Chemoecology (2011) 21:131–141
DOI 10.1007/s00049-011-0075-5
CHEMOECOLOGY
RESEARCH PAPER
Chemical defense in pelagic octopus paralarvae: Tetrodotoxin
alone does not protect individual paralarvae of the greater
blue-ringed octopus (Hapalochlaena lunulata) from common
reef predators
Becky L. Williams • Vanessa Lovenburg
Christine L. Huffard • Roy L. Caldwell
•
Received: 24 February 2011 / Accepted: 1 April 2011 / Published online: 14 April 2011
Ó Springer Basel AG 2011
Abstract Some pelagic marine larvae possess anti-predator chemical defenses. Occasionally, toxic adults imbue
their young with their own defensive cocktails. We examined paralarvae of the greater blue-ringed octopus
(Hapalochlaena lunulata) for the deadly neurotoxin tetrodotoxin (TTX), and if present, whether TTX conferred
protection to individual paralarvae. Paralarvae of H. lunulata possessed 150 ± 17 ng TTX each. These paralarvae
appeared distasteful to a variety of fish and stomatopod
predators, yet food items spiked with 200 ng TTX were
readily consumed by predators. We conclude that TTX alone
does not confer individual protection to paralarvae of
H. lunulata, and that they possess an alternative defense. In
larger doses, tetrodotoxin is a deterrent to the predatory
stomatopod Haptosquilla trispinosa (mean dose = 3.97
lg/g). This corresponds to 12–13 paralarvae per predator
based on the TTX levels of the clutch we examined. Thus,
the basic assumption that individual paralarvae of H. lunulata are defended by TTX alone was disproved. Instead,
functionality of TTX levels in paralarvae may arise through
alternative selective pathways, such as deterrence to
B. L. Williams (&)
Department of Biology, MSC 3AF,
New Mexico State University, P.O. Box 30001,
Las Cruces, NM 88003-8001, USA
e-mail: toxwilliams@gmail.com
V. Lovenburg R. L. Caldwell
Department of Integrative Biology, University of California,
Berkeley, 3060 Valley Life Science Bldg #3140,
Berkeley, CA 94720-3140, USA
C. L. Huffard
Conservation International Indonesia, 17 Jalan Dr. Muwardi,
Denpasar, Bali, Indonesia
parasites, through kin selection, or against predator species
not tested here.
Keywords Chemical defense Cephalopod
blue-ringed octopus Hapalochlaena lunulata
Palatability Tetrodotoxin Paralarvae Pelagic larvae
Introduction
Planktivorous predators in the nekton have shaped the
evolution of anti-predator defenses including morphologies
that are difficult to ingest (e.g. spines in crab zoeae;
Morgan 1989), transparency that serves as crypsis (e.g.
Johnson 2001), and chemical defenses including unpalatability (e.g. Lindquist and Hay 1996; Lindquist et al. 1992;
McClintock and Vernon 1990; Young and Bingham 1987).
Cephalopods comprise a diverse lineage of benthic and
midwater adults and paralarvae alike, with a diverse repertoire of anti-predator defenses. Adults are integral prey to
seabirds, sharks, marine mammals, and teleosts (e.g. Jereb
et al. 2005), and this demonstrated widespread palatability
suggests that planktonic paralarvae may also be at high
risk of predation. Because of morphological constraints in
cephalopods, paralarvae especially may benefit from
chemical defenses.
Inking represents one such chemical defense by mollusks such as cephalopods (e.g. Derby 2007). For example,
tyrosinase, a cytotoxin present in the ink of several cephalopods, may irritate chemosensory receptors and thus
deter predators (Prota et al. 1981; Russo et al. 2003).
Paralarvae of many octopuses can expel ink upon hatching
and during their tenure in the water column (reviewed by
Villanueva and Norman 2008). Immature common blanket
octopuses (Tremoctopus violaceus), mid-water animals,
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possess a different and unusual example of chemical
defense in octopods; they harvest man-o-war (Physalia)
tentacles and present these armaments to predators in
defense (Jones 1963). While inking has received some
attention, and the co-opting of cnidarian defenses serves as
a unique example, little else is known about chemical
defenses in pelagic phase cephalopods.
Blue-ringed octopuses (Hapalochlaena spp.) represent a
well-known example of chemically defended benthic
cephalopods, some of which produce pelagic paralarvae.
Noxious larvae coincide with noxious adults among other
marine taxa surveyed for chemical defenses (Lindquist and
Hay 1996). Adult blue-ringed octopuses harbor tetrodotoxin (TTX; Sheumack et al. 1978), which appears to be
produced by symbiotic bacteria (Hwang et al. 1989). This
deadly neurotoxin shuts down action potentials in nerve
and muscle tissue by blocking sodium channel pores (e.g.
