1207, and North Carolina Division
of Parks and Recreation Scientific Research and Collecting Permit R10-50. We
submitted data on all fish collected to the NCWRC as required by 10-ES00306.
Parasite surveys
We used stereo and compound microscopes to aid our necropsies of Waccamaw
Killifish, which included examination of the fins, body, buccal cavity and musculature
of the head, gills, eyes, brain, ureters, intestine, liver, heart, gallbladder,
gonads, air bladder, spleen, and mesenteries of preserved fishes following the procedures
of Harris and Vogelbein (2006) and King (2009). We examined the fixative
and sediment in each vial for dislodged ectoparasites. We prepared any parasites
encountered as temporary wet-mounts and identified each to species or the lowest
taxonomic level possible by comparing their morphological characters to taxonomic
keys (Hoffman 1999), original species descriptions, and in some cases, the
type material. We identified gyrodactylids by staining the haptoral bars of representative
specimens with Gomori’s trichrome (Kritsky et al. 1978) and examined all
sclerotized features of the opisthaptor (dorsal and ventral bars, anchors, and marginal
hooks) and male copulatory organ using bright-field, phase, and differential
Southeastern Naturalist
201
E.J. Burge and S.D. King
2015 Vol. 14, No. 1
interference-contrast optics (Malmberg 1970). We prepared gyrodactylid voucher
specimens by dehydration in absolute ethanol, clearing in xylene, and re-mounting
in Canada balsam all stained samples. Stephen S. Curran (Department of Coastal
Sciences, The University of Southern Mississippi, Hattiesburg, MS) and Eugene
M. Burreson (Department of Environmental and Aquatic Animal Health, Virginia
Institute of Marine Science, Gloucester Point, VA) provided supplemental and confirmatory
identifications of trematodes and nematodes, and annelids, respectively.
We deposited voucher specimens for the following species at the Harold W. Manter
Laboratory of Parasitology (University of Nebraska State Museum, Lincoln, NE)
under the accession number P-2014-034 and the following catalog numbers: Ergasilus
lizae Krøyer (HWML #64652 and 64653), Fundulotrema porterensis (HWML
#74999 and 75001), Fundulotrema prolongis (Hargis) (HWML #74998 and 75002),
Gyrodactylus stephanus Müller (HWML #75000 and 75003), Myzobdella lugubris
Leidy (HWML #64654), Pomphorhynchus bulbocolli Linkins (HWML # 64655),
and Posthodiplostomum minimum (MacCallum) (HWML #64656).
Data analysis
Prevalence and mean intensity as defined by Bush et al. (1997) with 95% confidence
intervals were calculated with the parasitology statistical software QPweb
1.0.6 (Rózsa et al. 2000). Confidence intervals for prevalence were calculated by
the Clopper-Pearson method, and those for mean intensity used bootstrap methods
with 2000 permutations (Rózsa et al. 2000).
Because the data presented on the parasite component community represent a
relatively small number of sampled hosts of this threatened species (n = 101), additional
analyses beyond describing the community are relatively limited. We include
them for illustrative purposes and as suggestions for future research. To calculate
a total parasite burden and examine seasonality and sex as factors affecting the
parasite infracommunities of hosts, an individual parasitization index (IPI) was calculated
for each host following the formula of Kalbe et al. (2002) and included all
parasite taxa. The correlation of IPI and host TL was compared with the nonparametric
Spearman’s rank correlation. Parasite burdens as IPI were compared between sex
and season using two-way analysis of variance on square-root transformed IPI after
confirming that the data were normally distributed (Shapiro-Wilk test) and of equal
variance (SigmaPlot v. 12.3, Systat Software, Inc.). Individual fish were grouped
by season as spring (March–April, n = 26); summer (July–August, n = 30); and fall
(October–November, n = 45).
We used nonmetric multidimensional scaling (NMDS) to examine preliminary
patterns of the parasite infracommunities by host sex and season in the dataset.
Bray-Curtis similarity on 4th-root transformed parasite abundances was calculated
in Plymouth Routines in Multivariate Ecological Research (PRIMER-E v. 5.2.9)
(Clarke 1993). Rarefaction analysis was conducted in EstimateS v. 9.1.0 with 100
randomized resamplings. The species richness estimation (Sobs) was considered to
be asymptotic if the 95% confidence interval of Sobs and the Chao2 parameter were
equal to the observed number of species (S obs) (Colwell 2013).
Southeastern Naturalist
E.J. Burge and S.D. King
2015 Vol. 14, No. 1
202
Results
We examined 101 Waccamaw Killifish (67 females and 34 males) from 3 sites
and 3 seasons (spring, summer, and fall) for the presence of ecto- and endoparasites.
Individual fish ranged in size from 25.9–92.2 mm TL, with a mean ± SD TL
of 63.4 mm ± 14.3, and we found no significant difference in TL by sex (ANOVA:
P = 0.18). Lengths of 8 individuals were less than the target size of 45 mm.
