Regulation of red fluorescent light emission in a cryptic marine fish
© Wucherer and Michiels; licensee BioMed Central Ltd. 2014
Received: 9 September 2013
Accepted: 23 December 2013
Published: 8 January 2014
Animal colouration is a trade-off between being seen by intended, intra- or inter-specific receivers while not being seen by the unintended. Many fishes solve this problem by adaptive colouration. Here, we investigate whether this also holds for fluorescent pigments. In those aquatic environments in which the ambient light is dominated by bluish light, red fluorescence can generate high-contrast signals. The marine, cryptic fish Tripterygion delaisi inhabits such environments and has a bright red-fluorescent iris that can be rapidly up- and down-regulated. Here, we described the physiological and cellular mechanism of this phenomenon using a neurostimulation treatment with KCl and histology.
KCl-treatment revealed that eye fluorescence regulation is achieved through dispersal and aggregation of black-pigmented melanosomes within melanophores. Histology showed that globular, fluorescent iridophores on the anterior side of the iris are grouped and each group is encased by finger-like extensions of a single posterior melanophore. Together they form a so-called chromatophore unit. By dispersal and aggregation of melanosomes into and out of the peripheral membranous extensions of the melanophore, the fluorescent iridophores are covered or revealed on the anterior (outside) of the iris.
T. delaisi possesses a well-developed mechanism to control the fluorescent emission from its eyes, which may be advantageous given its cryptic lifestyle. This is the first time chromatophore units are found to control fluorescent emission in marine teleost fishes. We expect other fluorescent fish species to use similar mechanisms in the iris or elsewhere in the body. In contrast to a previously described mechanism based on dendritic fluorescent chromatophores, chromatophore units control fluorescent emission through the cooperation between two chromatophore types: an emitting and an occluding type. The discovery of a second mechanism for fluorescence modulation strengthens our view that fluorescence is a relevant and adaptive component of fish colouration.
KeywordsPigmentation Fluorescence Tripterygiidae Triplefin blenny Camouflage Signalling Marine fishes
Colour vision is widespread in the animal kingdom and has driven the evolution of body colouration . Conspicuous colouration is often associated with mate choice [2–4], warning signals [5–7] or species recognition and communication [8–11]. Light emission through bioluminescence has also been proposed as a detection and communication mechanism . Cryptic colouration patterns, however, are required to hide from visual predators or to approach potential prey [9, 10, 13, 14]. Many colour patterns are therefore a compromise between being visible to the intended receivers while avoiding the attention of the unintended, e.g. predators [15–18]. These opposing forces drive the evolution of adaptive, context-dependent body colouration [19–21]. Cephalopods, bony fishes, amphibians and reptiles achieve this by complex arrangements of pigmented skin cells or chromatophores, such as melanophores (black), xanthophores (yellow), erythrophores (red) and iridophores (structural colours) [9, 21, 22]. It is the complex interplay of these cell types that generates colour appearances ranging from well-camouflaged lizards to the most brightly coloured reef fishes .
Colourful aquatic animals face the constraint that water absorbs long wavelengths (> 600 nm) to a much higher degree than short and medium wavelengths . Consequently, many marine environments below 10–20 m are essentially blue-green. In the absence of long wavelengths, however, none of the usual reflective pigmentation mechanisms can generate shades of red (600–700 nm). Fluorescent pigments can restore those “lost” colours by absorbing the available light and re-emitting it at a longer wavelength [24–26]. This process is different from bioluminescence, where photons are generated through a chemical reaction. In many fishes and cephalopods, the latter function is provided by microbial symbionts [26–28].
Many marine animal phyla are known to fluoresce, with cnidarians being the best investigated group [29–34]. We recently showed that a number of fish taxa show fluorescence in the near red range (600–630 nm) and proposed fluorescent pigmentation as a new signalling mechanism or a mechanism for highlighting prey or predators with reflecting eyes . Knowing that many marine fishes are trichromatic [35, 36], red fluorescence has the potential to generate strong, visible chromatic contrasts at depth. Conspicuous signals, however, may attract attentive predators that can see them. We would therefore expect that fluorescence can be modulated on demand – as is the case for (eye) colouration in other marine fishes . Recently, we described a first pigment cell type with this feature: a dendritic, red fluorescent chromatophore in the clear fins of the pygmy goby Eviota atriventris (previously misidentified as Eviota pellucida, see ) that actively disperses and aggregates intracellular fluorescent particles, modulating the brightness of the fluorescent emissions .
