Alterations in melanocytic lineage cells give rise to a plethora of distinct human diseases, including neurocristopathies, cutaneous pigmentation disorders, loss of vision and hearing, and melanoma. Understanding the ontogeny and biology of melanocytic cells, as well as how they interact with their surrounding environment, are key steps in the development of therapies for diseases that involve this cell lineage. Efforts to culture and characterize primary melanocytes from normal or genetically engineered mouse models have at times yielded contrasting observations. This is due, in part, to differences in the conditions used to isolate, purify and culture these cells in individual studies. By breeding ROSAmT/mG and Tyr::CreERT2 mice, we generated animals in which melanocytic lineage cells are identified through expression of green fluorescent protein. We also used defined conditions to systematically investigate the proliferation and migration responses of primary melanocytes on various extracellular matrix (ECM) substrates. Under our culture conditions, mouse melanocytes exhibit doubling times in the range of 10 days, and retain exponential proliferative capacity for 50-60 days. In culture, these melanocytes showed distinct responses to different ECM substrates. Specifically, laminin-332 promoted cell spreading, formation of dendrites, random motility and directional migration. In contrast, low or intermediate concentrations of collagen I promoted adhesion and acquisition of a bipolar morphology, and interfered with melanocyte forward movements. Our systematic evaluation of primary melanocyte responses emphasizes the importance of clearly defining culture conditions for these cells. This, in turn, is essential for the interpretation of melanocyte responses to extracellular cues and to understand the molecular basis of disorders involving the melanocytic cell lineage.
Genetic alterations that alter survival, migration, proliferation or differentiation of embryonic neural crest cells give rise to a variety of human disorders, collectively termed neurocristopathies. The latter include pigment, skin, thyroid and hearing disorders, as well as craniofacial and cardiac abnormalities (Noisa and Raivio, 2014). Mutations in several genes implicated in neural crest cell function are responsible for various human developmental defects, such as Waardenburg syndrome, characterized by sensorineural hearing loss and pigmentation anomalies in hair, skin and irises (Baxter et al., 2004; Etchevers et al., 2006). Waardenburg syndrome accounts for about 3% of congenital deafness worldwide (Issa et al., 2017). Significantly, many of the genetic mutations associated with human neurocristopathies also occur in rodents, manifesting themselves in the form of reduced and/or altered pigmentation phenotypes.
In mice, a subset of neural crest cells adopts a melanocytic fate around E9.5-10.5, becoming melanoblasts, which begin to spread from areas adjacent to the neural tube and through the developing dermis. Melanoblasts proliferate, and interact with their microenvironment to localize to specific body sites. They migrate along a dorsolateral path towards the face, ventral abdomen and the developing limbs. In the truncal region, melanoblasts move within the dermis, and begin to penetrate into the epidermis around E11.5. Melanoblasts localize to the epidermis by E15.5 and, by E16.5, they also home in developing hair follicles (Li and Machesky, 2012; Luciani et al., 2011; Mort et al., 2015). Melanoblasts subsequently establish a melanocyte stem cell population, which can self-renew or differentiate into melanin-producing mature melanocytes postnatally (Mort et al., 2015).