Narahasi 2001). This toxicity hypothetically supplants
inking as a chemical defense in this genus. Ink sacs in
adult blue-rings atrophy (Robson 1929), though adults of
H. lunulata and two undescribed congeners can still expel
ink (Huffard and Caldwell 2002; Norman 2000). The
benthic hatchlings of H. fasciata ink only at ages 1.5–4.5
wks (Tranter and Augustine 1973); newly hatched pelagic
paralarvae of H. lunulata also expel minute amounts of ink
(pers. obs.). However, these young octopuses ink infrequently and may depend instead on TTX as a chemical
defense. Sheumack et al. (1984) identified TTX in the eggs
of one species of blue-ringed octopus (probably H. fasciata
based on the authors’ locality). Whether TTX defends early
life stages from predators is unknown.
Additionally, chemical defenses can be costly as they
are in aspens and wild parsnip (Zangerl and Berenbaum
1997; Häikiö et al. 2009). In these taxa tradeoffs exist
between defense and growth and reproduction. Bullard
et al. (1999) empirically observed that many pelagic larvae
are chemically undefended. No young of any blue-ringed
octopus have yet been examined for the presence of TTX
or other evidence of chemical protection.
Despite the efficacy against vertebrate neurosystems
(e.g. Narahasi 2001) and the presence of the toxin in many
unrelated and widespread taxa (reviewed by Noguchi and
Arakawa 2008), the ecological function of TTX has rarely
been tested empirically (Williams 2010). In newts, TTX
appears to be an effective defense against avian, fish, and
snake predators (Brodie 1968; Mobley and Stidham 2000;
Mochida 2009; Williams et al. 2010). Although TTX is
common amongst pufferfish (e.g. Noguchi and Arakawa
2008), and some freshwater fish gustatory neurons respond
to TTX (Yamamori et al. 1987), empirical data on the
realized anitpredator efficacy is lacking. Conversely,
although originally thought to be a defense (Miyazawa
et al. 1987), TTX is used as venom in a polyclad worm
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B. L. Williams et al.
(Ritson-Williams et al. 2006). Here we test whether the
pelagic paralarvae of H. lunulata contain TTX and, if so,
whether TTX protects the paralarvae from predation by
common reef predators.
Materials and methods
Sampling
We obtained 30 adult Hapalochlaena lunulata, shipped
from Bali, Indonesia, through the tropical aquarium
industry between June 2004 and November 2006. Octopuses were wild-caught at our request and, according to the
importer, were in transit no more than 1 week. We also
obtained five male and two female adult Octopus cf.
mercatoris via the pet trade from Florida, USA; these small
octopuses occupy similar habitat but provided a non-TTX
bearing control. Adult octopuses were housed in 38 l
aquaria at 25°C. Hatchlings and paralarvae were housed
individually in 0.5 l cups with approximately 150 ml artificial seawater (ASW) mixed at 34 ppt (Aqua Craft, Inc.).
Every third day adult octopuses were fed live grass shrimp,
ghost shrimp, snails, brine shrimp, or thawed prawn or fish
pieces as availability permitted.
Males were introduced into home aquaria of females for
mating (see Cheng and Caldwell 2000 for a detailed
description of mating). Out of 14 introductions of H. lunulata, seven matings were completed. Two female
H. lunulata (one unmated at our facilities) deposited eggs.
These females were offered food approximately twice
weekly, but stopped feeding during brooding and expired
soon after eggs hatched as previously observed in semelparous octopuses (i.e. H. lunulata and H. maculosa, Overath
and von Boletzky 1974; Tranter and Augustine 1973). The
eggs of the unmated female did not develop. The other
female (mated three times) yielded a fertile clutch of *260
paralarvae, which hatched after 32–34 days. Approximately
100 paralarvae hatched synchronously in the early morning
on the second and third days. Newly hatched paralarvae
were *2–3 mm in length. Both control O. cf. mercatoris
females laid fertile eggs within one week of arrival and
hatchlings emerged 23–24 days hence at 5–6 mm in length.
Twelve H. lunulata paralarvae and two O. cf. mercatoris
hatchlings were immediately frozen at -80°C for later
toxicity analyses. The remaining animals were reserved for
behavioral trials (below).
Representative stomatopod predators (Haptosquilla trispinosa) were collected from Lizard Island, Queensland
Australia in 2005 and 2007. The stomatopods were housed
at UC Berkeley, California, USA in plastic cups (*150 ml
of 32 ppt ASW in 0.5 l cups), and kept under 14:10
light:dark conditions at 25°C. The water was changed twice
Chemical defense in pelagic octopus paralarvae
133
weekly. Various species of larger stomatopods, which were
wild-caught or obtained via the pet trade for other projects
during the previous 5 years, were housed at UC Berkeley
in larger cups (*300 ml ASW in 1 l cups) or individual
aquaria (38 l). Smaller stomatopods were fed twice weekly
with 10–20 live brine shrimp or an equivalent amount of
frozen brine shrimp or frozen Mysis shrimp as supply
permitted. Larger stomatopods were fed thawed shrimp or
fish, or freeze-dried krill.