Change in fluorescence brightness after KCl treatment
The long wavelength fluorescence in the iris of T. delaisi is emitted by red fluorescent guanine crystals, which are stacked in iridophores, the dominant cell type in the stratum argenteum. The brightness of fluorescence is modulated by rapid (2–6 min) transport of melanosomes between the soma of posterior melanophores and their finger-like extensions that stretch anteriorly through the stratum argenteum and cover the iridophores anteriorly. Given that the whole process can be controlled by the presence or absence of K+ ions indicates that it is under neuronal control . Histological investigation revealed that iridophores and melanophores cooperate in so-called chromatophore complexes or units, whereby multiple cells of one type interact and overlap with multiple cells of the other kind. This is mainly due to the network-like structure generated by the cellular extensions of the melanophores. Such complexes are known to control colouration in the skin of fishes, amphibians and reptiles [21, 23, 53]. Chromatophore units often consist of a xanthophore and/or iridophore plus a melanophore . In T. delaisi only two kinds of chromatophores are involved. In all cases, posterior melanophores aggregate or disperse melanosomes, thereby controlling the brightness  of the associated anterior iridophores. Our study now shows that such units are also used to control fluorescent emission.
The presence of red fluorescence in guanine crystals is a feature known from other red fluorescent fish species, including pipefish of the genus Corythoichthys. The iris of Corythoichthys paxtoni has a structure similar to that of T. delaisi. It is therefore quite likely that some pipefish also possess chromatophore units similar to the ones described here. Own field observations indicate that other triplefin species of the genera Tripterygion, Helcogramma and Enneapterygius and gobies belonging to the genus Ctenogobiops and Istigobius also show red fluorescent irides that can be quickly darkened or lightened (pers. observations, N. K. Michiels), suggesting that this mechanism is not limited to a few rare cases.
An active role for iridophores?
Our data do not allow us to make conclusive inferences whether the observed changes in fluorescent emission are in part caused by conformational changes in the orientation or distance of the guanine platelets in the stratum argenteum. Motile iridophores are known from cephalopods  as well as from fishes with prominent iridescent or structural colour patterns [57–61]. In some of these cases, rapid (within seconds) changes in hue and brightness can be observed through conformational changes in motile iridophores. Although our data do not allow us to exclude that such a process may have contributed to the observed changes in brightness, the emitted hue remained unaffected under the conditions tested (Figure 4).
Comparison with colour change mechanisms in cephalopods
An analogous, well-understood mechanism to modulate colour is the chromatophore organ in cephalopods . It also consists of different cell types that cooperate to control colour . In cephalopods, however, this is achieved by the action of radial muscles that change the shape of coloured chromatophores. Upon contraction, the muscles stretch and thereby display the pigmented content of a pigment sac inside the chromatophore [23, 64]. Muscle relaxation leads to spontaneous contraction of the pigment sac, hiding the pigment [63, 64]. Light passing through the system is reflected by iridophores that sit behind the complex.
As K+ stimulates action potentials in neurons, it is safe to conclude that T. delaisi modulates its fluorescence through a neuronally-controlled mechanism . We observed that specimens of T. delaisi become darker when stressed or when inactive, but during spontaneous activity, particularly when foraging, the brightness of the iridial fluorescence visibly increases (unpublished observations). The brightness of fluorescence therefore likely constitutes a relevant cue that is possibly used in a foraging context. Since peak emission is in the near-red spectral range (590–610 nm), it is very likely that other fish can perceive the fluorescence of T. delaisi. Work in progress confirms that T. delaisi is a trichromat including a LWS receptor, making it likely that it can see its own fluorescence.
Red fluorescence in the iris of T. delaisi is controlled by so-called chromatophore units, which consist of a melanophore and several fluorescent iridophores. Modulation of fluorescence is achieved by nervous control of the aggregation state of melanosomes in melanophores. The presence of this sophisticated control mechanism suggests that T. delaisi controls its fluorescence actively. This reduces the constraints raised by the colouration trade-off between contrast and camouflage at depths below -10 m. In shallower water, the same process will modulate the overall reflective properties of the iris.
