Wildlife Society Bulletin; DOI: 10.1002/wsb.832
Tools and Technology
A Remote Marking Device and Newly
Developed Permanent Dyes for Wildlife
Research
PATRICIA BAIRD,1,2 Kahiltna Research Group, Department of Biological Sciences, California State University Long Beach, Long Beach, CA 90840,
USA
DAN ROBINETTE,3 Kahiltna Research Group, Department of Biological Sciences, California State University Long Beach, Long Beach, CA 90840,
USA
SCOT A. HINK,4 Kahiltna Research Group, Department of Biological Sciences, California State University Long Beach, Long Beach, CA 90840, USA
ABSTRACT Noninvasive, safe, quick marking of individual animals using distinctive colors that are highly
visible and persistent is a valuable methodology, but practical techniques and permanent safe dyes are lacking.
Here we describe a novel, remotely controlled dye machine to rapidly mark stationary animals in predictable
locations, such as birds sitting on nests on the ground or mammals at a den or burrow site. From the month of
June when birds were on eggs, using the machine, we spot-dyed 77 California least terns (Sternula antillarum
browni) at a colony in California, USA, in 4 days without handling them. Concomitantly, we developed a
suite of permanent (until molt or shedding), mainly phthalocyanine dyes that are incorporated chemically
into feathers or fur of animals and cannot be preened or rubbed off, which have never been used before to dye
animals. We found no toxicity of the dyes during in vivo testing over 1 month. This method of remote
marking with permanent dyes should prove to be a useful method in animal ecology for distinguishing among
individuals with minimal disturbance. Ó 2017 The Wildlife Society.
KEY WORDS California least tern, colonial waterbirds, color-marking, marking remotely, permanent dyes, Sternula
antillarum browni.
There are a handful of field techniques for marking
individual animals quickly, with minimal disturbance.
Methods to individually mark birds have included colored
leg bands in a unique pattern (Marion and Shamis 1977,
Baird 1992, Calvo and Furness 1992), colored leg streamers
or ptagial tags, and field-readable leg bands (e.g., Marion and
Shamis 1977, Lebreton et al. 2003, Nichols et al. 2004).
Marking methods for mammals have included tattooing
(e.g., Evans and Griffith 1973, Klimisch 1986, McGregor
and Jones 2016) and field-readable collars (Moorehouse and
Macdonald 2005). Researchers also have used other marking
methods to identify individual animals from a distance,
including coded radios or dyes, but usually the animals must
be trapped to affix the marks or devices.
Hands-off marking techniques would be particularly useful
on endangered species. In California, USA, the California
Received: 31 December 2015; Accepted: 6 June 2017
1
Present address: Simon Fraser University, Centre for Wildlife Ecology,
Burnaby, B.C., Canada V5A 1S6
2
E-mail: pab7@sfu.ca
3
Present address: Point Blue, Marine Ecology Division, Lompoc, CA
93436, USA
4
Present address: Pacific Biosciences, Menlo Park, CA 94025, USA
Baird et al.
Remote Dye Machine and Permanent Dyes
least tern (Sternula antillarum browni) is designated as
Endangered under the 1973 United States Endangered
Species Act (as amended; but see Draheim et al. 2010, 2012
for the endangered status). One of this species’ largest colonies,
distributed over 3 subcolonies, is in southern California at San
Diego Bay (Fig. 1). Our research on subcolony-specific
foraging behavior needed a long-lasting, highly visible marker
because of the difficulty of identifying bands or tags on terns at
a distance of >30 m from a survey boat, as well as discerning
tagged individuals via telemetry signals, often lost in
background electronic noise. We needed marks visible from
distance and lasting 2–3 months with no need to remark, and
subsequently chose to use dyes because they are an easy and
potentially noninvasive way to mark animals (Murray and
Fuller 2000) and have been used with varying success on
feathers (Marion and Shamis 1977, Calvo and Furness 1992,
Donehower and Bird 2005) or fur (Keith et al. 1968, Evans and
Griffith 1973, Twigg 1975).
We wanted to minimize human disturbance at the colony;
therefore, trapping with hands-on dyeing methods was
problematic given long handling times. Hands-on methods
used elsewhere include feeding dye to animals, broadcast
spraying of animals, and marking eggs or nests. These
methods have negative side effects such as toxicity, dyeing
nontarget species, or disturbing the colony. We reviewed
1
Figure 1. Map of the California least tern colonies where we tested dyes and dye-marking equipment in San Diego, California, USA, during 1993–2009. Image
source, Google Earth (Google, Inc., Mountain View, CA, USA).
indirect marking methods to find remote methods of dyeing
that satisfied conditions of speed, ease, lack of handling, and
nondisturbance to the colony (Marion and Shamis 1977,
Donehower and Bird 2005; summary of hands-off dyeing
methods in Text S1 and Table S1-1, available online in
Supporting Information).
One of us (S. A. Hink) developed a compact remote device
for dyeing with little colony disturbance, adequate range,
accurate aim (a 2–3-cm spot on the breast), and enough force
to dye >1 bird at a time. We describe this device, the “dye
machine,” as well as an experimental dye set developed for
longevity, visibility, and safety for use in the machine, which
we tested alongside our permitted (“conventional”) dyes for
visibility and longevity.