Fish predators were housed at the Octopus’ Garden pet
store in Berkeley, California, USA. This retail marine
aquarium store provided a high diversity of tropical reef
fish, many of which occur sympatrically with Hapalochlaena and may be natural predators of octopus
paralarvae. Fish were housed in 5 l aquaria.
after mixing. A water jacket cooled the derivatization
products before detection by a Jasco FP-1512 (or Dynamax
model FL-2) fluorescence detector with excitation wavelength set at 365 nm and emission wavelength at 510 nm.
The Beckman System Gold Software (or a Hewlitt Packard
3390A Integrator) recorded the chromatographs and calculated peak areas. Tetrodotoxin peaks in tissue samples
were identified and quantified by comparison with a standard of 1.0 lg/ml TTX in 0.10 N acetic acid (or 2.5 lg/ml
TTX in 0.05 N acetic acid depending on the sensitivity of
the HPLC system used). Paralarvae of H. lunulata were
compared with the hatchlings of O. cf. mercatoris (which
do not contain TTX) as a control. We used a peak skimming formula to conservatively calculate peak areas where
the TTX peak eluted on top of a broad band.
Tetrodotoxin extraction and quantification
Antipredator efficacy of TTX
Tetrodotoxin was extracted from samples by modifying the
methods of Hanifin et al. (1999). We extracted TTX from
paralarvae by grinding in the microcentrifuge tube with a
plastic pestle or via sonication at level 3 in 100 ll of
0.05 N acetic acid. Food samples spiked with TTX (see
Experiments 2–4 below) and O. cf. mercatoris hatchlings
were extracted individually in the same manner. Extracts
were heated to 100°C in boiling water for 5 min before
cooling in an ice bath. The extracts were then centrifuged
at 13,000 rpm for 15 min, the supernatant collected, and
the supernatant was filtered through 5,000 nominal
molecular weight limit (NMWL) 0.5 ml Ultrafree-MC
Millipore tubes by centrifugation at 13,000 rpm for
20 min. Filtrates were stored at -80°C until quantification.
We quantified TTX in sample extracts using 20 ll aliquots on two different reverse phase high performance
liquid chromatography (HPLC) systems by modifying the
procedures of Yotsu et al. (1989), and Hanifin et al. (1999)
to optimize peak separation and quantification for each
system. Data sets used for statistical analyses were collected on one system or the other; samples were not split
between both. Samples were eluted with either an isocratic
gradient of 1.0% (or 3.0%) by volume acetonitrile, 1.28%
(or 0.97%) by weight heptafluorobutyric acid, and 0.29%
by volume acetic acid. Each mobile phase was adjusted to
pH 5.0 with 50% NH4OH. We separated analytes with a
Synergi 4 lm Hydro-RP 80A C18 column (250 9 4.6 mm,
Phenomenex, USA) on both systems. A Beckman Coulter
System Gold 126 Solvent Module provided a primary flow
rate of 0.5 ml per min for the mobile phase and a secondary
flow rate of 1.0 ml per min of 5 N sodium hydroxide for
mixing post-column (or a Shimadzu LC-10ADvp module
and a Beckman 110A for the primary [0.5 ml/min] and
secondary [0.9 ml/min] flow rates, respectively). A Pickering CRX 400 reactor heated elutants to 115°C (or 130°C)
Fish and stomatopod predators were offered treatment and
control food items in each of five experiments. Experiments
were not conducted concurrently; individual predators are
not necessarily the same between experiments. No individual predator was used more than once per experiment.
‘‘Injections’’ of treatment or control solution were carefully
made under a dissecting microscope on a paper towel to
ensure no solution leaked from the food items before presentation to the predators. Dry food items absorbed the TTX
or control solutions coated on the outside and were rehydrated. Mysis were injected in between the carapace and first
body segment; any applied pressure (i.e., handling by the
predator) consequently released the body cavity contents. As
an additional control, food items injected with treatment
solution were dipped in water, to simulate the time a food
item was in the water during behavioral trials, and then
extracted to quantify TTX via HPLC. The ‘‘injection’’ procedure and HPLC assay verified that injected solutions did
not diffuse from food items before predators accepted them
and that TTX was accessible to the predator as the food item
was sampled. Food items were introduced into home aquaria
or cups that were occupied by a single predator. We randomized the order of control or treatment food items.
We recorded whether treatment and control items were
taken into the predator maw (sampled), and whether they
were eaten if sampled. Any organism possesses a suite of
defenses, including behavioral, morphological, and chemical. Because we were interested in the ‘‘last line of
defense’’ chemical defenses, we focused on the interaction
of predators and prey beginning when the predator physically contacted the prey item (sampling). If the item was
sampled the two possible outcomes were ‘Eaten’ or
‘Rejected.’ ‘Eaten’ literally meant that the food item was
consumed and was not ejected at any later time. ‘Rejected’
was recorded when the item was sampled but then ejected/
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B. L. Williams et al.