Material and methods
Fluorescence in Tripterygion delaisi
Tripterygion delaisi (Tripterygiidae) occurs throughout the East-Atlantic Ocean and West-Mediterranean Sea. It is a small (up to 6 cm), cryptic, benthic predator feeding on micro-crustaceans between -5 and -40 m depth. When approached, individuals freeze rather than flee, indicating that they rely on their camouflage. Yet, T. delaisi has prominent red fluorescent irides (Figure 1). Its fluorescence is characterized by light absorption across a broad range of the ambient spectrum (Figure 2) and a peak emission at 600 nm (bright red). The relationship between fluorescence and ambient light will be published in detail elsewhere (Michiels et al. in prep.). All juvenile (< 1 cm) and adult stages show fluorescent irides throughout the year. The brightness of fluorescence can vary strongly and quickly (Figure 1). Pilot studies in the field and in the lab showed that downregulation is associated with inactivity or stress (e.g. when handled). Upregulation is often seen in the context of foraging.
Specimens of T. delaisi were collected in Corsica, France at the STARESO Marine Science Station, under the general sampling permit of the station. In Tübingen, Germany, fish were kept in individual divisions of a large flow-through aquarium (20°C, salinity 34%, pH 8.2). For the experiments, fish were decapitated, dissected and the eyes were stored in physiological saline as described by Wucherer and Michiels . All work was carried out and recorded in accordance to German animal protection legislation.
Temporal change in fluorescence area and brightness
Eyes were immersed in saline by placing them on a perforated 8 mm ∅ plastic platform in a 35 mm ∅ petri dish. They were investigated under a Leica MZ 16 F fluorescence stereomicroscope (band-pass filter with 530–560 nm for excitation). Fluorescent emission was viewed through a second, non-overlapping bandpass-filter (590–650 nm) and documented using a Nikon D300 DSLR. For each treatment, a 450 s time-lapse recording was taken providing an image every 5 s. At the start (0 s) we replaced the saline with a high KCl-solution (in mM: NaCl 78, KCl 50, CaCl2 1.8, MgCl2 1.8, D(+)-Glucose 5.6, Tris–HCl 5.0; pH 7.2). Total ion concentration was identical to the saline solution. Eyes from eight fish were analysed, one of each fish exposed to the KCl-treatment, the other one to the control treatment.
In order to calculate the fluorescent area, images were imported as stacks into ImageJ (v. 10.2, J. Rasband, NIH, USA), set to 8-bit grey-scale and inverted. A threshold was set to distinguish between fluorescent and non-fluorescent areas (black in the original image). Then the fluorescent area of every image was determined by counting the proportion of fluorescent pixels relative to those of the whole iris. For statistical analysis, time and the proportion of fluorescent area were entered into JMP (v. 9, SAS, USA).
Fluorescence brightness (photon radiance) was measured using a SpectraScan PR670 spectroradiometer (Photoresearch, Chatsworth, CA, USA). Six eyes were dissected from three fish and pre-treated as described above. Each eye was illuminated at an angle of 45° with an LED light source with peak emission at 455 nm (LLS455, Sandhouse, Dunedin, FL, USA). Fluorescence was measured from above, perpendicular to the iris with the measuring point aimed to exactly cover the complete iris (0.5° measurement angle). Measurements were taken before and at 8 time points after application of the KCl solution: 0, 90, 120, 180, 240, 300, 360, 420, 450 s. Data were summarized as the cumulative sum of photons.s-1.sr-1.m-2 across the emission range (500–750 nm) (= fluorescence brightness).
Following KCl-treatment, eyes were fixed and embedded as described for fin tissue by Wucherer and Michiels . We cut 1.5 μm sections parallel to the axis of vision (axial plane) using a diamond knife and mounted the sections in a non-fluorescent medium (Vectashield, Vector). Digital micrographs of each section were stacked to generate a 3D-reconstruction of the chromatophore unit (chromatophores and surrounding cells) using TrakEM2 [66, 67]. The 3D-model was smoothed and vertices were reduced using Blender (v. 2.63a).
Sub-cellular structures in an iris cross-section were visualised by scanning electron microscopy of the fracture zone of an untreated freeze-dried T. delaisi iris by Oliver Meckes and Nicole Ottawa from Eye of Science GbR (http://www.eyeofscience.com) (Figure 6C).