Of the 101 Waccamaw Killifish examined, we found parasites infecting 96
individuals (overall parasite prevalence = 95%) and identified 13 parasite taxa
(Table 1). We present parasite prevalence, mean intensity, life stage, location on
or in the host, and taxa in Table 1. The parasite-component community consisted
of 200 individuals of 6 ectoparasites (3 monogenoids, 1 unionid, 1 copepod, and 1
leech) and 1560 individuals of 7 endoparasites (3 digeneans, 1 cestode, unidentified
nematodes, and 2 acanthocephalans).
Parasite-species richness ranged from 1 to 5 per host individual, with a mean
± SD = 2.3 ± 1.0 species per infected host. Rarefaction analysis suggested that
the sample size of hosts examined was sufficient to capture the richness of the
parasite-component community of the Waccamaw Killifish (Fig. 1). Both the Chao2
parameter and extrapolated species richness (data not shown) converged on the
observed species richness.
Figure 1. Rarefaction-curve analysis of parasite-species richness assessed from Waccamaw
Killifish (n = 101). Drop points on the line represent the estimated numbers of individual
fish required to capture 50%, 75%, and 95% of the observed paras ite-species richness.
Southeastern Naturalist
203
E.J. Burge and S.D. King
2015 Vol. 14, No. 1
Table 1. Biological information and descriptive statistics for the parasite-component community found infecting Fundulus waccamensis (n = 101). Terminology
follows the definitions of Bush et al. (1997). Location on/in host refers to the parasite habitat as F = fins, G = gills, H = head (buccal cavity and
musculature), I = intestine, L = liver, M = mesenteries, O = operculum, S = swim bladder, and V = ovary. Confidence intervals (95% CI) for prevalence
were calculated by the Clopper-Pearson method and values for mean intensity are bootstrapped from 2000 permutations. All values were calculated as
described in Rózsa et al. (2000) using QPWeb 1.0.6.
Parasite Location % prevalence Mean intensity
Parasite taxa life stage on/in host (95% CI) (95% CI)
Phylum Platyhelminthes, Class Monogenea
Gyrodactylus stephanus Müller Adult F, G, O 8.91 (4.2–16.2) 1.67 (1.11–2.44)
Fundulotrema prolongis (Hargis) Adult F 14.90 (8.6–23.3) 6.40 (3.53–13.7)
Fundulotrema porterensis King & Cone Adult F, G 2.97 (0.6–8.4) 1.00
Phylum Platyhelminthes, Class Trematoda
Posthodiplostomum minimum MacCallum Metacercariae H, M, V 70.30 (60.4–79) 17.27 (13.9 - 21.5)
Homalometron cf. pallidum Stafford Adult I 20.80 (13.4–30) 8.38 (4.14–17.2)
Unidentified digenean (Allocreadiidae?) Adult I 2.97 (0.6–8.4) 1.67 (1–2.33)
Phylum Platyhelminthes, Class Cestoidea
Proteocephalus sp. Metacestode M 8.91 (4.2–16.2) 1.33 (1–1.56)
Phylum Nematoda
Unidentifed nematodes (Eustrongylides sp. and Spiroxys sp.?) Larvae L, M, S, V 50.50 (40.4–60.6) 2.41 (2–2.86)
Phylum Acanthocephala, Class Eoacanthocephala
Neoechinorhynchus sp. Cystacanth L, M 11.90 (6.3–19.8) 1.42 (1.08–1.58)
Phylum Acanthocephala, Class Palaeacanthocephala
Pomphorhynchus bulbocolli Linkins Adult I 1.00 (0–5.4) 1.00
Phylum Annelida, Class Hirudinea
Myzobdella lugubris Leidy Adult F 2.97 (0.6–8.4) 1.00
Phylum Arthropoda, Class Maxillopoda
Ergasilus lizae Krøyer Adult G 8.91 (4.2–16.2) 2.89 (2–4.11)
Phylum Mollusca, Class Bivalvia
Unionid spp. Glochidia G 16.80 (10.1–25.6) 3.35 (2.06–5.53)
Southeastern Naturalist
E.J. Burge and S.D. King
2015 Vol. 14, No. 1
204
There was a significant positive correlation (Spearman r = 0.238, P = 0.03)
between host standard length and individual parasitization index (IPI) independent
of sex, although the relationship was not particularly predictive. We
also examined IPI with regards to sex and season and found no significant differences
in total parasite burden (two-way ANOVA: season P = 0.15, sex P =
0.92). In contrast, analysis of Bray-Curtis similarity between individual hosts
using nonmetric multidimensional scaling (NMDS) suggested that there may be
seasonal differences in parasite infracommunities (Fig. 2); spring samples were
largely spatially separate from summer and fall samples, which substantially
overlapped. Spring samples were distinguishable from summer and fall samples
by the prevalence of up to 3 gyrodactylid species (Gyrodactylus stephanus,
Figure 2. Nonmetric multidimensional scaling (NMDS) ordination map of parasite burden
in Fundulus waccamensis (Waccamaw Killifish) constructed from the Bray-Curtis similarity
matrix of all host infracommunities. Bubbles are shaded by season of host collection
and the sizes of points scaled by the individual parasitization index (IPI) for that individual.