discarded. Trials were discarded in the following instances:
on the uncommon occurrence (29 in all experiments) that
items were repeatedly mouthed and rejected prior to
ingestion because TTX may have been dispelled from the
food item; if the predator did not appear to see the food
item within 5 s to control for possible diffusion of TTX
away from the food item; and if the predator did not sample
both treatment food items and controls we assumed they
were not hungry (if they sampled both we assumed they
were hungry even if both items were rejected and scored
this data). If the food item was investigated but not sampled by stomatopods, we recorded ‘Rejected.’ For example,
stomatopods may approach, investigate with antennae or
antennules, and may or may not strike at the food item
without taking it in toward the mouth parts before disregarding the item. This is akin to sampling in other
predators and is a typical mode of ‘‘smelling’’ for stomatopods. Regardless of whether stomatopods rejected
Table 1 Results of Experiment
1: blue-ringed octopus
paralarvae palatability
experiment
paralarvae by ‘‘smelling’’ or ‘‘tasting,’’ the paralarvae can
still be considered ‘‘rejected.’’ Predators that ingested a
food item containing TTX were observed for intoxication
or any ill effects for approximately 60 min and then again
24 h after the experiment.
Experiment 1
We tested palatability of paralarvae in the first experiment
with potential octopus predators both sympatric and allopatric to H. lunulata. Paralarval H. lunulata (2.5 mm
length 9 1.5 mm diameter) between one and two days
after emerging from their egg cases were offered to fish (13
species, N = 13) and stomatopod (5 species, N = 17)
predators (Table 1). Live brine shrimp were offered to
predators as controls because of their similar size and
movement compared to paralarvae and because they were
available at the time paralarvae hatched.
Scientific name
Common name
PS
Paralarvae
Brine Shrimp
Acanthurus triostegus
Amblygobius rainfordi
Convict tang
Old glory
Y
Y
R
R
E
E
Amphiprion ocellaris
Clown anenomefish
Y
R
E
Centropyge aurantonotus
Flameback anglefish
N
R
E
Centropyge flavicauda
Whitetail pygmy anglefish
Y
R
E
Cirrhilabrus rubriventralis
Social wrasse
N
R
E
Dendrochirus brachypterus?
Dwarf lionfish
Y
R
E
Gonodactylus chiragra
Mantis shrimp
N
R
E
Gonodactyaceus falcatus
Mantis shrimp
Y
R
E
Gonodactyaceus falcatus
Mantis shrimp
Y
E
E
Gonodactyaceus falcatus
Mantis shrimp
Y
R
E
Gonodactyaceus falcatus
Mantis shrimp
Y
R
R
Gonodactyaceus falcatus
Mantis shrimp
Y
R
E
Gonodactyaceus falcatus
Mantis shrimp
Y
R
E
Gonodactyaceus falcatus
Mantis shrimp
Y
R
E
Gonodactyaceus falcatus
Lienardella fasciata
Mantis shrimp
Harlequin tusk wrasse
Y
Y
R
E
E
E
Odonodactylus havanensis
Mantis shrimp
N
E
E
Odonodactylus havanensis
Mantis shrimp
N
R
R
Odonodactylus havanensis
Mantis shrimp
N
R
E
Odonodactylus havanensis
Mantis shrimp
N
R
E
Odonodactylus havanensis
Mantis shrimp
N
R
E
Paralarvae of Hapalochlaena
lunulata and brine shrimp
controls were offered to
predators. Predators rejected H.
lunulata paralarvae more often
than brine shrimp controls
Odonodactylus scyllarus
Peacock mantis shrimp
Y
E
E
Paraglyphidodon nigroris
Black-and-gold chromi
Y
R
E
Pseudochromis diadema
Diadem dottyback
Y
R
E
Pseudochromis paccagnellae
Royal dottyback
Y
R
E
Raoulserenea pygmaea
Mantis shrimp
N
R
E
PS possible sympatry, E eaten,
R rejected
Raoulserenea pygmaea
Mantis shrimp
N
E
E
v2 = 16.03, df = 1, N = 30,
P \ 0.001
Salarius sp.
Blenny
?
R
E
Unknown
Wrasse (yellow)
?
R
E
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Chemical defense in pelagic octopus paralarvae
Experiment 2
with either 200 ng TTX (2 ll of a 0.1 mg/ml solution in
ASW with 0.01 N acetic acid) or control ASW (Table 3).
In Experiment 2 we tested the antipredator efficacy of TTX
against a large diversity of predators. Fish and stomatopod predators were offered dry food items (11 mm
length 9 2 mm diameter) injected with either 200 ng TTX
(5 ll of a 0.04 mg/ml solution in ringer solution) based on
the average amount of TTX measured by HPLC in
H. lunulata paralarvae (see ‘‘Results’’ section) or a control
injection of 5 ll Ringer’s solution (Table 2). Fish (8 species, N = 9) were given floating tropical food pellets while
stomatopods (9 species, N = 15) were offered pieces of
freeze dried krill, typical food items for these captive
animals. However, unknown constituents in these food
items interfered with accurate quantification of TTX in
samples by HPLC (see ‘‘Results’’ section).