Fish were sacrificed under permit no. ZO 1/10 from 18 Oct 2010, prolonged on 26 Nov 2011 till 15 Dec 2012 to the corresponding author. The permit was issued by the Animal Protection Office at the Regierungspräsidium, Referat 35, Konrad-Adenauer-Straβe 20, 72072 Tübingen, Germany.
This work was supported by Koselleck grant Mi482/13-1 from the Deutsche Forschungsgemeinschaft DFG to NKM. The manuscript benefited greatly from constructive criticism provided by Nils Anthes, Shaun P. Collin, Sandra Dangelmayer, Melissa Meadows and two anonymous referees. We are also very grateful to Oliver Meckes from Eye of Science GbR (http://www.eyeofscience.com) for producing excellent SEM pictures of the iris of T. delaisi together with Silke Probst. Thanks to Julia Steigleder for making the pictures for Figure 1B and C. Rita Triebskorn and Stefanie Krais (Uni Tübingen) kindly helped us with the histological sectioning. Thanks also to Oeli Oelkrug for taking care of the fish. Gregor Schulte provided constant support in microscopy, spectrometry and photography, for which we are very grateful.
- Marshall J: Why are animals colourful? Sex and violence, seeing and signals. Colour Des Creativity. 2010, 8: 1-8.Google Scholar
- Kozak GM, Head ML, Lackey ACR, Boughman JW: Sequential mate choice and sexual isolation in threespine stickleback species. J Evol Biol. 2013, 26: 130-140. 10.1111/jeb.12034.PubMedView ArticleGoogle Scholar
- Maan ME, Seehausen O, Van Alphen JJM: Female mating preferences and male coloration covary with water transparency in a Lake Victoria cichlid fish. Biol J Linn Soc. 2010, 99: 398-406. 10.1111/j.1095-8312.2009.01368.x.View ArticleGoogle Scholar
- Blakeslee C, McRobert SP, Brown AC, Clotfelter ED: The effect of body coloration and group size on social partner preferences in female fighting fish (Betta splendens). Behav Processes. 2009, 80: 157-161. 10.1016/j.beproc.2008.11.005.PubMedView ArticleGoogle Scholar
- Saporito RA, Zuercher R, Roberts M, Gerow KG, Donnelly MA: Experimental evidence for aposematism in the dendrobatid poison frog Oophaga pumilio. Copeia. 2007, 2007: 1006-1011. 10.1643/0045-8511(2007)7[1006:EEFAIT]2.0.CO;2.View ArticleGoogle Scholar
- Aronsson M, Gamberale-Stille G: Evidence of signaling benefits to contrasting internal color boundaries in warning coloration. Behav Ecol. 2013, 24: 349-354. 10.1093/beheco/ars170.View ArticleGoogle Scholar
- Guilford T: How do warning colors work - conspicuousness may reduce recognition errors in experienced predators. Anim Behav. 1986, 34: 286-288.View ArticleGoogle Scholar
- Siebeck UE, Parker AN, Sprenger D, Mäthger LM, Wallis G: A species of reef fish that uses ultraviolet patterns for covert face recognition. Curr Biol. 2010, 20: 407-410. 10.1016/j.cub.2009.12.047.PubMedView ArticleGoogle Scholar
- Mäthger LM, Denton EJ, Marshall NJ, Hanlon RT: Mechanisms and behavioural functions of structural coloration in cephalopods. J R Soc Interface. 2009, 6: S149-S163. 10.1098/rsif.2008.0366.focus.PubMedPubMed CentralView ArticleGoogle Scholar
- Losey GS: Crypsis and communication functions of UV-visible coloration in two coral reef damselfish Dascyllus aruanus and Dascyllus reticulatus. Anim Behav. 2003, 66: 299-307. 10.1006/anbe.2003.2214.View ArticleGoogle Scholar
- Kelley CD, Hourigan TF: The function of conspicuous coloration in chaetodontid fishes - a new hypothesis. Anim Behav. 1983, 31: 615-617. 10.1016/S0003-3472(83)80090-6.View ArticleGoogle Scholar