Stress of the ordination was 0.10 from 30 random restarts.
Southeastern Naturalist
205
E.J. Burge and S.D. King
2015 Vol. 14, No. 1
Fundulotrema prolongis, Fundulotrema porterensis) and the lower intensity and
prevalence of Posthodiplostomum minimum. The latter trematode species was the
parasite found at highest prevalence and intensity in our samples. Gyrodactylids
had a combined spring prevalence (95% confidence interval) of 65.4% (44.3–
82.8). Eight Waccamaw Killifish had co-infections of 2 species of gyrodactylids
and 1 specimen was host to all 3, but none of the fish we collected during the
summer or fall showed evidence of infection with this group of parasites. In
contrast, in specimens collected in summer and fall, P. minimum was at high
prevalence and high intensity—88.0% (78.4–94.4) and 18.2 (15–23.5) metacercariae
per fish, respectively—compared to spring specimens (prevalence = 19.2%
[6.6–39.4]), mean intensity = 4.6 (1–11.4).
We identified parasites to the lowest taxonomic unit possible using morphological
characteristics (Table 1). Known reported hosts and information about life
cycles for the identified parasites are presented in Table 2. The unidentified parasites
included an adult digenean similar to members of the Allocreadiidae and present
in 3 hosts (3% prevalence). Larval nematodes were relatively common (51%) but
could not be separated to species without DNA analyses. Likewise, metacestodes
of Proteocephalus sp. (9%), cystacanths of Neoechinorhynchus sp. (12%), and
unionid glochidia (17%) require further morphological and DNA-sequence data to
identify to species.
Table 2. Reported hosts and life-cycle information for parasites identified to species infecting Fundulus
waccamensis (Waccamaw Killifish). Parasite information is from Hoffman (1999) except for
AKing and Cone (2009). Reported hosts known from Lake Waccamaw reported in BShute et al. (1981),
CDillon et al. (2013), and DCahoon (2005). For life-cycle information, intermediates are numbered and
definitive hosts noted (Def).
Parasite taxa Reported hosts Life cycle
Gyrodactylus stephanus Müller Fundulus diaphanus, F. grandis, Direct, viviparous
F. heteroclitus, F. majalis, Pungitius
pungitius (L.) (Nine-spined Stickleback)
Fundulotrema prolongis (Hargis) F. diaphanus, F. grandis, F. heteroclitus Direct, viviparous
Fundulotrema porterensis King F. diaphanus, F. heteroclitusA Direct, viviparous
& Cone
Posthodiplostomum minimum FW fishes including Fundulus, especially 1: Physa snailsC,
MacCallum centrarchids and cyprinidsB 2: FW fishes, Def:
piscivorous birds
Homalometron cf. pallidum F. diaphanus, F. heteroclitus, Aplodinotus 1: Hydrobiid snailsC,
Stafford grunniens Rafinesque (Freshwater Drum), Gemma clams,
Morone americanaB (Gmelin) (White Perch) Def: FW fishes
Pomphorhynchus bulbocolli FW fishes including Fundulus 1: Gammarid
Linkins amphipodsD
Myzobdella lugubris Leidy FW fishes including Fundulus Direct, oviviparous
Ergasilus lizae Krøyer FW and marine fishes, F. diaphanus, Direct, oviviparous
F. grandis, F. heteroclitus, F. similis
(Baird & Girard) (Longnose Killifish)
Southeastern Naturalist
E.J. Burge and S.D. King
2015 Vol. 14, No. 1
206
Discussion
Here we report, for the first time, on the parasite-component community of the
threatened, endemic Waccamaw Killifish. This species had a relatively depauperate
parasite community—13 taxa—compared to reports of 65 described parasite
species for its allopatric progenitor, Banded Killifish (Harris and Vogelbein 2006,
King 2009). The high numbers of parasite taxa reported from Banded Killifish and
Mummichog, also found locally, are certainly influenced by their wide geographic
ranges and the sizeable amount of investigative effort devoted to describing their
parasite faunas. Fundulid-parasite surveys from a single or several close localities
more narrowly constrained in time (months to years) have reported a variety of
parasite-species richness values: 27 species for Banded Killifish (protozoan and
metazoan, n = 869 hosts; Wiles 1975), 22 species for Mummichogs (protozoan
and metazoan, n = 150 hosts; Harris and Vogelbein 2006), 10 species for Fundulus
luciae (Baird) (Spotfin Killifish; metazoan only, n = 341 hosts; Byrne 1978),
and 44 species from F. grandis Baird & Girard (Gulf Killifish; metazoan only,
n = 3200 hosts; Ruiz 2013). It remains to be seen whether the parasites of other
fundulid sibling-species pairs with a common representative and a rare/endemic
one such as F. parvipinnis Girard (California Killifish)–F. lima Vaillant (Baja California
Killifish) (Reyes-Valdez et al. 2011) and F. olivaceus Storer (Blackspotted
Topminnow)–F. euryzonus Suttkus & Cashner (Broadstripe Topminnow) (Schaefer
et al. 2009) also demonstrate the apparent large disparity in parasite-species
richness. It would be of interest to test this observation by examining the parasite
community of the North Carolina allopatric Banded Killifish species complex that
includes Waccamaw Killifish and a genetically distinct, undescribed species, F. sp.
cf. diaphanus (“Lake Phelps” Killifish; Tracy et al. 2013).