Experiment 3
Experiment 3 confirmed the results of Experiment 2 with a
subset of predators offered another food item that did not
interfere with TTX quantification. In this experiment,
stomatopods (8 species, N = 23) were offered Mysis
shrimp (6 mm length 9 1 mm diam.) that were injected
Table 2 Results of Experiment
2: dried food palatability
experiment
135
Experiment 4
In Experiment 4 we opportunistically tested another nonTTX bearing cephalopod as the food item. During Experiment 4 we offered predators a small set of benthic Octopus
cf. mercatoris hatchlings. Sixteen hatchlings were injected
with either 200 ng TTX (5 ll of a 0.04 mg/ml solution in
Ringer’s solution) or a control injection of 5 ll Ringer’s
solution. We offered one spiked and one control hatchling
to each of four species of fish and four species of stomatopods (N = 8).
Experiment 5
In the fifth experiment we offered multiple food items
spiked with TTX to in a single population sample of stomatopods (Haptosquilla trispinosa from Queensland,
Australia) to test the possibility that greater quantities of
TTX than found in paralarvae may be deterrent. Tetrodotoxin (1 mg) was dissolved in 1 ml of 0.05 N acetic acid in
ASW, then diluted by half in ASW. Mysis shrimp were
Scientific name
Common name
PS
Spiked food
Control
Balistapus undulatus
Undulated triggerfish
Y
E
E
Balistoides conspicillum
Clown triggerfish
Y
E
E
Ctenochaetus tominiensis
Tomini tang
Y
E
E
Gonodactylus chiragra
Mantis shrimp
N
R
E
Gonodactylus chiragra
Mantis shrimp
N
E
E
Gonodactylus chiragra
Mantis shrimp
N
R
R
Gonodactyaceus falcatus
Mantis shrimp
Y
R
R
Haptosquilla stoliura
Mantis shrimp
Y
R
E
Haptosquilla stoliura
Mantis shrimp
Y
R
E
Lysiosquillina maculata
Odonodactylus brevirostris
Mantis shrimp
Mantis shrimp
Y
N
E
E
E
E
Odonodactylus havenensis
Mantis shrimp
N
E
E
Odonodactylus havenensis
Mantis shrimp
N
E
E
Odonodactylus havenensis
Mantis shrimp
N
R
R
Odonodactylus latirostris
Mantis shrimp
Y
R
E
Odonodactylus scyllarus
Peacock mantis shrimp
Y
E
E
Odonodactylus scyllarus
Peacock mantis shrimp
Y
E
E
Plepidogenys?
Damsel
?
E
E
Pseudochromis splendens
Splendid dottyback
Y
E
E
Pseudosquilla ciliata
False mantis/rainbow mantis
Y
E
E
Rhinecanthus aculeatus
Picasso triggerfish
Y
E
E
PS possible sympatry, E eaten,
R rejected
Siganus puellus
Blue line rabbitfish
Y
E
E
v2 = 0.421, df = 1, N = 24,
P = 0.516
Siganus puellus
Blue line rabbitfish
Y
E
E
Yongeichthys nebulosus
Shadow goby
Y
E
E
We injected commercial food
items (dried krill and tropical
fish food pellets) with either
200 ng TTX or ringer solution
as a control. Predators did not
discriminate between innocuous
food items and those spiked
with TTX
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136
Table 3 Results of Experiment
3: Mysis shrimp palatability
experiment
B. L. Williams et al.
Scientific name
Common name
PS
Spiked Mysis
Control
Acanthosquilla multifasciata
Mantis shrimp
Y
R
R
Acanthosquilla multifasciata
Mantis shrimp
Y
E
E
Acanthosquilla multifasciata
Mantis shrimp
Y
E
E
Gonodactylellus caldwelli
Blue-lined mantis shrimp
Y
R
R
Gonodactylus chiragra
Mantis shrimp
N
E
E
Gonodactylus chiragra
Mantis shrimp
N
E
R
Gonodactylus smithii
Purple spotted mantis shrimp
Y
E
E
Gonodactylus smithii
Purple spotted mantis shrimp
Y
E
E
Haptosquilla stoliura
Mantis shrimp
Y
E
E
Haptosquilla stoliura
Mantis shrimp
Y
E
E
Haptosquilla stoliura
Mantis shrimp
Y
R
R
Haptosquilla stoliura
Mantis shrimp
Y
E
E
Haptosquilla trispinosa
Mantis shrimp
Y
E
R
Haptosquilla trispinosa
Mantis shrimp
Y
E
E
Haptosquilla trispinosa
Neogonodactylus curacaoensis
Mantis shrimp
Mantis shrimp
Y
N
R
R
E
R
Odontodactylus havenensis
Mantis shrimp
N
R
E
Odontodactylus havenensis
Mantis shrimp
N
E
E
Odontodactylus havenensis
Mantis shrimp
N
E
E
Odontodactylus scyllarus
Peacock mantis shrimp
Y
E
E
PS possible sympatry, E eaten,
R rejected
Odontodactylus scyllarus
Peacock mantis shrimp
Y
E
E
v2 = 0.000, df = 1, N = 23,
P = 1.00
Odontodactylus scyllarus
Peacock mantis shrimp
Y
E
E
Pseudosquilla ciliata
False mantis/rainbow mantis
Y
R
R
We injected Mysis shrimp with
either 200 ng TTX or artificial
seawater as a control. No
difference existed in the number
of spiked versus control Mysis
shrimp consumed
spiked with either 2 ll of 500 lg/ml TTX solution (1 lg
TTX injected in total) for the treatment group, or 2 ll of
0.025 N acetic acid in ASW as a control. Stomatopods of
approximately the same size class were chosen for the
experiment. Immediately after injections the Mysis shrimp
were presented to the stomatopods in their cups via small
forceps. The stomatopods were offered control or TTXspiked Mysis shrimp until rejection or until they accepted a
total of five.