- Howland HC, Murphy CJ, McCosker JE: Detection of eyeshine by flashlight fishes of the family anomalopidae. Vision Res. 1992, 32: 765-769. 10.1016/0042-6989(92)90191-K.PubMedView ArticleGoogle Scholar
- Leclercq E, Taylor JF, Migaud H: Morphological skin colour changes in teleosts. Fish Fish. 2010, 11: 159-193.View ArticleGoogle Scholar
- Sumner FB: Does “protective coloration” protect? Results of some experiments with fishes and birds. Proc Natl Acad Sci USA. 1934, 20: 559-564. 10.1073/pnas.20.10.559.PubMedPubMed CentralView ArticleGoogle Scholar
- Endler JA: Variation in the appearance of guppy color patterns to guppies and their predators under different visual conditions. Vision Res. 1991, 31: 587-608. 10.1016/0042-6989(91)90109-I.PubMedView ArticleGoogle Scholar
- Endler JA: Some general comments on the evolution and design of animal communication systems. Philos Trans R Soc Lond B Biol Sci. 1993, 340: 215-225. 10.1098/rstb.1993.0060.PubMedView ArticleGoogle Scholar
- Marshall NJ: Communication and camouflage with the same ‘bright’ colours in reef fishes. Philos Trans R Soc Lond B Biol Sci. 2000, 355: 1243-1248. 10.1098/rstb.2000.0676.PubMedPubMed CentralView ArticleGoogle Scholar
- Hemmi JM, Marshall J, Pix W, Vorobyev M, Zeil J: The variable colours of the fiddler crab Uca vomeris and their relation to background and predation. J Exp Biol. 2006, 209: 4140-4153. 10.1242/jeb.02483.PubMedView ArticleGoogle Scholar
- Price AC, Weadick CJ, Shim J, Rodd FH: Pigments, patterns, and fish behavior. Zebrafish. 2008, 5: 297-307. 10.1089/zeb.2008.0551.PubMedView ArticleGoogle Scholar
- Cott HB: Adaptive coloration in animals. 1940, London: MethuenGoogle Scholar
- Hawkes JW: Structure of fish skin 2. Chromatophore unit. Cell Tissue Res. 1974, 149: 159-172. 10.1007/BF00222271.PubMedView ArticleGoogle Scholar
- Fujii R: The regulation of motile activity in fish chromatophores. Pigment Cell Res. 2000, 13: 300-319. 10.1034/j.1600-0749.2000.130502.x.PubMedView ArticleGoogle Scholar
- Bagnara JT, Hadley ME: Chromatophores and color change: the comparative physiology of animal pigmentation. 1973, Englewood Cliffs, N.J: Prentice-HallGoogle Scholar
- Lythgoe JN: The Ecology of Vision. 1979, Oxford: Clarendon PressGoogle Scholar
- Michiels N, Anthes N, Hart N, Herler J, Meixner A, Schleifenbaum F, Schulte G, Siebeck U, Sprenger D, Wucherer M: Red fluorescence in reef fish: a novel signalling mechanism?. BMC Ecol. 2008, 8: 16-10.1186/1472-6785-8-16.PubMedPubMed CentralView ArticleGoogle Scholar
- Johnsen S, Marshall NJ: Through the looking glass: are silvery fish safe from viewers with polarization vision?. Integr Comp Biol. 2012, 52: E87-E87.Google Scholar
- Haddock SHD, Moline MA, Case JF: Bioluminescence in the sea. Ann Rev Mar Sci. 2010, 2: 443-493. 10.1146/annurev-marine-120308-081028.PubMedView ArticleGoogle Scholar
- Widder EA: Bioluminescence in the ocean: origins of biological, chemical, and ecological diversity. Science. 2010, 328: 704-708. 10.1126/science.1174269.PubMedView ArticleGoogle Scholar
- Shimomura O, Johnson FH, Saiga Y: Extraction, purification and properties of Aequorin, a bioluminescent protein from the luminous hydromedusan Aequorea. J Cell Comp Physiol. 1962, 59: 223-239. 10.1002/jcp.1030590302.PubMedView ArticleGoogle Scholar
- Chalfie M, Tu Y, Euskirchen G, Ward W, Prasher D: Green fluorescent protein as a marker for gene expression. Science. 1994, 263: 802-805. 10.1126/science.8303295.PubMedView ArticleGoogle Scholar