Naturally occurring mouse coat color mutants have provided valuable information regarding the pathways that regulate melanocytic cell specification, proliferation, survival, migration and stem cell renewal (Baxter et al., 2004). For example, in heterozygous dominant megacolon mice, white spotting is evident. This phenotype arises from a point mutation in the Sox10 gene, which introduces a premature stop codon. Sox10 activates Mitf transcription, functions during melanocyte specification, and maintains melanocyte-specific gene expression later in development (Herbarth et al., 1998; Wegner, 2005). Genetically engineered mutant mouse models that use Cre recombinase-mediated targeting of genes in pigment-producing cells have also been generated and used to examine the roles of many genes in melanocytic cell specification, homing, maturation and survival. Amongst them are included transgenic lines that express Cre or Cre fused to a modified estrogen receptor (CreERT2) under the control of the Mitf, Tyr, Dct, Tyrp1 or MART-1 (Melan-A) promoter (Alizadeh et al., 2008; Aydin and Beermann, 2011; Bosenberg et al., 2006; Colombo et al., 2007; Delmas et al., 2003; Guyonneau et al., 2002; Mori et al., 2002). Some of these transgenes additionally target non-melanocytic cells; others express Cre at low levels, whereas in tamoxifen-inducible Cre lines, targeting of relatively small fractions of cells is often observed. For example, in Dct::Cre mice, melanoblasts and melanocyte stem cells are targeted, as well as cells in the telencephalon (Guyonneau et al., 2002). Tyrp1::Cre mice exhibit Cre expression in retinal pigmented epithelium and, ectopically, in the neural retina (Mori et al., 2002), and the efficiency of tamoxifen induction of Cre-mediated recombination can range from 12% to >80% (Bosenberg et al., 2006). The development of mouse genetic tools and imaging approaches that exploit the properties of fluorescent proteins specifically expressed in the melanocytic lineage, and which allow in vivo and ex vivo studies of melanocytic cell characteristics, as well as molecular studies of melanocytic cell behavior, has been more limited (Colombo et al., 2012; Li et al., 2011; Woodham et al., 2017). Moreover, the use of melanocytic cells cultured under a variety of conditions, together with studies using melanoma tumor cells as surrogates to model normal melanocytic cells, can yield contrasting information and significantly complicate the elucidation of cellular and molecular processes important in these cells. In an effort to address this void, we have bred ROSAmT/mG and Tyr::CreERT2 mice, generating animals in which melanocytic lineage cells are identified through expression of green fluorescent protein. We have also defined the growth characteristics of primary melanocytes isolated from mouse epidermis, and now describe the diverse responses of these cells to various extracellular matrix substrates. Our models will facilitate a more systematic exploration and understanding of melanocytic lineage cell biology, and its alterations in various human pigmentation disorders and neurocristopathies.
Generation of a melanocytic lineage reporter mouse model for cell fate mapping
Melanocytes arise from precursor melanoblasts, which begin to migrate from the mouse neural crest at embryonic day (E)9.5, and by E16.5 are found in both the epidermis and the hair follicles (Luciani et al., 2011; Mort et al., 2015). We have generated a reporter mouse model that allows tracing of melanoblasts and their progeny to better examine the processes involved in melanoblast migration, survival and differentiation into pigment-producing melanocytes. These animals, hereafter termed Tyr::CreERT2-mT/mG, have been bred into a reporter ROSAmT/mG background and express specifically in cutaneous melanocytic cells Cre recombinase fused to a modified estrogen receptor (CreERT2) under the control of the Tyr promoter, beginning at E10.5 (Bosenberg et al., 2006; Muzumdar et al., 2007). Tamoxifen administration to these mice activates CreERT2 and induces expression of a membrane-targeted form of green fluorescent protein (mGFP). Non-targeted cells constitutively express mTomato, a membrane-targeted red fluorescent protein form. Analysis of E20.5 skins harvested from embryos exposed to tamoxifen at E11.5 days revealed mGFP immunoreactivity detected exclusively in a subpopulation of cells in the hair follicle (Fig. 1A) and in the interfollicular epidermis (data not shown). These cells also expressed the melanocytic-specific enzyme dopachrome tautomerase (DCT), confirming the melanocytic origin of the targeted cells (Fig. 1B). No detectable recombination was observed in embryos from dams treated with vehicle only (data not shown).
Characteristics of cultured melanocytes
The isolation of primary melanocytes and their culture to high purity is a prerequisite for thorough cellular and molecular characterization of biological processes in melanocytic lineage cells. We generated single-cell suspensions from newborn Tyr::CreERT2-mT/mG mouse epidermis mainly composed of melanocytes and keratinocytes. The cells were cultured in selective growth medium supplemented with endothelin-3 (ET-3), which we found favored melanocyte growth. 48 h after isolation, we observed mixed cultures composed of 9% tyrosinase-related protein 1 (TRP1)-positive melanocytic cells, which increased to 29% after 6 days, as the culture conditions did not allow contaminating keratinocytes to proliferate (Fig. 2A). Through the combination of differential trypsinization (Huang et al., 2013) and serial passaging, we increased the proportion of melanocytes in the cultures to 69% and >95%, respectively, after the first and second passages (Fig. 2A). The cultures maintained >95% purity from passages 2 through 6 (data not shown). The identity of melanocytic cells in these cultures was further confirmed by their ability to oxidize L-DOPA to a dark brown pigment (Fig. 2A). Analysis of melanocytic cell markers demonstrated detectable levels of Kit, Mitf-M, Sox10, Tyr and Trp1 transcripts in these cultures as early as passage (P)1 (Fig. 2B). The abundance of these markers increased with the purity of the cultures, and was maintained for as long as 60 days, the last time analyzed corresponding to P6 cells (Fig. 2B).