Half of the stomatopods, chosen at random, were
tested with control Mysis and half with TTX-spiked
Mysis on the first day. On a different day, those that first
received controls received TTX-spiked Mysis and vice
versa. Stomatopods were typically fed twice a week.
Trials were conducted on a regular feeding day; all
experimental subjects were fed *15 Mysis shrimp as per
their normal feeding schedule at the conclusion of the
experiment.
Analyses
Tetrodotoxin was extracted and quantified in spiked food
samples and compared with unspiked samples to confirm the
validity of the spiking procedure. We tested whether food
items were rejected more often than controls in Experiments
1–3 with v2 goodness-of-fit tests (Tables 1, 2, 3). In order to
123
test whether dose (amount of TTX/size predator) varied
between experiments we compared size of predators
between experiments.
We estimated fish to the nearest cm and stomatopods to
the nearest 0.5 cm after feeding trials as we did not anesthetize predators and wished to reduce handling time. We
then assigned size classes to predators based on 2 cm gradations for the analyses to account for error of our estimates.
We used t-tests to evaluate whether predator size class
varied between the blue-ring paralarvae palatability
(Experiment 1) and each of the two spiked food palatability
experiments (dry food and Mysis shrimp; Experiments 2 and
3). Data from Experiment 4 (O. cf. mercatoris hatchlings)
were not analyzed because of the small sample size. In
Experiment 5 we compared the number of TTX-injected
Mysis shrimp eaten to the number of controls eaten with the
non-parametric Wilcoxon Sign-Rank test. Although we
chose predators of similar size for this experiment, we also
evaluated whether the number of TTX-spiked Mysis eaten
varied with predator size with ANOVA. For this analysis,
the number of TTX-spiked Mysis was transformed [log (#
eaten ? 1)] to approximate a normal distribution as
indicated by the Shapiro–Wilks Test. Untransformed stomatopod size did not differ from a normal distribution.
Analyses were performed with JMP version 7.0, copyright
2007 SAS Institute, Inc.
Chemical defense in pelagic octopus paralarvae
Results
The paralarvae of H. lunulata contained mean ± SE =
150 ± 17 ng TTX per parlarava (N = 11); no TTX was
found in the O. cf. mercatoris hatchlings examined
(Fig. 1). The lower detection limit of this HPLC was
*10 ng TTX.
Antipredator efficacy of TTX
137
dipped in water. Mysis shrimp presented no interfering
compounds to hamper the quantification of TTX in the
spiked samples. Estimated TTX quantity in two samples of
Mysis shrimp spiked with 200 ng TTX were 263 and
321 ng of TTX respectively. Because the amount we
injected into food items was near the lower detection limit,
variability of estimates was high. However, given that we
injected 200 ng TTX—approximately 33% above the mean
amount of TTX in paralarvae (150 ± 17 ng)—and anything under 100 ng was undetectable on this machine, we
Spiked food items such as dried krill, fish food pellets, or
Mysis shrimp, were compared to un-spiked samples of the
same food via HPLC. Tetrodotoxin peaks were visualized
in chromatographs of dried food items (krill and fish food
pellets); however, the presence of a co-eluting, unidentified
constituent interfered with highly accurate quantification of
the TTX peak (Fig. 2). Given that the limit of detection of
this HPLC was 100 ng and that the injected TTX was
visualized in spiked food samples, we could ascertain that
more than 100 ng of the 200 ng of TTX injected was
recovered from spiked food samples even after having been
Fig. 1 Chromatographs illustrating a recovery of tetrodotoxin (TTX)
in a paralarvae of Hapalochlaena lunulata, and b absence of TTX in
an Octopus cf. mercatoris hatchling
Fig. 2 Chromtographs illustrating recovery of tetrodotoxin (TTX) in
food items spiked with 200 ng of TTX, and absence of TTX in control
food items. A commercial standard of TTX is given for comparison.
The dotted line is an aid to visualize the retention time of TTX.
a Extract of dried krill. b Extract of dried krill spiked with TTX.
c Extract of Mysis shrimp. d Extract of Mysis shrimp spiked
with TTX
123
138
are confident that the amount of TTX in all spiked food
items equaled or exceeded the amount of TTX in
paralarvae.
Predators rejected H. lunulata paralarvae more often
than brine shrimp controls (Experiment 1; v2 = 16.03,
df = 1, N = 30, P \ 0.001; Table 1). Most paralarvae
sampled were rejected instantly. Only 5 of 30 predators ate
paralarvae. Neither predators that ate paralarvae nor those
that rejected paralarvae displayed any obvious signs of
TTX intoxication such as unsteadiness, paralysis, or
reduced ventilation rate (e.g. Kao 1966; Noguchi and
Ebesu 2001). All rejected paralarvae survived attempted
ingestion by predators.