STUDY AREA
We studied California least terns breeding at 3 nesting areas
(subcolonies) at the San Diego, California, Naval Base
Coronado: North Island colony, Delta Beach colony, and
Ocean colony, 1993–1996, 2009 (Fig. 1). One nesting area
was in a developed area near a Navy airfield, lightly covered
with sand brought from nearby beaches, with low beach
vegetation. The second area was on a sand beach facing the
Pacific Ocean with sparse low-beach vegetation. The third
was an area facing San Diego Bay with packed soil and sparse
sand with patchy low-beach vegetation.
battery-operated squirt guns (Shout-N-Shoot Squirt Gun
Motor and Pump; Fig. 5). The transmitter sent a signal to
the radio-activated remote distribution unit filled with dye
that was attached to tubes buried in the sand leading to squirt
guns pointed at a nest (Fig. 6). A camouflaged tan bowl with
sand added to the freshly painted surface hid the squirt gun.
The entire system fit into a fishing tackle box (Fig. 7;
Table S1-2, Fig. S1-1, S1-2, S1-3).
Premarking technique.—Before using the dye machine, we
removed all tern eggs from the nest and placed them in a
covered bowl filled with bird seed as cushioning, kept in our
blind. Then we substituted water-filled speckled plastic eggs
resembling real tern eggs in appearance and weight. We
exchanged the eggs to prevent damage to the live eggs during
the dyeing operation.
We were permitted to use the basic dyes Malachite Green,
Methylene Blue, and Rhodamine B (red), and the acid dye
Picric Acid (yellow). We purchased all dyes from Sigma
Aldrich Corporation, St. Louis, Missouri, USA. We tested
these in the dye machine, and determined which 3 of the 4
METHODS
Remotely Controlled Dyeing Machine
Construction of dye machine.—We developed a remotely
controlled dye machine that could dye several birds at a time.
The remote control system (hereafter, RC; Fig. 2) consisted
of a transmitter that we disassembled (Airtronics AM
transmitter; Fig. 3), a remote distribution unit (Airtronics
AV2R receiver and Servo motor; Fig. 4), and up to 4
2
Figure 2. Remote control system of dye machine used to remotely mark
California least terns in San Diego, California, USA, during 1993–2009.
Wildlife Society Bulletin
9999()
Figure 5. Inside of squirt gun in dye machine used to remotely mark
California least terns in San Diego, California, USA, during 1993–2009.
Figure 3. Disassembled transmitter of dye machine used to remotely mark
California least terns in San Diego, California, USA, during 1993–2009.
dyes we would use for the 3 subcolonies. We only dyed adults
on eggs that were 7–19 days old (adults are least likely to
abandon after 7 days, and the earliest hatching time for eggs
was 19 days). Before setting up the equipment, we checked
the sites to ensure that we had no target nests with starred
eggs ready to hatch (starred eggs means that first visible
cracks have appeared).
Figure 4. Inside of remote distribution unit for dye machine used to
remotely mark California least terns in San Diego, California, USA, during
1993–2009.
Baird et al.
Remote Dye Machine and Permanent Dyes
Operation of the dye machine.—From the blind, we used
each transmitter control to send a signal to the receiver in the
RC distribution unit, move a switch on the squirt gun, turn
on the pump and motor, and squirt dye out the nozzle onto a
precise 3–4-cm patch on the bird’s breast from a distance of
10 cm (Fig. 8). We could operate up to 4 squirt gun units
from 1 RC distribution unit. We determined each bird’s
preferred incubation position for machine setup, and buried
the nozzle with the tip sticking up about 2 cm, and angled
slightly up, aimed at the location the bird would normally
face when sitting on the eggs. We used 8 dyeing machines at
a time. Each transmitter had 2 squirt gun units so that birds
on 2 nests could be dyed at a time. We assigned one of the 3
colors (Malachite Green, Rhodamine B, Methylene Blue) to
each colony, excluding picric acid because in a priori tests, it
was too light to be seen at distance. Each dye mixture was
saturated in 30% ethanol, and 1 mL Synthrapol or Calsolene
(Dharma Trading Compay, San Rafael, CA), for better
penetration (Baird et al. 1997). We dyed for 3–4-hr periods
to minimize disturbance and did not dye when temperatures
were >29.48 C or <128 C, or when the wind speed was
Beaufort >3.
We logged total time that each tern was off-nest from the
beginning of setup until its return to incubate on the nest.
We allowed each tern 30 min to return before we aborted the
session. Once the bird returned and sat facing the nozzle, we
Figure 6. Concealed squirt gun of dye machine at nest of California least
tern, next to tile shelter in San Diego, California, USA, during 1993–2009.
3
Figure 7. Complete dye machine and accompanying field equipment used
to remotely mark California least terns in San Diego, California, USA,
during 1993–2009.
fired the dye gun. After dyeing, we observed the tern in
flight, noting the visibility of the mark. We then retrieved the
equipment, checked the final condition of the nest site,
removed the plastic eggs, pulled up the nozzle and hose, filled
in any surface disturbance, and removed any excess dye from
overshoot. Once we restored the site, we replaced the live
eggs in the nest. We noted the time until the tern or its mate
returned and began incubating again.