A statistically significant difference in the parasite infracommunities was not
evident by sex or season, although the results of NMDS ordination (Fig. 2) suggest
that seasonality may be a factor of importance for gyrodactylids and Posthodiplostomum
minimum. Seasonality in gyrodactylid infection in Mummichog has been
previously reported (Barse 1998). Both factors have been implicated as important
in some host systems but no universal conclusions seem to fit the variety of patterns
(or lack thereof) observed (Kennedy 2009; Poulin 1996, 2007a). Conversely, strong
evidence supports the relationship between corresponding increases between hostfish
size or age and parasite intensity (Poulin 2000, Wilson et al. 2002).
All of the parasites reported from Waccamaw Killifish represent new host records
for those species. Waccamaw Killifish is a lacustrine-derived sibling species
of the Banded Killifish, but the two species inhabit quite different habitats in the
southern portion of their ranges in the Carolinas. Waccamaw Killifish are restricted
to Lake Waccamaw and found seasonally in adjacent canals, while Banded Killifish
are considered residents of clear-flowing waters, including inland streams and the
shallow, tidal portions of larger rivers like the Waccamaw and Cape Fear rivers.
The Waccamaw River basin represents the southern limit of the range for Banded
Killifish, where it has only rarely been collected in the downstream portions of the
river (see Rohde et al. 2009, Shute et al. 1981), ~80 km from Lake Waccamaw.
Southeastern Naturalist
207
E.J. Burge and S.D. King
2015 Vol. 14, No. 1
The observed parasite fauna of Waccamaw Killifish probably reflects that of the
component community infecting the ancestral host at the time Lake Waccamaw
was originally colonized. Once isolated, this host was likely buffered from acquiring
infections of new parasites, except generalist parasites with complex life cycles
that may have been added to the lake via motile intermediate or definitive hosts
(see Table 2). The parasite community of Waccamaw Killifish may have also experienced
a reduction in membership due to seasonal fluctuations in parasite populations
and the inability for re-colonization after local extinctions (Dunn et al. 2009,
Lafferty and Kuris 2009), further explaining the paucity of parasite species. This
may, in part, explain the absence of several monoxenous taxa that we expected to
be present on our samples because they are common as infections of Banded Killifish
(Harris and Vogelbein 2006, Hoffman 1999, King 2009). These taxa include
protozoan trichodinids, fungal microsporidians, the cnidarian myxozoa, and mongenean
dactylogyrids, all of which commonly infect Banded Killifish over a broad
geographic range.
The parasite community of Waccamaw Killifish was strikingly similar to that of
Banded Killifish. All of the taxa we documented on Waccamaw Killifish, except the
unidentified digenean, had previously been reported from Banded Killifish (Harris
and Vogelbein 2006, Hoffman 1999, King 2009, King and Cone 2009, Wiles 1975),
thus supporting the probable shared evolutionary history of these 2 host species.
Interestingly, the host record for Fundulotrema porterensis is the first report of this
gyrodactylid species outside of 2 adjacent lakes in Nova Scotia (King and Cone
2009), and our observation suggests a wider distribution for this species than has
been demonstrated. One of our research objectives was aimed at investigating if any
undescribed species of gyrodactylid infected Waccamaw Killifish. The 2 proposed
mechanisms responsible for speciation in the Gyrodactylidae are via host-switching
and parasite/host co-speciation (Bakke et al. 2002, Huyse et al. 2003, Ziętara and
Lumme 2002). Although speciation via host switching is suspected to play a larger
role in the speciation of gyrodactylids (Ziętara and Lumme 2002), there have been
examples of co-speciation reported (Huyse and Volckaert 2005, Huyse et al. 2003).
If patterns of co-speciation persist, the phylogeny of the parasite should be congruent
with the phylogeny of the host, as suggested by Fahrenholz’s rule (Poulin
2007b). The isolation of Lake Waccamaw provided a unique opportunity to examine
the co-speciation potential in gyrodactylids. Lake Waccamaw is suspected to
have been isolated no more than 32,000 years BP (Stager and Cahoon 1987), so we
can estimate that Waccamaw Killifish has likely undergone a maximum of 32,000
generations (assuming first spawning at 1+ years old). Clearly there have been a
sufficient number of generations to accrue visible morphological differences from
Banded Killifish (Hubbs and Raney 1946, Krabbenhoft et al. 2009a). Comparatively,
the reproductive rate of gyrodactylids is much higher (reviewed in Bakke et al.
2002), and if assumed to be similar to Gyrodactylus bullatarudis Turnbull, which
infects another cyprinodontid host, the total number of generations for the same
time period is estimated to be orders of magnitude larger (~5.8 million generations;
Scott 1982). Yet, the gyrodactylids infecting Waccamaw Killifish are morphologically
very similar if not identical to individuals infecting Ba nded Killifish.