Predators did not discriminate between spiked and
innocuous dry food items (Experiment 2; v2 = 0.421,
df = 1, N = 24, P = 0.516; Table 2). Similarly, no difference existed in the number of spiked (16/23) versus control
(16/23) Mysis shrimp consumed by predators (Experiment
3; v2 = 0.000, df = 1, N = 23, P = 1.00; Table 3). Predators also found O. cf. mercatoris hatchlings palatable
whether they were injected with TTX or Ringer’s solution
(Experiment 4; 7/8 hatchlings consumed in both treatments).
As in Experiment 1, no predators exhibited any signs of TTX
intoxication or ill effects after Experiments 2–4. The predator size classes for Experiment 1 involving the blue-ring
paralarvae (mean ± SD = 3.47 ± 1.07) and Experiment 2
involving dry food (3.66 ± 1.27) were not significantly
different (t = 0.614, df = 45, P = 0.542), but that for
Experiment 3 involving Mysis shrimp (2.65 ± 0.83) was
smaller (t = -3.11, df = 51, P = 0.003). Thus, predators
presented with TTX-spiked food items received an equal or
higher dose of TTX (dose incorporates mass of predator)
than predators exposed to TTX in paralarvae, yet still consumed spiked food items with impunity.
In Experiment 5 we searched for deterrence by TTX in a
sample of stomatopods from one population (Haptosquilla
trispinosa). More control Mysis shrimp (mean ± SD =
3.91 ± 1.36) were eaten than TTX-spiked Mysis (1.91 ±
1.45, Z = 21.50, n = 11, df = 11, P = 0.0127). Because
each Mysis shrimp was injected with 1 lg TTX these stomatopods consumed on average 1.9 lg of TTX before
rejection of the food items. Each paralarvae of H. lunulata
averaged *150 ng TTX in the clutch we examined. By
extrapolation, we estimated that stomatopods in our sample
group could have consumed approximately 12–13 of these
paralarvae before reaching a noxious dose of TTX. Although
TTX-spiked Mysis were rejected, we observed no obvious
signs of intoxication in the stomatopods. However, we did
not explicitly test intoxication; because TTX inhibits locomotor function (e.g. Brodie and Brodie 1999), swimming
speed or endurance may be a viable assay to test intoxication
of predators in future experiments. Because we chose stomatopods of roughly the same size, there was no correlation
123
B. L. Williams et al.
between predator mass and amount of TTX consumed in this
study (F(1,9) = 0.0507, P = 0.8269). While body size does
influence the effect of xenobiotics, there was not enough
variation in body size in our sample to discern this effect
here. Additionally, individual susceptibility to a toxin will
likely play a role but was not assessed in this study.
Discussion
Paralarvae of Hapalochlaena lunulata were unpalatable to
most predators. Although TTX is fast-acting and onset of
symptoms in humans and garter snakes occurs in as little as
1–15 min (Kao 1966; Williams et al. 2003), predators
rejected paralarvae of H. lunulata upon immediate contact
(\1 s)—faster than expected. Additionally, predators did
not find TTX-spiked food items distasteful and were not
intoxicated after consuming either paralarvae or TTXladen food items. Thus, a heretofore-unknown substance is
implicated in paralarval distastefulness. This substance
may or may not act in concert with TTX. A distasteful
compound need not directly harm a predator. It may
facilitate predator learning through multiple cues (e.g.
Fisher 1930; Nicolaus et al. 1983). In this scenario, the
compound signals the onset of more detrimental symptoms
of TTX. While it is theoretically possible the unknown
defense is not chemical, we favor this hypothesis because:
most young octopus are highly palatable; H. lunulata
paralarvae possess no unusual morphologies compared to
other cephalopods and do not display the aposematic blue
rings of adults; paralarvae were rejected only upon sampling by predators and this limits paralarval options for
behavioral defenses; and cephalopods in general are not
known for their morphological defenses (the beak is the
only hard part; Hanlon and Messenger 1996). It is clear,
however, that the quantity of TTX in individual paralarvae
was not deterrent to the predators tested here and an
alternative defense must exist.