Testing Conventional and Experimental Dyes In Vitro
In the a priori test we found that, of our permitted dyes,
Picric Acid did not wash off from feathers. The dyes that we
were permitted to use in the dye machine washed off, so we
researched other dyes similar in chemical structure to Picric
Acid that have been used on feathers for fly-tying, dyeing
cloth, and were known to resist fading when wet. However,
because high heat was needed to set them (Talleur 1999,
2010; D. Talleur, freelance author of fly-tying methods and
dyes, Clinton Corners, New York, USA, www.dicktalleur.
com, personal communication; P. Burch, hand dyeing
consultant, Houston, Texas, USA, www.paulaburch.net,
personal communication), they were not a suitable method
for live birds.
Subsequently, we reviewed dyes used by others, noting
species dyed, how dye was applied, dyes used, their visibility,
Figure 8. Characteristically dyed California least tern following use of a
remotely triggered dye machine in San Diego, California, USA, during
1993–2009.
4
longevity, and toxicity (Table S2, available online in
Supporting Information). All dyes had varying success,
methods of application varied, and species dyed were
diverse: bird species ranged from passerines to seabirds, and
mammals ranged from rabbits (Leporidae) to ground
squirrels (Sciuridae). Durability of dyes (how long they
remained the same color as when they were applied) and
their visibility from distances >30 m varied (New 1959,
Twigg 1975, Marion and Shamis 1977, Spencer 1978,
Savarie et al. 1992). Many of the dyes had solvents that were
combustible or toxic (e.g., nyanzol, silver nitrate, picric
acid), carcinogenic, or hazardous (e.g., nyanzol, Rhodamine
B), otherwise poisonous (e.g., aniline dyes, see Moffitt
1942), or which are systemic and may result in internal
marking of tissues (Evans and Griffith 1973, Paton and
Pank 1986). We rejected these dyes and sought to find dyes
similar in structure to Picric Acid, but that did not need
high heat to apply.
With the help of biochemists from Sigma-Aldrich
Corporation (Roubal 1997; T. Roubal, Sigma Aldrich,
Seattle, Washington, USA, personal communication), a
fishing fly-tying business (Talleur 1999, 2010; D. Talleur,
personal communication), and an independent textile dye
biochemist, (P. Burch, personal communication,), we found
26 other acid dyes or dyes with phthalocyanine, all of which
stain amino acids (Table 1). We call these dyes “experimental” because they have never been used to dye animals,
although 10 of the 26 are used in food, medicine, or
cosmetics.
We set up parallel in vitro tests for the 4 permitted
(“conventional”) dyes and 26 experimental dyes in a 2-month
test to select 3 dyes for the foraging study. The dyes had to
fulfill the following criteria: 1) able to be distinguished from
each other through time; 2) require just 1 application; 3) not
fade or run; 4) seen easily at a distance of >30 m; 5) last >2
months; 6) adhere to the feathers without having to hold
birds until dry; 7) retain their color and adhesiveness after
contact with seawater; and 8) nontoxic.
Assuming that dyed birds would bathe in the ocean before
the dye dried, we rinsed the feathers in seawater immediately
after marking. We used dyes in 30% ethanol because this
concentration proved best for longevity, brightness, and
visibility at distance (Baird et al. 1997). We made all
solutions with nonchlorinated, nonfluorinated distilled
water. In the 1997 pilot study, we discovered that adding
1 mL Synthrapol, a detergent and a surfactant, to each 100mL solution of dye gave better penetration of the feather.
Synthrapol solution, a detergent that helps suspend loose dye
particles and promotes the best penetration of dye, is used to
prescour natural fibers before dyeing, as well as to remove
excess dyes during the washing-out process postdyeing (P.
Burch, personal communication). The compound has a
neutral pH and is gentler on protein fibers (e.g., keratin in
feathers) than other detergents. We also found that
Calsolene had the same effect by promoting penetration
of the dye. This liquid wetting agent breaks the surface
tension of the water on the feather and increases the evenness
of dyeing, making feathers easier to dye. In our pretrials,
Wildlife Society Bulletin
9999()
Baird et al.
Table 1. List of all dyes tested to potentially remotely mark California least terns in San Diego, California, USA, during 1993–2009.a
Remote Dye Machine and Permanent Dyes
Common name
Color index name
Acid Orange 63
Acid Red 52
Amido Black 10B
Acid Orange 63
Acid Rhodamine B or Aizen
Food Red
Acid Black 1
C22H14N6Na2O9S2
Analine blue
Azo Eosin
Acid Red 4
C32H25N3O9S3Na2
C17H13N2NaO5S
Cobalt phthalocyanine
Molecular formula
C35H26N6Na2O10S3
C27H29N2NaO7S2
Other additives
50% acetic acid
50% acetic acid
10% acetic or citric
acid
C32H16CoN8
Coomasie G250
Coomassie R
Copper Phthalocyanine
tetrasulfonic acid
Lissamine Green (Disodium
Phthalocyanine)
Eosin Y
Acid Blue 90
Acid Blue 83
Acid Blue 249
C47H48N3NaO7S2
C45H44N3NaO7S2
C32H12CuN8Na4O12S4 10% calsolene
Acid Green 50
C27H25N2NaO7S2
10% calsolene
Acid Red 87
C20H6BrNa2O5
Added polar solvent
(DMSO)
Erioglaucine (FD&C 1)
Fast Green FCF
Indigo Carmine
Iron (III) phthalocyanine
Magnesium phthalocyanine
Malachite Green
Manganese (II) Phthalocyanine
Acid Blue 9
Food Green 3
Acid Blue 74
C37H34N2Na2O9S3
C37H34N2Na2O10S3
C16H8N2Na2o8s2
C32H16FeN8
C32H16MgN8
C23H25ClN2
C32H18MnN8
Methyl Blue
Methyl Orange
Methylene Blue
Nigrosin (Acid dye)
Ninhydrin Purple
Orange G
Picric Acid
Remazol Brilliant Blue R
Rhodamine B
Tartrazine
Zinc phthalocyanine
Acid Blue 93
Acid Orange 52
Basic Blue 9
a
Basic Green 4
Acid Orange 10
Reactive Blue 19
Basic Violet 10
Acid Yellow 23
C37H27N3Na2O9S3
C14H14N3NaO3S
C16H18CIN3S
C22H16N603
C9H6O4
C16H10N2Na207S2
C6H3N3O7
C22H18N2O11Na2S3
C28H31CIN2O3
C16H9N4Na3O9S2
C32H16N8Zn
10% citric acid
10% calsolene
Base
10% calsolene
Base
Acid
Base
All dyes purchased from Sigma-Aldrich Corporation (St. Louis, MO, USA; www.sigmaaldrich.com/).