We next determined the growth characteristics of the cultured melanocytes. We observed that P2 and P3 cultures maintained normal proliferation as late as 28 days after plating, and exhibited doubling times of about 10 days (Fig. 2C). In contrast, little if any cell growth was observed in cultures at P4, P5 and P6 (Fig. 2C). Thus, under our culture conditions, primary melanocytes remain exponentially proliferative as late as 50 days following initial isolation. Significantly, whereas the average melanin content of P2 and P3 cultures was 54.3 and 66.7 µg/106 cells, respectively, it increased almost threefold in P4 and P6 cultures, coinciding with pronounced morphological changes characterized by reduced nucleus:cytoplasm surface ratios and increased size, changes typical of senescent cells (Fig. 2D; Fig. S1). Mouse melanocytes escape senescence through inactivation of Cdkn2a, which encodes the cyclin-dependent kinase inhibitor p16Ink4a. Significantly, the reduction in proliferative capacity and development of senescence we observed in higher passage melanocytes was not accompanied by increases in Cdkn2a transcripts. Based on the observed growth characteristics of these cells, all subsequent experiments were conducted with >95% pure P2 or P3 cultures.
Effect of extracellular matrix substrates on mouse melanocyte dendricity
Melanocytes in situ interact with extracellular matrix (ECM) proteins in the skin basement membrane through proteins that include integrins α3β1, α6β1 and αvβ1. In culture, human primary melanocytes additionally express integrins α5β1 and αvβ3 (Hakkinen et al., 2001), which allow them to interact with substrates such as fibronectin, collagen and laminins. In embryonic and in postnatal intact epidermis, melanocytes interact with a basement membrane mainly composed of laminin-332. On the other hand, melanocytes, keratinocytes and fibroblasts in wounded epidermis play important roles in wound healing and subsequent scar formation. In particular, melanocytes can mitigate keratinocyte-dependent contraction in co-culture models of wounds composed of fibroblasts, keratinocytes and melanocytes in the presence of collagen I. Melanocytes may thus contribute to reducing the formation of fibrotic scars through interactions with collagen I, a major ECM substrate found in wounded skin (Rakar et al., 2015). In an effort to better understand melanocyte responses to ECM substrates, we next addressed whether melanocytes exhibit different responses when stimulated by laminin-332 or collagen I. Because laminin-binding integrins can mediate cellular responses distinct from those elicited by fibronectin- or collagen-binding integrins, we first compared the morphology and ability of primary mouse melanocytes to migrate on no exogenous ECM, low or intermediate concentrations of collagen I (5 µg/cm2 or 15 µg/cm2), or laminin-332 isolated from 804G rat bladder epithelial cells. Cells cultured in the absence of exogenous ECM were able to spread, frequently exhibiting polygonal morphologies with or without formation of dendrites (Fig. 3A). In contrast, melanocytes seeded on collagen adopted an elongated, and frequently bipolar, morphology (Fig. 3A and data not shown). The presence of laminin-332 induced formation of extensive and frequently branched dendritic extensions (Fig. 3A). Quantification of the fraction of cells that exhibited a spread, bipolar or dendritic phenotype revealed that in the absence of exogenous matrices about 40% of cells were either spread or dendritic and in the presence of 15 µg/cm2 collagen I, about 50% of the cells were bipolar, whereas 87% of melanocytes seeded on laminin-332 were dendritic (Fig. 3B). Of note, laminin-332 also increased significantly the average number of dendrites per cell. Specifically, only 6% and 25% of cells seeded without exogenous ECM or on collagen, respectively, showed >3 dendrites/cell, whereas almost 45% of cells in contact with laminin-332 formed >3 dendritic extensions (Fig. 3C). Thus, primary mouse melanocytes exhibit differential responses to various ECM substrates, and their interaction with laminin-332 appears to promote the formation of dendritic processes. The optimal formation of dendrites is essential for normal interactions between melanocytes and adjacent keratinocytes in the epidermis.