- Salih A, Larkum A, Cox G, Kuhl M, Hoegh-Guldberg O: Fluorescent pigments in corals are photoprotective. Nature. 2000, 408: 850-853. 10.1038/35048564.PubMedView ArticleGoogle Scholar
- Kenkel CD, Traylor MR, Wiedenmann J, Salih A, Matz MV: Fluorescence of coral larvae predicts their settlement response to crustose coralline algae and reflects stress. Proc R Soc B-Biol Sci. 2011, 278: 2691-2697. 10.1098/rspb.2010.2344.View ArticleGoogle Scholar
- Field SF, Matz MV: Retracing evolution of red fluorescence in GFP-like proteins from Faviina corals. Mol Biol Evol. 2010, 27: 225-233. 10.1093/molbev/msp230.PubMedPubMed CentralView ArticleGoogle Scholar
- Mazel HC: Spectral measurements of fluorescence emission in Caribbean cnidarians. Mar Ecol Prog Ser. 1995, 120: 185-191.View ArticleGoogle Scholar
- Hart NS, Lisney TJ, Marshall NJ, Collin SP: Multiple cone visual pigments and the potential for trichromatic colour vision in two species of elasmobranch. J Exp Biol. 2004, 207: 4587-4594. 10.1242/jeb.01314.PubMedView ArticleGoogle Scholar
- Siebeck UE, Wallis GM, Litherland L: Colour vision in coral reef fish. J Exp Biol. 2008, 211: 354-360. 10.1242/jeb.012880.PubMedView ArticleGoogle Scholar
- Nicol JAC: The Eyes of Fishes. 1989, Oxford: Clarendon PressGoogle Scholar
- Greenfield DW, Suzuki T: Eviota atriventris, a New Goby Previously Misidentified as Eviota pellucida Larson (Teleostei: Gobiidae). Zootaxa. 2012, 55-62. 3197
- Wucherer MF, Michiels NK: A fluorescent chromatophore changes the level of fluorescence in a reef fish. Plos One. 2012, 7 (6): 7-View ArticleGoogle Scholar
- Zander CD, Heymer A: Tripterygion tripteronotus Risso 1810 und Tripterygion xanthosoma n. sp., eine ökologische Speziation. Vie Milieu A. 1970, 21: 363-394.Google Scholar
- Louisy P: Meeresfische: Westeuropa und Mittelmeer. 2002, Stuttgart: Ulmer VerlagGoogle Scholar
- Johnsen S: The Optics of Life: A Biologist’s Guide to Light in Nature. 2012, Princeton: Princeton University PressView ArticleGoogle Scholar
- Sugimoto M: Morphological color changes in fish: regulation of pigment cell density and morphology. Microsc Res Tech. 2002, 58: 496-503. 10.1002/jemt.10168.PubMedView ArticleGoogle Scholar
- Zarnescu O: Ultrastructure of the skin melanophores and iridophores in paddlefish Polyodon spathula. Micron. 2007, 38: 81-84. 10.1016/j.micron.2006.03.015.PubMedView ArticleGoogle Scholar
- Logan DW, Burn SF, Jackson IJ: Regulation of pigmentation in zebrafish melanophores. Pigment Cell Res. 2006, 19: 206-213. 10.1111/j.1600-0749.2006.00307.x.PubMedView ArticleGoogle Scholar
- Taylor JD, Bagnara JT: Dermal chromatophores. Am Zool. 1972, 12: 43-62.View ArticleGoogle Scholar
- Bagnara JT: Developmental aspects of vertebrate chromatophores. Am Zool. 1983, 23: 465-478.View ArticleGoogle Scholar
- Fujii R, Novales RR: Cellular aspects of the control of physiological color changes in fishes. Am Zool. 1969, 9: 453-463.PubMedView ArticleGoogle Scholar
- Collin SP, Collin HB: The morphology of the retina and lens of the sandlance, Limnichthyes fasciatus (Creeiidae). Exp Biol. 1988, 47: 209-218.PubMedGoogle Scholar
- Levy-Lior A, Pokroy B, Levavi-Sivan B, Leiserowitz L, Weiner S, Addadi L: Biogenic guanine crystals from the skin of fish may be designed to enhance light reflectance. Cryst Growth Des. 2008, 8: 507-511. 10.1021/cg0704753.View ArticleGoogle Scholar