Color
Yellow
Red
Comments
Faded
Light fastness not good
Did not dye Needs input of energy (heat) to enter feather
(e.g., hair dryer)
Did not dye Dyes connective tissue
Bright red
Even blueblack
Blue
Blue
Bright Blue
Even dark
blue
Red
Did not dye
Did not dye
Did not dye
Dark black
Dark teal
Green
Medium
black
Did not dye
Did not dye
Blue
Did not dye
Did not dye
Food medicine
cosmetics
Cosmetics
Medical research
Food, cosmetics
Medical use
Medical use
Medical use
Medical use, Cosmetics,
Tattoos
Medical use
Faded
Medical use
Rinsed out- precipitated out
Rinsed out
Medical use
Rinsed out
Dyes proteins–amines
Did not dye
Very light
Yellow
Did not dye
Violet-red
Rinsed out
Yellow
Rinsed out
Light teal
Rinsed out and precipitated
Medical use
Medical use
5
some dyes proved to be brighter with the addition of
Calsolene HSO, which acidifies the solution.
Our standardized tests for all 30 dyes used a solution of 30%
ethanol and 1% Synthrapol or Calsolene on 2 kinds of
feathers: 1) feathers from a pillow, and 2) naturally molted
contour feathers. We acquired the first set of molted feathers
from dropped gull (Laridae) feathers found on the beach.
Later, we acquired feathers from black-necked swans
(Cygnus melancoryphus), donated by the Greater Los Angeles
Zoo (M. Hines, Curator). The latter proved the best testing
feathers in part because they were large, undamaged, and free
of sand. Pillow feathers had been bleached and treated so, to
compensate, we simulated natural oils by applying canola oil.
To test the effects of the oil on dye penetration, we left half of
the feathers unoiled. We did not oil the gull or swan feathers
because they had natural oils. To simulate effects of
immersion in the ocean after being marked, we washed
dyed feathers by dipping and swirling in seawater. To
simulate the birds’ preening, we wrung dyed feathers with
moderate pressure between index finger and thumb 3 times.
We set up time increments of 5, 10, 15, and 30 min after
dyeing to wash and wring feathers. Also, we included a subset
of feathers dried with a hand-held hair dryer before washing
and wringing for a control. One hour after the initial rinsing
treatments, we put all feathers in the sun, and washed and
wrung them for 2 min every 30 min for 3 hr, simulating
immersion in the ocean and preening. We left all feathers in
the sun for 2 months and observed them every 2 weeks, from
10, 20, and 30 m, noting color quality and detectability at
each distance. On completion, we ranked all of the dyed
feathers qualitatively based on the amount of fading that had
taken place over the course of the initial tests and at what
distance we could see the colors well. We did not use
scientific instruments to measure visibility (e.g., reflectance
measured by a spectrophotometer) because we wanted data
showing qualitative values based on a practical human
determination of visibility.
Testing Experimental Dyes In Vivo
The goal was to use these dyes on endangered California least
terns, so we first tested them on a surrogate species, brownheaded cowbirds (Molothrus ater; hereafter, cowbirds; mass
38–50 g), a common bird similar in mass to least terns
(30–45 g; Cornell Laboratory of Ornithology 2015). We
trapped and then banded 35 free-living cowbirds with U.S.
Geological Survey Bird Banding Laboratory (USGS) bands
and uniquely colored plastic leg bands and kept them in a
flight cage 4.57-m (15 ft) 3-m (10 ft) 2.44-m (8 ft) in
height, equipped with dowels to perch on. We provisioned
water and birdseed daily. Cowbirds were free to fly short
distances and forage on the ground.
We chose 6 dyes from the 26 dyes from Sigma Aldrich (St.
Louis, MO, USA), which we tested in the in vitro trials, to
use on the surrogates, because they were approved by
the U.S. Food and Drug Administration for use in food,
cosmetics, or medicine: Azo Eosin (Acid Red 4), Copper
Phthalocyanine (Acid Blue 249), Lissamine Green (Acid
Green 50), Manganese (II) Phthalocyanine, Cobalt Phtha6
locyanine, and Iron (II) Phthalocyanine. Most compounds
toxic to mammals are also toxic to birds (Dumonceaux and
Harrison 1997); therefore, an in vivo test on cowbirds (as
examples of all birds) would suffice for one on mammals, and
vice versa. We divided the 35 birds into 7 groups of 5 birds
each: 1 group for each experimental dye tested and 1 control
group that we painted with isopropyl alcohol and Synthrapol.