Savage and Howden (1977) reported the presence of a
second toxic component called hapalotoxin in addition to
maculotoxin in H. fasciata adults (maculotoxin = TTX;
Sheumack et al. 1978). Hapalotoxin was deemed similar in
size to TTX, but exhibited some unique properties and thus
may have been an analog of TTX. Additional TTX analogs
are common in TTX bearing taxa, though few are as efficacious as TTX itself (Yasumoto and Yotsu-Yamashita
1996). Our analysis revealed no peaks in the HPLC profile
of H. lunulata paralarvae that suggested the presence of
additional TTX analogs (Fig. 1). Furthermore, to our
knowledge, none of the known analogs have been reported
as distasteful. Our extraction technique eliminated large
molecules over 5000 NMWL by filtration and smaller
peptides were likely denatured during the boiling process
Chemical defense in pelagic octopus paralarvae
and thus likely removed constituents other than TTX and
its analogs. Therefore, further work is required to identify
any additional defensive compound in paralarvae of
H. lunulata.
Although predators were not deterred by the amount of
TTX found in an individual paralarva, paralarval TTX may
provide benefit against certain predators, such as H. trispinosa, through kin selection. TTX in quantities larger
than those contained by individual paralarvae did deter
predators. Moths (Utetheisa ornatrix) endow their eggs
with a protective pyrolizidine alkaloid. Green lacewing
larvae (Ceraeochrysa cubana) sample the moths’ eggs
before consuming the whole clutch, destroying some eggs
in the process, but leaving the siblings intact when the
toxicity of the clutch exceeds the lacewing’s tolerance
(Eisner et al. 2000). In one sample of stomatopod predators, H. trispinosa, weighing on average 479 ? 34
(SE) mg, the lower level of deterrence was 1.9 lg of TTX.
This corresponds to approximately 12–13 paralarvae in the
clutch examined here. Blue-ring octopus paralarvae may
benefit from kin selection during egg development and
even immediately after hatching. Paralarvae of H. lunulata
hatch synchronously and diurnally (Overath and von
Boletzky 1974; this study) and the group may therefore be
subject to predation as they hatch and disperse into the
water column.
Even in the absence of kin selection, the level of TTX
seen in this study may still be functionally defensive. At
hatching the entire paralarvae possessed a concentration of
16.14 ± 4.84 lg TTX/g. Parasites of the paralarvae may
be negatively affected at this dose. Alternately, smaller
zooplankters, such as fish or crustacean larvae that might
prey upon octopuses in the water column, might be
intoxicated or even killed by the level of TTX in paralarvae
(*150 ng). Susceptibility to TTX varies by orders of
magnitude between taxa (e.g. Brodie 1968) and TTX may
be more effective against predators or parasites that were
not tested in this study. Thus, antipredator efficacy of TTX
(and any potential unknown distasteful substance, if discovered) should be tested in a variety of contexts.
Another reason that predators were not deterred by the
TTX levels found in the clutch examined could arguably be
that the concentration of TTX in this clutch was lower than
wild-hatched conspecifics or that TTX levels vary considerably among clutches. Animals that obtain chemical
defenses exogenously, such as poison dart frogs (e.g. Daly
et al. 1997), often lose toxicity in captivity. For example,
puffer fish exhibit very low or no TTX levels when raised in
captivity (e.g. Matsui et al. 1982; Matsumura 1996; Noguchi
et al. 2006; Saito et al. 1984). However, the TTX levels
found in adult H. lunulata from this area (Bali, Indonesia)
are comparable to levels found in other species of the
genus (Williams and Caldwell 2009; Yotsu-Yamashita et al.
139
2007). Also, TTX stores increase in developing embryos of
H. lunulata in captivity after eggs have been laid but before
hatching, suggesting that the mechanism of TTX production
remains intact (Williams et al. 2011). Finally, the TTX
levels in this clutch are comparable to those of other
developing embryos of H. lunulata before hatching
(Williams et al. 2011). Thus, we conclude that the TTX
levels in the clutch examined here are representative of
natural conditions.
Tetrodotoxin is present in paralarvae of H. lunulata.
This TTX is deterrent to predators, but only at amounts far
greater than those possessed by paralarvae. Even so,
paralarvae were rejected immediately. Predators rejected
83% of the paralarvae and all rejected paralarvae survived.
These results suggest the presence of an additional mechanism that confers protection to individual paralarvae of
H. lunulata. Further investigation is needed to clarify the
role of TTX, if any, and to discover the chemical identity
of any additional defensive compound(s) in paralarvae.
Acknowledgments The UC Berkeley ACUC authorized this
research (protocol #R302-0407). The Great Barrier Reef Marine Park
Authority provided a collecting permit to BLW and RLC for
Haptosquilla trispinosa (#G05/13381.1). Dr. Charles Hanifin at
Hopkins Marine Station, Stanford University, and Dr. Edmund
D. Brodie, Jr. at Utah State University provided assistance with HPLC
analyses. Stephanie Bush, Julie Himes, and Calida Martinez assisted
in the animal behavior lab and at Octopus’ Garden pet store in
Berkeley, CA. We would like to thank the owner of Octopus Gardens,
Erin Janoff, and an employee, Laith Shabbas, for their indispensable
help identifying fish and for logistical support. The manuscript benefited from comments by Dr. Akira Mori at Kyoto University, Maya
DeVries, Stephanie Bush, Joey Pakes, Jean Alupay, Dr. Dustin
Rubenstein, and Dr. David Lindberg at UC Berkeley, and Krista
Heideman, Dr. Jamie Howard, Anne Jacobs, and Anna Garliss at New
Mexico State University. Funding was provided by a Sigma Xi Grantin-Aid-of-Research and the Department of Integrative Biology, at UC
Berkeley.
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