Southeastern Naturalist
E.J. Burge and S.D. King
2015 Vol. 14, No. 1
208
It was hypothesized that undescribed gyrodactylid diversity may be present in
Lake Waccamaw given the unique conditions of the lake and its documented endemicity
for many taxa (reviewed in LeGrand et al. 2012), but this was not the case for
the Waccamaw Killifish. However, these parasites are renowned for their morphological
conservation, and there are multiple examples of cryptic species being identified
only after molecular genotyping (Cunningham et al. 2001, Ziętara and Lumme
2003). The same cryptic diversity may be at play here, but molecular investigation is
needed. In the absence of molecular data, this study provides anecdotal evidence that
speciation of the host does not always facilitate speciation in gyrodactylids, at least
over relatively short evolutionary temporal frames.
Building on this baseline description of the parasite-component community of
Waccamaw Killifish, future work should focus on how changes in land-use patterns,
water quality, and biota within Lake Waccamaw affect population resiliency and
parasitism of endemics. A large body of research has demonstrated that parasites
often respond differently than their hosts to pollution and changes in water quality
(reviewed in Blanar et al. 2009). Parasites are often keystone species (McCallum
and Dobson 1995), and changes to the host or parasite community facilitated by deteriorating
water quality may have profound effects on the lake as a whole. In future
studies, it would also be of interest to elucidate the host-parasite relationships of
rare and endemic Lake Waccamaw mussel glochidia, which would require molecular
analyses. Lastly, the parasites of Carolinian populations of Banded Killifish and
another lacustrine-derived sister species within the Banded Killifish-complex, the
“Lake Phelps” Killifish, have not yet been investigated and may provide insights on
community structure of parasites during allopatric speciation of their hosts.
Acknowledgments
We were assisted with field collections by R. Burge, P. Burge, and W. Burge; C. Hill
(Coastal Carolina University, Department of Biology); Coastal Carolina University marine
science students S. Dumoff, A. Ruis, T. Schacht, L. Scribner, and J. Yunginger; and Coastal
Marine and Wetland Studies graduate students M. Helms, G. Lockridge, C. Smith, and
C. Wessel. For help with site selection and orientation, the authors thank R. Heise (NCWRC)
and F. Rohde (NOAA). Parasite identification assistance was generously provided
by S. Curran (Department of Coastal Science, University of Southern Mississippi) and E.
Burreson (Department of Environmental and Aquatic Animal Health, Virginia Institute of
Marine Science). Collecting equipment, supplies, and transportation were partially funded
by the Coastal Carolina University departments of Biology and Marine Science, and page
charges were provided by the Dean of the College of Science. S. King was funded in part
by a Natural Sciences and Engineering Research Council (NSERC) CGS-D grant, and the
New Brunswick Museum (Canada) and the Royal BC Museum (Canada) funded taxonomic
work on gyrodactylids.
Literature Cited
Bakke, T.A., P.D. Harris, P.A. Jansen, and L.P. Hansen. 1992. Host specificity and dispersal
strategy in gyrodactylid monogeneans, with particular reference to Gyrodactylus salaris
(Platyhelminthes, Monogenea). Diseases of Aquatic Organisms 13:63–74.
Southeastern Naturalist
209
E.J. Burge and S.D. King
2015 Vol. 14, No. 1
Bakke, T.A., P.D. Harris, and J. Cable. 2002. Host-specificity dynamics: Observations on
gyrodactylid monogeneans. International Journal for Parasitolog y 32:281–308.
Barber, I., D. Hoare, and J. Krause. 2000. Effects of parasites on fish behavior: A review and
evolutionary perspective. Reviews in Fish Biology and Fisheries 10:131–165.
Barse, A.M. 1998. Gill parasites of Mummichogs, Fundulus heteroclitus (Teleostei: Cyprinodontidae):
Effects of season, locality, and host sex and size. Journal of Parasitology
84:236–244.
Bennetts, R., J. Grady, F. Rohde, and J. Quattro. 1999. Discordant patterns of morphological
and molecular change in broadtail madtoms (genus Noturus). Molecular Ecology
8:1563–1569.
Blanar, C.A., K.R. Munkittrick, J. Houlahan, D.L. MacLatchy, and D.J. Marcogliese. 2009.
Pollution and parasitism in aquatic animals: A meta-analysis of effect size. Aquatic
Toxicology 93:18–28.
Brooks, D.R., and E. Hoberg. 2000. Triage for the biosphere: The need and rationale for
taxonomic inventories and phylogenetic studies of parasites. Journal of the Helminthological
Society of Washington 67:1–25.
Bush, A.O., K.D. Lafferty, J.M. Lotz, and A.W. Shostak. 1997. Parasitology meets ecology
on its own terms: Margolis et al. revisited. Journal of Parasitology 83:575–583.
Byrne, D.M. 1978. Life history of the Spotfin Killifish, Fundulus luciae (Pisces: Cyprinodontidae),
in Fox Creek Marsh, Virginia. Estuaries 1:211–227.