Dyes painted on birds were dissolved in the same
concentration as dyes used on the in vitro-tested feathers
(30% isopropyl alcohol with 1 mL Synthrapol). For Copper
Phthalocyanine, Lissamine Green, and Manganese (II)
Phthalocyanine, we added 10% Calsolene for better wetting.
For Azo Eosin, we added 10% citric acid for better
penetration. We painted dyes onto the scapulars, tail, and
right foot of each bird with a foam brush. We held birds until
the dye dried—<5 min. We monitored birds for 30 days, and
observed each bird for 10 min twice per day at randomly
assigned times, to determine if they were active and eating.
We scored birds in the same way we had scored them during
the acclimatization period.
We monitored for signs of listlessness, imbalance, or other
gross indicators of ill health to assess whether there was an
acute poisoning or adverse effect from the dyes. Also, we
looked for specific signs of photophobia, epiphora (tearing),
coughing, sneezing, hyperventilation, shortness of breath,
somnolence, salivation, bloody feces, or vomiting, which are
acute markers of toxins in the blood (Dumonceaux and
Harrison 1997). Scores were on a qualitative scale of 1–3 for
each 10-min period of observation, with 3 being highest, for
a) activity level (1 ¼ listless, 2 ¼ inactive, 3 ¼ active), b)
eating (1 ¼ did not eat, 2 ¼ tried to eat but could not,
3 ¼ ate), c) apparent health (1 ¼ wings droopy or eyes closed,
2 ¼ feathers not preened or eyes irritated, 3 ¼ normal
appearance). We did not measure seed or water consumption, nor weigh birds. We dosed these birds only once with
dye, so we expected no long-term or chronic effects. At the
end of 30 days, we released all birds.
We followed protocol on permits from the U.S. Fish and
Wildlife Service Endangered Species Office, the USGS
Bird-Banding Permits and on the Memorandum of
Understanding from the State of California. During all
research, we adhered to the Ornithological Council’s
trapping and marking guidelines for birds (Fair et al. 2010).
RESULTS
Testing Conventional and Experimental Dyes In Vitro
Pillow feathers did not hold the conventional dye well. All
basic dyes tested with washing increments of 5 and 10 min
washed out of all sets of feathers (molted and treated). All
dyed feathers from the 15-min washing increment faded
considerably, so that they were hard to see at a distance of
>10 m. Only molted feathers dried with a hair dryer or
washed after 30 min were visible at a distance of 20 m after
washing. Even for these, all of the conventional basic dyes
that had not rinsed out immediately faded during the 3-hr
postdyeing washing regime and lasted no longer than
2 weeks; then were only visible at <10 m. Picric Acid did not
Wildlife Society Bulletin
9999()
Table 2. Success rates of marking and percentage of remotely dye-marked California least terns in San Diego, California, USA, during 1993–2009.
Colony
Delta
North Island
Ocean
Total
Population
No. of
attempts
Attempts: %
of population
No. of hits
Success rate:
hits/attempts
Dyed population
218
48
76
342
20
30
54
104
9.17%
62.5%
71.05%
30.4%
18
16
43
77
90.0%
53.33%
79.63%
74.04%
8.26%
33.33%
56.58%
22.51%
fade up to 2 months postdyeing, but its color was too light to
be visible at a distance of >10 m.
Colors of the 6 chosen experimental dyes did not rinse out,
and were visible from 30 m over >2 months without
fading. These 6 were 1) the sulfonated derivative of Copper
Phthalocyanine (Copper Tetrasulfonic acid, Color Index
Acid Blue 249), 2) Azo Eosin (Color Index Acid Red 4), 3)
Lissamine Green B (Color Index Acid Green 50), 4) Cobalt
Phthalocyanine, 5) Manganese Phthalocyanine, and 6) Iron
(II) Phthalocyanine.
Development of Dye Machine Using Conventional Dyes
The dye machine marked terns with minimal disturbance,
and all dyed birds returned to incubate their eggs. Operating
the machine improved with experience, and the “colony
success rate” (birds dyed per attempt), increased from the first
colony where we dyed, North Island, to the last, Delta colony
(Table 2). Subcolonies differed in numbers of nesting pairs
(48 North Island, 76 Ocean, 218 Delta); thus, our success
rate (% of dyed birds/colony) depended both on our
technique and colony size.The overall success of dyed birds
per dye attempt was 74%. We dyed a mean of 22.5% of all
nesting birds on the 3 colonies [range ¼ 8.3–56.6%]).
We labeled a dye shoot unsuccessful if the tern remained
off-nest for >30 min before we could attempt to dye or if it
sat in an incorrect position for aiming the nozzle for
>30 min. We divided off-nest times into 1) time from when
we first flushed the adult from the nest while we set up the
dye machine until it resettled on the dummy eggs, and 2)
time from when the adult left the nest postmarking until it
again settled on the real eggs. The average total off-egg time
before marking was greater than after marking, but it was
well within the 30 min we had set as a maximum for being
off-nest (Table 3). In 96 dye bouts, the mean minutes we
spent on-site (setup, in the blind waiting for return, and
removal of the machine) were 22.7 12.3, and median
minutes onsite was 20.0. During our setup activities, terns
generally flew above or stood within 6–8 m of the nest,
watching. Our time onsite and time of terns off the nest
differ because we often dyed >1 tern simultaneously, using
2 machines at once.