Effect of ECM substrates on melanocyte motility
In addition to regulating morphology, integrins enable melanocytes to interact with and migrate on ECM substrates (Pinon and Wehrle-Haller, 2011). To assess the effect of collagen and laminin on motility, we seeded melanocytes at single-cell densities and followed their movement for 16 h using time-lapse video microscopy. Plots of cell trajectories revealed substantial differences in melanocyte motility, depending on the underlying substrate. Cells seeded in the absence of exogenous ECM or on collagen I (15 µg/cm2) displayed average speeds of 0.12 µm/min and 0.05 µm/min, respectively. The presence of laminin-332 increased cell speed four- to ninefold, to 0.47 µm/min (Fig. 4A,B). Over 75% of cells plated without exogenous ECM or on collagen I exhibited speeds lower than 0.2 µm/min. In stark contrast, 90% of cells seeded on laminin-332 showed speeds that exceeded 0.2 µm/min (Fig. 4C). In agreement with the stimulatory effects of laminin-332 on melanocyte speed, we also observed an increase in mean accumulated distance migrated during the course of this experiment to about 450 µm, compared with 48 µm for cells plated on collagen, and 112 µm in cells plated without exogenous ECM, representing a fivefold increase (Fig. 4D). Further analysis revealed that in the presence of collagen, up to 85% of cells did not migrate distances greater than 100 µm, whereas laminin-332 promoted migration distances greater than 200 µm in 85% of melanocytes (Fig. 4E). We conclude that, in the concentrations used in these studies, laminin-332 promotes, whereas collagen appears to hamper, random melanocyte motility.
The distinct effects of collagen and laminin-332 on random melanocyte motility prompted us to investigate their effects on directional migration, using scrape-wound assays. We evaluated the cell-free surface area remaining at timed intervals after wounding. Within one and three days after wounding, cells plated on laminin-332 had covered 40, 65 and 80% of the wound area in 1, 3 and 6 days, respectively (Fig. 5). By comparison, those melanocytes without exogenous ECM had covered 22, 40 and 60% of the original denuded area 1, 3 and 6 days after wounding (Fig. 5). In stark contrast, cells plated on collagen I (15 µg/cm2) had barely covered about 35% of the cell-free area as late as 6 days following wounding (Fig. 5). Together our data show that laminin-332, but not collagen I, induces random motility and directional migration in primary mouse melanocytes.
Through the combined use of a transgenic mouse strain that specifically expresses Cre recombinase in cutaneous melanocytic lineage cells (Bosenberg et al., 2006), together with the ROSAmT/mG double fluorescent protein reporter background, we were able to efficiently trace Cre-targeted embryonic melanocytes both in interfollicular epidermis and in the developing hair follicles. The presence of mGFP allows the simultaneous analyses by immunofluorescence microscopy of multiple proteins within a clearly identified targeted melanocytic cell, an approach that has remained difficult with various other melanocytic reporter mouse models. Following in utero induction at E11.5, the fraction of mGFP-positive cells observed in E20.5 embryos constituted about 10-30% of DCT-positive melanocytes, in line with the targeting efficiency reported for the original Tyr::CreERT2 transgenic mouse line (Bosenberg et al., 2006).
Melanocytes derive from multipotent neural crest cells, after they delaminate from the dorsal neuroepithelium, and are thought to arise from two different developmental waves (Baggiolini et al., 2015; Mort et al., 2015). The first wave of cutaneous melanocytes arises directly from neural crest cell-derived progenitors that first migrate dorsolaterally, and then ventrally through the dermis to finally populate the epidermis and hair follicles (Adameyko et al., 2009). In these cells, the genes encoding tyrosinase, TRP-1 and dopachrome tautomerase, three major enzymes involved in the synthesis of melanin, are expressed shortly after E9 (Steingrimsson et al., 2004). A second subset of melanocytes arises later, from neural crest-derived Schwann cell progenitors found along the ventral pathway (Nitzan et al., 2013), which express MITF, TYR, and TRP-1 later than those directly derived from neural crest cells (Adameyko et al., 2009; Mort et al., 2015). Administration of tamoxifen at E10-11.5 to our reporter mice allows selective labeling of the first wave of migrating melanoblasts, excluding those generated later from Schwan cell precursors.