- Goda M, Fujii R: The blue coloration of the common surgeonfish Paracanthurus hepatus—II. Color revelation and color changes. Zoolog Sci. 1998, 15: 323-333. 10.2108/zsj.15.323.PubMedView ArticleGoogle Scholar
- Bagnara JT, Fernandez PJ, Fujii R: On the blue coloration of vertebrates. Pigment Cell Res. 2007, 20: 14-26. 10.1111/j.1600-0749.2006.00360.x.PubMedView ArticleGoogle Scholar
- Kasukawa H, Oshima N: Divisionistic generation of skin hue and the change of shade in the Scalycheek Damselfish, Pomacentrus lepidogenys. Pigment Cell Res. 1987, 1: 152-157. 10.1111/j.1600-0749.1987.tb00406.x.PubMedView ArticleGoogle Scholar
- Grether GF, Kolluru GR, Nersissian K: Individual colour patches as multicomponent signals. Biol Rev. 2004, 79: 583-610. 10.1017/S1464793103006390.PubMedView ArticleGoogle Scholar
- Raposo G, Marks MS: Melanosomes-dark organelles enlighten endosomal membrane transport. Nat Rev Mol Cell Biol. 2007, 8: 786-797. 10.1038/nrm2258.PubMedPubMed CentralView ArticleGoogle Scholar
- Collin HB, Collin SP: Ultrastructure and organization of the cornea, lens and iris in the pipefish, Corythoichtyes paxtoni (Syngnathidae, Teleostei). Histol Histopathol. 1995, 10: 313-323.PubMedGoogle Scholar
- Kasukawa H, Oshima N, Fujii R: Control of chromatophore movements in Dermal Chromatic Units of Blue Damselfish .2. The Motile Iridophore. Comp Biochem Physiol C Pharmacol Toxicol Endocrinol. 1986, 83: 1-7.View ArticleGoogle Scholar
- Lythgoe JN, Shand J: Changes in spectral reflexions from the iridophores of the neon tetra. J Physiol(Cambridge). 1982, 325: 23-34.Google Scholar
- Lythgoe JN, Shand J: The structural basis for iridescent colour changes in dermal and corneal iridophores in fish. J Exp Biol. 1989, 141: 313-325.Google Scholar
- Oshima N, Fujii R: Motile Mechanism of Blue Damselfish (Chrysiptera-Cyanea) Iridophores. Cell Motil Cytoskeleton. 1987, 8: 85-90. 10.1002/cm.970080112.View ArticleGoogle Scholar
- Mäthger LM, Land MF, Siebeck UE, Marshall NJ: Rapid colour changes in multilayer reflecting stripes in the paradise whiptail, Pentapodus paradiseus. J Exp Biol. 2003, 206: 3607-3613. 10.1242/jeb.00599.PubMedView ArticleGoogle Scholar
- Mäthger LM, Hanlon RT: Malleable skin coloration in cephalopods: selective reflectance, transmission and absorbance of light by chromatophores and iridophores. Cell Tissue Res. 2007, 329: 179-186. 10.1007/s00441-007-0384-8.PubMedView ArticleGoogle Scholar
- Cloney RA, Florey E: Ultrastructure of Cephalopod Chromatophore Organs. Zeitschrift Fur Zellforschung Und Mikroskopische Anatomie. 1968, 89: 250-10.1007/BF00347297.PubMedView ArticleGoogle Scholar
- Bell GRR, Kuzirian AM, Senft SL, Mäthger LM, Wardill TJ, Hanlon RT: Chromatophore radial muscle fibers anchor in flexible squid skin. Invertebr Biol. 2013, 132: 120-132. 10.1111/ivb.12016.View ArticleGoogle Scholar
- Nagaishi H, Oshima N: Neural control of motile activity of light-sensitive iridophores in the neon tetra. Pigment Cell Res. 1989, 2: 485-492. 10.1111/j.1600-0749.1989.tb00243.x.PubMedView ArticleGoogle Scholar
- Cardona A, Saalfeld S, Schindelin J, Arganda-Carreras I, Preibisch S, Longair M, Tomancak P, Hartenstein V, Douglas RJ: TrakEM2 software for neural circuit reconstruction. Plos One. 2012, 7 (6): 7-View ArticleGoogle Scholar
- Saalfeld S, Fetter R, Cardona A, Tomancak P: Elastic volume reconstruction from series of ultra-thin microscopy sections. Nat Methods. 2012, 9: 717-10.1038/nmeth.2072. U280PubMedView ArticleGoogle Scholar
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