Cahoon, L.B. 2005. Demersal zooplankton vs. net plankton abundances in Lake Waccamaw,
North Carolina. Journal of the North Carolina Academy of Science 121:125–134.
Cahoon, L.B., J.R. Kucklick, and J.C. Stager. 1990. A natural phosphate source for Lake
Waccamaw, North Carolina, USA. Internationale Revue der gesamten Hydrobiologie
und Hydrographie 75:339–351.
Casterlin, M.E., W.W. Reynolds, D.G. Lindquist, and C.G. Yarbrough. 1984. Algal and physiochemical
indicators of eutrophication in a lake harboring endemic species: Lake Waccamaw,
North Carolina. Journal of the Elisha Mitchell Scientific Society 100:83–103.
Clarke, K.R. 1993. Non-parametric multivariate analyses of changes in community structure.
Australian Journal of Ecology 18:117–143.
Colwell, R.K. 2013. EstimateS: Statistical estimation of species richness and shared species
from samples. Version 9. Available online at http://purl.oclc.org/estimates. Accessed 10
February 2014.
Cunningham, C.O., T.A. Mo, C.M. Collins, K. Buchmann, R. Thiery, G. Blanc, and A. Lautraite.
2001. Redescription of Gyrodactylus teuchis Lautraite, Blanc, Thiery, Daniel &
Vigneulle, 1999 (Monogenea: Gyrodactylidae): A species identified by ribosomal RNA
sequence. Systematic Parasitology 48:141–150.
Dillon, R.T., Jr., M. Ashton, M. Kohl, W. Reeves, T. Smith, T. Stewart, and B. Watson. 2013.
The freshwater gastropods of North America. Available online at http://www.fwgna.org.
Accessed 20 March 2014.
Dobson, A., K.D. Lafferty, A.M. Kuris, R.F. Hechinger, and W. Jetz. 2008. Homage to Linnaeus:
How many parasites? How many hosts? Proceedings of the National Academy of
Sciences 105:11,482–11,489.
Dunn, R.R., N.C. Harris, R.K. Colwell, L.P. Koh, and N.S. Sodhi. 2009. The sixth mass
coextinction: Are most endangered species parasites and mutualists? Proceedings of the
Royal Society B: Biological Sciences 276:3037–3045.
Frey, D.G. 1949. Morphometry and hydrography of some natural lakes of the North Carolina
coastal plain: The bay lake as a morphometric type. Journal of the Elisha Mitchell
Scientific Society 65:1–37.
Southeastern Naturalist
E.J. Burge and S.D. King
2015 Vol. 14, No. 1
210
Frey, D.G. 1950. Carolina bays in relation to the North Carolina Coastal Plain. Journal of
the Elisha Mitchell Scientific Society 66:44–52.
Glover, J.B., and M.A. Floyd. 2004. Larvae of the genus Nectopsyche (Trichoptera: Leptoceridae)
in eastern North America, including a new species from North Carolina. Journal
of the North American Benthological Society 23:526–541.
Harris, C.E., and W.K. Vogelbein. 2006. Parasites of Mummichogs, Fundulus heteroclitus,
from the York River, Virginia, USA, with a checklist of parasites of Atlantic Coast Fundulus
spp. Comparative Parasitology 73:72–110.
Heise, R.J., and B.K. Jones. 2010. Lake Waccamaw fish- and mollusk-status surveys. North
Carolina Wildlife Resources Commission, Aquatic Wildlife Diversity Program, Raleigh,
NC. 14 pp.
Heise, R.J., and B.K. Jones. 2013. Lake Waccamaw fish and mollusk-status surveys. North
Carolina Wildlife Resources Commission, Aquatic Wildlife Diversity Program, Raleigh,
NC. 18 pp.
Hoffman, G.L. 1999. Parasites of North American Freshwater Fishes. Comstock Publishing
Associates, Cornell University Press, Ithaca, NY. 539 pp.
Hubbs, C.L., and E.C. Raney. 1946. Endemic fish fauna of Lake Waccamaw, North Carolina.
Miscellaneous Publications 65. University of Michigan Museum of Zoology, Ann
Arbor, MI. 38 pp.
Huyse, T., and F.A.M. Volckaert. 2005. Comparing host and parasite phylogenies: Gyrodactylus
flatworms jumping from goby to goby. Systematic Biology 54:710–718.
Huyse, T., V. Audenaert, and F.A.M. Volckaert. 2003. Speciation and host–parasite relationships
in the parasite genus Gyrodactylus (Monogenea, Platyhelminthes) infecting gobies
of the genus Pomatoschistus (Gobiidae, Teleostei). International Journal for Parasitology
33:1679–1689.
International Union for Conservation of Nature (IUCN). 2013. IUCN Red List of Threatened
Species, Fundulus waccamensis. IUCN Version 2013.2. Available online at http://
www.iucnredlist.org. Accessed 6 January 2014.
Kalbe, M., K.M. Wegner, and T.B.H. Reusch. 2002. Dispersion patterns of parasites in
0-year+ Three-spined Sticklebacks: A cross-population comparison. Journal of Fish
Biology 60:1529–1542.