All dyed birds went to the water immediately after being
dyed, but soon returned to their nests. Terns plunge-dive and
constantly wet their feathers, so the conventional dyes we
used washed off after 2 days and we could not distinguish
birds from different colonies.
Testing Experimental Dyes In Vivo
The acid and metal phthalocyanine dyes that we wanted to
use in the dye machine had never been tested on live animals.
Baird et al.
Remote Dye Machine and Permanent Dyes
Although they were not as visible on the brown feathers as
they were on white feathers in our in vitro tests, testing on
cowbirds of the same mass as least terns sufficed for testing
toxicity. None of the birds in any test group (including the
control group) showed any signs of ill health or inactivity.
No birds scored a 1 (listless) or 2 (inactive) on the 3
measures of: activity, eating, and general health. Two birds
ingested the dye by biting the brush as the dye was applied
(Acid Blue 249 and Iron (II) Phthalocyanine). Neither of
these showed any ill effects over the 30 days held. The
activity, eating habits, and health of dyed birds were the
same as undyed birds. All birds had a score of 3 for all
periods of observation in the categories activity, eating, and
apparent health. All birds had a score of 3; therefore, we did
not perform test statistics.
DISCUSSION
Development of a Remotely Controlled Dye Machine
Our remotely activated dye machine was an improvement on
previously used remote marking units and superior to other
methods for marking birds without handling them. The
squirt gun provided an efficient and nonintrusive method of
marking, and we recommend the dye machine for marking
large numbers of ground-nesting birds, or mammals that
have regular lookout sites or areas in front of their dens or
burrows. The technique is especially effective for marking
colonial ground-nesters because many birds can be dyed
simultaneously.
Previous devices that squirted dye were not suitable for
targeting individuals because of inaccurate dye application
(e.g., broad-swath sprinklers or throwing dye-filled objects at
birds), or faults in the equipment (e.g., cumbersome
equipment with disturbance issues, or by low pressure at
the output; Moffitt 1942, Tickell 1968, Moseley and Mueller
1975, Wendeln et al. 1996). Passive methods such as dyeing
Table 3. Mean (SE) minutes of off-egg times of California least terns
before and after being remotely dye-marked in San Diego, California, USA,
during 1993–2009.
Off-egg
n
Mean min.
Median min.
Before markeda
After markedb
Total
101
19.03 1.00
18
80
13.83 1.39
9
181
32.41 2.02
29
a
Before marked: From when the adult was first flushed from the nest while
we set up the apparatus until it resettled on the dummy eggs once we were
in the blind.
b
After marked: When the adult left the nest postmarking until it again
settled on the nest.
7
eggs or placing dye in front of or in nests potentially
jeopardizes live eggs (Mossman 1960, Paton and Pank 1986,
Cavanagh et al. 1992, Belant and Seamans 1993, Donehower
and Bird 2005). Donehower and Bird (2005) state likewise
that the technique of self-marking by birds where dye is
placed in the nest is not good because the pattern of dye is
more random and individuals cannot be marked at a targeted
part of their bodies. The same is true for techniques such as
paintball land mines Fox (2010) and eggshells or light bulbs
thrown at birds (Bendell and Fowle 1950).
The physical layout of the North Island colony contributed
to the low success rate of dyeing. This colony was located on a
concrete airfield with a thin layer of sand on top, which
caused a problem in the placement and concealment of the
nozzle and hose. Concealment of the hose helps to keep it in
place, but on the concrete airfield with little ground cover or
sand, the hose could move slightly with a light breeze or from
the force of the dye going through it; because of this, the aim
of the hose there was not perfect. However, despite these
factors, the overall success rate of the dye machine on all 3
subcolonies (hits/attempts) was 74%; excluding North
Island, the success rate was 82%.
Most of the unsuccessful attempts after the first week were
due to the terns’ positions once on the nest and not problems
with the gun. Wendeln et al. (1996) encountered similar
problems with differences between bird orientation and
nozzle direction making dyeing impossible. Lack of success
was also not from an adult being off-nest during the dye
session for >30 min. Terns did not react to the presence of
our equipment or us, once we returned to the blinds.
The entire process did not appear to have negative effects
on the birds. All birds dyed hatched the eggs on which they
had been sitting when dyed. We did not observe any increase
in frequency of predation on dyed birds. Average total offegg time both before and after marking was small, suggesting
minimal disturbance to the terns. We did not have data on
hatch success of other terns that we did not dye.
Testing Conventional and Experimental Dyes In Vitro
We fulfilled our goal to find dyes that lasted 2 months and
were visible from >30 m without having to be dried after
application; these were either acid or phthalocyanine
“experimental” dyes. Most dyes used in prior studies on
birds or mammals faded and were difficult to detect at
distance depending on how much of the animal was dyed
(Kozlik et al. 1959), or how saturated the dye became (M.
Haramis, U.S. Geological Survey, personal communication;
Table S2, available online in Supporting Information).