In culture, we have observed that 4-hydroxytamoxifen treatment results in activation of mGFP expression in ≥80% of melanocytes (data not shown), whereas no mGFP-positive cells are observed in untreated or vehicle-treated cultures. Our model thus demonstrates tight spatial and temporal regulation of genetic recombination in melanocytic cells. The generation of pure primary melanocyte cultures is challenging, as they constitute only 3-7% of all epidermal cells (Hsu et al., 2005). Several reports describing a variety of growth conditions for human and mouse melanocytes exist, including the use of phorbol ester and cholera toxin, which yield cultures with doubling times of about 5 and 12 days, respectively (Eisinger and Marko, 1982). Neonatal mouse melanocytes have been successfully cultured in medium containing placental extracts (Larue et al., 1992), or in the presence of keratinocyte feeder layers (Godwin et al., 2014). For our studies, we used melanocyte growth medium supplemented with ET-3, which was found to improve plating efficiency and cell growth (data not shown).
Under our culture conditions, mouse melanocytes in a C57/BL6 strain background retain full proliferative capacity for up to 7-9 weeks following isolation, with a doubling time of about 10 days. Although our studies did not measure the number of cell doublings that occurred in mixed melanocyte-keratinocyte cultures prior to P2, we estimate that the primary melanocyte cultures remain proliferative during approximately 9-10 population doublings, at which time they senesce. In the presence of keratinocyte feeder layers, primary mouse melanocytes reportedly exhibit doubling times of about 4-5 days, and become senescent after 4-5 weeks in culture (Sviderskaya et al., 2002). Notably, immortalization of mouse melanocytes through spontaneous or targeted inactivation of the Cdkn2a locus yields cells with doubling times as low as 2.3 days, which, however, also display substantially reduced melanogenic capacity (Sviderskaya et al., 2002), potentially as a result of increased genetic instability (Fung et al., 2013). Thus, our isolation and culture conditions allow for expansion and characterization of mouse melanocytes without the need of feeder layers and, because they retain full capacity to produce melanin, they are ideal to investigate the consequences of targeted genetic manipulations on melanogenic functions.
In intact epidermis, melanocyte adhesion to the basement membrane involves binding of α6β1 integrins to laminin-332 secreted by neighboring epidermal keratinocytes, as well as interactions with collagen IV and collagen XVII (Hara et al., 1994; Tanimura et al., 2011). In culture, laminin-111 and collagen IV also promote formation of dendrites in human melanocytes, whereas fibronectin or vitronectin induce bipolar or polygonal morphologies. We now show that mouse melanocytes exhibit substantially different responses to laminin-332 and collagen I, developing numerous dendrites in the presence of the former, but not the latter ECM substrate. Further, the characterization and interpretation of primary cultured melanocyte responses on a given ECM substrate, such as laminin-332, may also be critically dependent on the origin of the ECM tested. Further, different maturation/processing products can induce distinct adhesive and/or migratory cellular responses (Rousselle and Beck, 2013). Laminin-332 is synthesized by epidermal keratinocytes and other epithelial cells as a 460-kDa precursor protein, which is secreted into the ECM milieu and subsequently processed into smaller forms (Rousselle and Beck, 2013), and laminin-332 from rat bladder epithelial 804G cells differs from that secreted by SCC25 squamous carcinoma cells or HaCaT immortalized human keratinocytes (Scott et al., 1999; Zhang et al., 2013). Functionally, laminin-332 from 804G cells is vastly superior in supporting adhesion and clonal growth of primary human melanocytes than HaCaT-derived laminin-332 (Scott et al., 1999; Zhang et al., 2013). Similarly, whereas we observed pronounced positive effects of 804G-derived laminin-332 on both random and directional migration in our melanocyte cultures, SCC25-derived laminin-332 matrix failed to stimulate random migration in human melanocytes (Scott et al., 1999).