Kat, P.W. 1984. Parasitism and the Unionacea (Bivalvia). Biological Reviews 59:189–207.
Kennedy, C.R. 2009. The ecology of parasites of freshwater fishes: The search for patterns.
Parasitology 136:1653–1662.
King, S.D. 2009. Ecology and taxonomy of ectoparasites infecting sympatric Fundulus
heteroclitus, F. diaphanus, and their asexual hybrid in two Nova Scotian lakes. M.Sc.
Thesis. Saint Mary’s University, Halifax, NS, Canada. 124 pp.
King, S.D., and D.K. Cone. 2009. Morphological and molecular taxonomy of a new species
of Fundulotrema and comments on Gyrodactylus stephanus (Monogenea: Gyrodactylidae)
from Fundulus heteroclitus (Actinopterygii: Cyprinodontiformes) in Nova Scotia,
Canada. Journal of Parasitology 95:846–849.
Krabbenhoft, T.J., M.L. Collyer, and J.M. Quattro. 2009a. Differing evolutionary patterns
underlie convergence on elongate morphology in endemic fishes of Lake Waccamaw,
North Carolina. Biological Journal of the Linnean Society 98:636–645.
Krabbenhoft, T.J., F.C. Rohde, and J.M. Quattro. 2009b. Threatened fishes of the world:
Fundulus waccamensis (Hubbs and Raney, 1946) (Fundulidae). Environmental Biology
of Fishes 84:173–174.
Kritsky, D.C., P.D. Leiby, and R.J. Kayton. 1978. A rapid stain technique for the haptoral
bars of Gyrodactylus species (Monogenea). Journal of Parasitology 64:172–174.
Southeastern Naturalist
211
E.J. Burge and S.D. King
2015 Vol. 14, No. 1
Kuris, A.M., R.F. Hechinger, J.C. Shaw, K.L. Whitney, L. Aguirre-Macedo, C.A. Boch, A.P.
Dobson, E.J. Dunham, B.L. Fredensborg, T.C. Huspeni, J. Lorda, L. Mababa, F.T. Mancini,
A.B. Mora, M. Pickering, N.L. Talhouk, M.E. Torchin, and K.D. Lafferty. 2008.
Ecosystem energetic implications of parasite and free-living biomass in three estuaries.
Nature 454:515–518.
Lafferty, K.D. 2008. Ecosystem consequences of fish parasites. Journal of Fish Biology
73:2083–2093.
Lafferty, K.D., and A.M. Kuris. 2009. Parasites reduce food-web robustness because they
are sensitive to secondary extinction as illustrated by an invasive estuarine snail. Philosophical
Transactions of the Royal Society B: Biological Sciences 364:1659–1663.
Lafferty, K.D., A.P. Dobson, and A.M. Kuris. 2006. Parasites dominate food-web links.
Proceedings of the National Academy of Sciences 103:11,211–11,216.
LeGrand, H.E., Jr., J.T. Finnegan, S.P. Hall, A.J. Leslie, and J.A. Ratcliffe. 2012. Natural
Heritage Program list of the rare animal species of North Carolina 2012, Revised 25
March 2013. North Carolina Natural Heritage Program, Office of Conservation, Planning,
and Community Affairs, NC Department of Environment and Natural Resources
Raleigh, NC. 160 pp.
Lindquist, D.G., and C.G. Yarbrough. 1982. Status of the endemic ichthyofauna of Lake
Waccamaw, North Carolina. North Carolina Wildlife Resources Commission. 108 pp.
Malmberg, G. 1970. The excretory systems and the marginal hooks as a basis for the systematics
of Gyrodactylus (Trematoda, Monogenea). Arkiv för Zoologi 23:1–235.
McCallum, H., and A. Dobson. 1995. Detecting disease and parasite threats to endangered
species and ecosystems. Trends in Ecology and Evolution 10:190–194.
Moser, M.L., F.C. Rohde, R.G. Arndt, and K.W. Ashley. 1998. Occurrence of the Brook
Silverside, Labidesthes sicculus (Atheriniformes:Atherinidae), in North Carolina. Brimleyana
25:135–139.
Porter, H.J. 1985. Rare and endangered fauna of Lake Waccamaw, North Carolina, watershed
system: Molluscan census and ecological interrelationships. North Carolina Wildlife
Resources Commission, Raleigh, NC. 187 pp.
Porter, H.J., and K.J. Horn. 1980. Freshwater-mussel glochidia from Lake Waccamaw,
Columbus County, North Carolina. Bulletin of the American Malacological Union
1980:13–17.
Poulin, R. 1996. Sexual inequalities in helminth infections: A cost of being a male? American
Naturalist 147:287–295.
Poulin, R. 2000. Variation in the intraspecific relationship between fish length and intensity
of parasitic infection: Biological and statistical causes. Journal of Fish Biology
56:123–137.
Poulin, R. 2007a. Are there general laws in parasite ecology? Parasitology 134:76 3–776.
Poulin, R. 2007b. Evolutionary Ecology of Parasites. Princeton University Press, Princeton,
NJ. 342 pp.