Depending on methods of application and concentrations of
solutions, some dyes lasted no more than 2 weeks (Cavanagh
et al. 1992, Belant and Seamans 1993), although Evans and
Griffith (1973) used Rhodamine B, Malachite Green, or
Picric Acid, which lasted 4 days to 5 months, depending on
application method and dye. The success of basic dyes for >2
weeks on most animals was because either the animals were
held until drying of the dyed feathers (Kozlik et al. 1959,
Moseley and Mueller 1975, Warnock et al. 1995,
Donehower and Bird 2005) or dyed fur (Evans and
8
Holdenried 1943, Keith et al. 1968, Evans and Griffith
1973), or because of the large amount of dye placed on the
animal. Evans and Griffith (1973) placed so much dye on
rabbits, that they found dye internally, dyeing organs, and
Forster (1973) put so much dye on swans that they could not
fly. Commercial fur dyes lasted a median of 30–60 days on
Beechey ground squirrels (Otospermophilus beecheyi; Evans
and Holdenried 1943), although today, the dyes are
considered hazardous, explosive, and unsuitable for use on
live animals. Dyes that lasted the longest without fading
ranged from a maximum of 3 weeks for Belant and Seamans
(1993), 28–42 days for Cavanagh et al. (1992), to 4.5 months
for Furness and Galbraith (1980).
Others have used Batik dye or permanent markers, which
we determined unsuitable for our use because of their
harmful ingredients and their impermanence (Wadkins
1948, Kennard 1961, Donehower and Bird 2005). Kennard
(1961) used Drimark markers applied via a with a sponge, on
black-capped chickadees (Poecile atricapillus), and only the
red Drimark lasted >4 weeks. However, ingredients in
Drimark dyes might be unsafe because they contain toxic
ingredients (commercial dye in a highly volatile organic
carrier solvent, methyl isobutyl ketone–n-butyl acetate,
diethylene glycol monobutyl ether–ethyl acetate–poly ethylene glycol, or polycarboxylic acid, and has metallic dye
particles suspended in a resin polymer, Sukhna and
Reichmann 2003). Vegetable and commercial wool dyes,
and stamp-pad ink did not last for >2 weeks (Kennard
[1961]); and ink-jet printer ink ran when in contact with
water (Fox 2010). The ink is also basic and thus similar to
textile dyes (Nyman and Hakala 2011).
Of the 26 experimental dyes we tested, 10 proved to be the
best in longevity and detectability among other acid and basic
conventional dyes, and 10 were used in medicine or in the
cosmetic or food industry of the United States and approved
as safe by the U.S. Food and Drug Administration. Of dyes
approved as safe, only 8 had good longevity and detectability.
We were left with 6 good dyes because Coomasie G250 and
Coomasie R were too expensive. Copper Phthalocyanine
Tetrasulfonic acid–Acid Blue 249 is used to color
polypropylene nonabsorbable sutures for use in general
and ophthalmic surgery (Food and Drug Administration
2010, pubMed.gov 2014) and in tattoos (Kaur 2016). Azo
eosin–Acid Red 4 is used to inhibit toxins of fungus in food
(Hitokoto et al. 1980) and added to nail polish (Sharma and
Kaur 1994) and lipstick (Anstead 1959). Lissamine Green–
Acid Green 50 is used in ophthalmological surgery or
diagnostics (Manning et al. 1995, Kim 2000, Abelson and
Ingerman 2005, Hamrah et al. 2011), and Manganese (II)
Phthalocyanine is used in photodynamic therapy for
treatment of cancer (Moreira et al. 2008). Cobalt Phthalocyanine and Iron (II) Phthalocyanine are in a class of drugs
that is pharmacologically inactive, but when exposed to
ultraviolet radiation or sunlight is converted to its active
metabolite that affects diseased tissue (Staicu et al. 2013).
These compounds can be administered topically or
systemically and have been used therapeutically to treat
psoriasis and various types of neoplasms as well as
Wildlife Society Bulletin
9999()
Alzheimer’s disease (Pankratov et al. 2014, Tabassum et al.
2015). Cobalt Phthalocyanine is also an antitumor delivery
system by itself when combined with citric acid (Medvedev
and Leshchenko 2012). The phthalocyanines themselves
seem to have useful properties for cancer therapy (Ben-Hur
and Rosenthal 1988).
Using this suite of acid and phthalocyanine dyes in the dye
machine would be ideal for marking large numbers of
colonial seabirds or mammals that are stationary in
predictable places. There are permit restrictions on handling
endangered species, so the dye machine would be an easy
hands-off way for marking endangered colonial birds or
endangered mammals. Paired with the permanent dyes,
using the dye machine would also be a way to deliver dye to
animals that researchers do not want to trap in order for the
dye to dry. We define “permanent” as not fading and keeping
a true color until molt or shed of feathers or fur.
Biochemical Differences between Acid (Experimental)
and Basic (Conventional) Dyes
The superiority and permanence of acid or metal phthalocyanine dyes compared with basic dyes lies in the molecular
structure of the dye itself, not of the wetting compound.
Unlike basic dyes that are topical, acid dyes and metal
phthalocyanine dyes have the ability to form hydrogen bonds
with the amino acid groups on the keratin protein, which
makes up the majority of feathers or fur. Thus, they are
incorporated into the feathers or fur themselves. The 2 also
attract each other by van der Waals forces (P. Burch, personal
communication). Acid dyes typically have a colorless cation
such as sodium, and a colored anion. Amino acids on feathers
or fur have a positive charge so that the negatively charged
anion of dye binds to them.
Basic dyes have a colored cation, such as Methylene Blue,
combined with a colorless anion, such as chloride. The
negatively charged and colorless anion of chloride will not
cause a noticeable color change when bonded to the positive
amino acids of the fur or feathers. When rinsed, the colored
positive cation will wash away because it is not incorporated
into the feather (P. Burch, personal communication; Talleur
2010; D. Talleur, personal communication).
Colors of basic dyes attach to the feather only when bound
to an adherent such as silica gel so that they sit on top of the
feather, temporarily sticking to it (Belant and Seamans 1993,
Talleur 2010, D. Talleur, personal communication). The
colored portion is never incorporated into the feather, and
essentially is glued to the surface of the feather (summary of
biochemistry of acid dyes in Supplement S3, available online
in Supporting Information).
Dyes thus incorporated into feathers or fur are unable to be
ingested or preened off and, therefore, are particularly suited
for use in wild animals as harmless dyes. In contrast, basic
dyes are ingestible because they are only physically and
topically adhered to the top of feathers or fur via resins or
gels, and thus potentially more toxic than are acid or
phthalocyanine dyes. Any choice of acid or phthalocyanine
dyes should be limited to those used in either foods for
human consumption, in cosmetics, or in medical testing.
Baird et al.
Remote Dye Machine and Permanent Dyes
Dyes other than these should be tested on live animals for
toxicity.
Testing of Experimental Dyes In Vivo on a Surrogate
Species
We showed that the 5 experimental dyes were not harmful to
brown headed cowbirds over a 30-day period postdyeing.
The subjects showed no signs of photophobia, epiphora
(tearing), coughing, sneezing, hyperventilation, shortness of
breath, somnolence, salivation, bloody feces, or vomiting,
which are symptoms of toxins (Dumonceaux and Harrison
1997). It was beyond the scope of this project to analyze any
blood markers for toxins. The dyes did not mat the feathers
because they dried quickly; there was such a small amount of
liquid squirted onto the feathers that we presume the dye did
not change the thermal properties of the feathers.
Advantages of using acid and phthalocyanine dyes are 1)
permanence of color until molt in birds or shedding in
mammals, 2) no change in observed color over time, and 3)
inability of an animal to ingest the dye because it chemically
binds with the feather or fur on contact. The experimental
dyes would be ideal to mark species that contact water.
Conventional dyes (basic dyes, indelible ink markers, Batik,
etc.) have the disadvantages of fading quickly, nonadherence
to feathers or fur, and potentially toxic carriers able to be
ingested because they are not chemically incorporated into
the animal’s feather or fur. Conventional dyes also have a
wide range in durability or in visibility from >30 m, and most
colors fade quickly over time.
Some acid or metal phthalocyanine dyes hold promise for
permanent marking of animals because these experimental
dyes seemed to have had no adverse effects on cowbirds, and
so the next step for an approval of this suite of dyes by
the U.S. Geological Survey Bird Banding Laboratory and
the U.S. Fish and Wildlife Service would be to apply these
dyes to other birds such as seabirds or ducks (Anatidae) and
test the in vivo permanence of the dyes in conditions where
the bird is exposed to water. They could also be applied to
mammals that use water, although the majority of these have
dark fur and the dye probably could not be detected.
ACKNOWLEDGMENTS
We thank the U.S. Southwest Navy Facilities Engineering
Command for their generous support of this project,
Contract #N68711-95-LT-C006, especially our project
officer, T. Burr. Baird thanks Hink for his creativity and
ingenuity, and ability to come up with such a Rube Goldberg
device as the dye machine, and thanks both Hink and
Robinette for their tireless efforts in building and rebuilding,
testing and retesting the machine until it worked perfectly.
The masterminds behind development of the acid dyes were
Hink and Robinette and the research would not have
happened without their work. P. Baird thanks my graduate
and undergraduate students at California State University for
their enthusiasm, novel ideas, and persistence: V. Wawerchak, K. Marantos, T. Carpenter, R. Johnston, R. Rita, C.
Miller, K. Mabb, and B. Henderson; and for help with the in
vivo study, we thank H. Baird-Herron and J. D. Herron. We
9
thank M. Hines and C. Christel of the Greater Los Angeles
Zoo, who supplied black-necked swan feathers. We also
thank the 2 anonymous reviewers and also R. Elner and H.
Streby for their helpful comments. Thanks to T. Robinson
for help with the figures.
This paper is dedicated to Dick Talleur, fly-tying expert
(1932–2011); Ted Roubal, chemist; Sigma Aldrich (1930–
2014); and Paula Burch, biochemist and hand dyeing
consultant, Houston, Texas, USA—without the many hours
of background research they graciously undertook on their
dime, as well as the time they took discussing dyes with us,
we never would have been able to come up with a good list of
dyes to test. We owe the success of our project to them.
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Associate Editor: Streby.
Baird et al.
Remote Dye Machine and Permanent Dyes
SUPPORTING INFORMATION
Additional supporting information may be found in the
online version of this article at the publisher’s web-site.
Supplement S1. Detailed methods of dye machine with
tables, figures, references.
Table S1-1. Marking techniques used in other studies.
Table S1-2. Parts list of the remote dye applicator (“squirt
gun”).
Table S1-3. Parts list key to distribution unit.
Figure S1-1. Remote dye applicator “squirt gun.”
Figure S1-2. Top view of remote distribution unit.
Figure S1-3. Front view of remote distribution unit.
Supplement S2. Table of summary of other studies on
dyeing birds, including species, dyes used, longevity, toxicity,
duration, references.
Supplement S3. Biochemistry of dyes. Summary and
references.
11