Quattro, J.M., W.J. Jones, and F.C. Rohde. 2001. Evolutionarily significant units of rare
pygmy sunfishes (Genus Elassoma). Copeia 2001:514–520.
Reyes-Valdez, C.A., G. Ruiz-Campos, F. Camarena-Rosales, J.L. Castro-Aguirre, and G.
Bernardi. 2011. Population morphometric variation of the endemic freshwater killifish,
Fundulus lima (Teleostei: Fundulidae), and its coastal relative F. parvipinnis from the
Baja California Peninsula, Mexico. Reviews in Fish Biology and Fisheries 21:543–558.
Rohde, F.C., and R.G. Arndt. 1987. Two new species of pygmy sunfishes (Elassomatidae,
Elassoma) from the Carolinas. Proceedings of the Academy of Natural Sciences of
Philadelphia 139:65–85.
Southeastern Naturalist
E.J. Burge and S.D. King
2015 Vol. 14, No. 1
212
Rohde, F.C., R.G. Arndt, J.W. Foltz, and J.M. Quattro. 2009. Freshwater Fishes of South
Carolina. University of South Carolina Press, Columbia, SC. 430 pp.
Rohde, K. 1993. Ecology of Marine Parasites: An Introduction to Marine Parasitology.
CAB International, Wallingford, UK. xiv + 298 pp.
Rózsa, L., J. Reiczigel, and G. Majoros. 2000. Quantifying parasites in samples of hosts.
Journal of Parasitology 86:228–232.
Ruiz, C.F. 2013. Parasite-component community of Gulf Killifish, Fundulus grandis, in an
oiled Louisiana saltmarsh. M.Sc. Thesis. Auburn University, Auburn, AL. 170 pp.
Schaefer, J., B.R. Kreiser, C. Champagne, P.M. Mickle, and D.D. Duvernell. 2009. Patterns
of co-existence and hybridisation between narrowly endemic (Fundulus euryzonus) and
broadly distributed (F. olivaceus) topminnows in a riverine contact zone. Ecology of
Freshwater Fish 18:360–368.
Scott, M.E. 1982. Reproductive potential of Gyrodactylus bullatarudis (Monogenea) on
Guppies (Poecilia reticulata). Parasitology 85:217–236.
Sharitz, R.R. 2003. Carolina bay wetlands: Unique habitats of the southeastern United
States. Wetlands 23:550–562.
Shute, J.R., P.W. Shute, and D.G. Lindquist. 1981. Fishes of the Waccamaw River drainage.
Brimleyana 6:1–24.
Shute, J.R., P.L. Rakes, J.T. Baxter, and P.W. Shute. 2000. Survey of Lake Waccamaw and
the Waccamaw watershed with emphasis on imperiled fishes. Conservation Fisheries,
Inc., for US Fish and Wildlife Service, Asheville Field Office, Knoxville, TN. 35 pp.
Shute, P.W., D.G. Lindquist, and J.R. Shute. 1983. Breeding behavior and early life history
of the Waccamaw Killifish, Fundulus waccamensis. Environmental Biology of Fishes
8:293–300.
Stager, J.C., and L.B. Cahoon. 1987. The age and trophic history of Lake Waccamaw, North
Carolina. Journal of the Elisha Mitchell Scientific Society 103: 1–13.
Sukhdeo, M.V. 2012. Where are the parasites in food webs? Parasites and Vectors 5:239.
Tracy, B.H., W.C. Starnes, and F.C. Rohde. 2013. North Carolina’s imperiled fish fauna,
part XIII: “Lake Phelps” Killifish, Fundulus sp. cf. diaphanus. North Carolina Chapter
of the American Fisheries Society Newsletter Winter 2013/2014:7–11.
US Fish and Wildlife Service (USFWS). 1987. Endangered and threatened wildlife and
plants: Determination of threatened status and critical habitat for the Waccamaw Silverside.
Final Rule. Federal Register 52:11,277–11,286.
Wiles, M. 1975. Parasites of Fundulus diaphanus (LeSueur) (Pisces: Cyprinodontidae) in
certain Nova Scotian freshwaters. Canadian Journal of Zoology 5 3:1578–1580.
Wilson, K., O.N. Bjørnstad, A.P. Dobson, S. Merler, G. Poglayen, S.E. Randolph, A.F.
Read, and A. Skorping. 2002. Heterogeneities in macroparasite infections: Patterns and
processes. Pp. 6–44, In P.J. Hudson, A. Rizzoli, B.T. Grenfell, H. Heesterbeek and A.P.
Dobson (Eds.). The Ecology of Wildlife Diseases. Oxford University Press, Cary, NC.
240 pp.
Ziętara, M.S., and J. Lumme. 2002. Speciation by host switch and adpative radiation
in a fish-parasite genus Gyrodactylus (Monogenea, Gyrodactylidae). Evolution
56:2445–2458.
Ziętara, M.S., and J. Lumme. 2003. The crossroads of molecular, typological, and biological
species concepts: Two new species of Gyrodactylus Nordmann, 1832 (Monogenea:
Gyrodactylidae). Systematic Parasitology 55:39–52.