Functional differences also exist between laminin- and collagen-binding integrins (Stipp, 2010). For example, responses of epithelial cells to laminins frequently involve strong activation of Rac1 and Cdc42, which induce formation of lamellipodia and filopodia, respectively, as well as formation of smaller focal contacts and a dynamic actin cytoskeleton that promotes rapid migration. In contrast, responses to collagen or fibronectin are frequently associated with RhoA activation, formation of robust stress fibers and focal adhesions (Stipp, 2010). Cell motility and adhesion are also influenced by ECM substrate concentration. For example, high concentrations of fibronectin or collagen (>30 µg/cm2) promote cell adhesion and spreading, and inhibit formation of cell protrusions and forward movement. Conversely, intermediate concentrations (5-10 µg/cm2) provide optimal levels of cell-matrix adhesion and ability to form protrusions, which facilitate migration (Cox et al., 2001; Gehler et al., 2017). Although melanocytes are not epithelial in origin, we similarly observed optimal migration on laminin-332 matrix, compared to intermediate concentrations of collagen I. However, unlike epithelial and mesenchymal cells, primary melanocytes did not display a spread morphology when cultured on collagen I, but rather adopted a long bipolar morphology with reduced dendrite formation, and occupied smaller surface areas than those seeded on laminin or without exogenous ECM. Primary melanocytes are known to shed melanosomes primarily through dendritic extensions (Wu and Hammer, 2014), although shedding events can also be induced from central areas in cells seeded on collagen-rich substrates (Wu et al., 2012). Given the effects of various extracellular matrices on melanocyte morphology and dendricity, an important area of future research will be to systematically examine the effect of ECM substrates on the diverse pathways that modulate melanosome shedding by melanocytes and their uptake by neighboring epidermal keratinocytes.
In conclusion, we have developed a mouse model for in vivo tracing of melanocytic lineage cells. We have also developed efficient isolation and culture methods to systematically examine the characteristics of mouse primary melanocytes and their responses to various ECM substrates. Our studies underline the importance of clearly defining culture conditions and cell passage number during characterization of melanocyte biological processes. The combined use of our mouse reporter model and our clearly defined and characterized culture systems will provide valuable tools to decipher the cellular and molecular mechanisms that regulate melanocytic cell behavior, and how their alterations may contribute to neurocristopathies and pigmentation disorders.
MATERIALS AND METHODS
All animal experiments were approved by the University of Western Ontario Animal Care Committee (Protocol No. 2016-022), in accordance with regulations and guidelines from the Canadian Council on Animal Care. The mice used for these studies express Cre recombinase fused to a modified estrogen receptor under the control of the Tyr promoter (Bosenberg et al., 2006). For in vivo lineage tracing studies, these mice were bred to homozygosity with mice containing ROSAmT/mG Cre reporter allele background (Muzumdar et al., 2007). Genotyping was conducted as previously described (Sayedyahossein et al., 2015). To induce Cre recombinase activation, tamoxifen (1 mg/25 g body weight dissolved in ethanol:Cremophore:PBS 1:1:5 v/v) was administered intraperitoneally once to 11.5 days post-coitus (dpc) pregnant dams. 0.5 dpc for timed pregnancies was considered to be at midday of the day vaginal plugs appeared. In vivo tracing studies were conducted with 3-5 embryos from at least two litters.
Reagents and antibodies
Rat tail Collagen Type I (354236) was from Corning Inc. (NY, USA), endothelin-3 (CC-4510) was purchased from Lonza (Walkersville, MD, USA), Permount mounting medium (SP15-100) was from Fisher Scientific (Ottawa, Ontario, Canada). Cremophor (Kolliphor EL; C-5135), L-DOPA (59-92-7), synthetic melanin (M8631) and all other chemicals were purchased from Sigma (St. Louis, MO, USA). Antibodies purchased from Abcam (Cambridge, UK) were: Mouse anti-TRP1 [cat. no. 3312, lot no. GR239310-1, diluted 1:200 in phosphate-buffered saline (PBS) containing 5% goat serum] (Delevoye et al., 2009) and chicken anti-GFP (cat. no. 13970, lot no. GR279236-1, diluted 1:1000 in PBS containing 5% goat serum) (Jackson et al., 2015). The rabbit anti-keratin 14 antibody (cat. no. CLPRB-155P, lot no. D14IF01918, diluted 1:1000 in PBS containing 5% goat serum) (Jackson et al., 2015) was from Covance (Cranford, NJ, USA). The goat polyclonal anti-DCT antibody (cat. no. 10452, lot no. 10616, diluted 1:100 in PBS containing 5% donkey serum) (Smith et al., 2013) was purchased from Santa Cruz Biotechnology (CA, USA). Alexa Fluor®-conjugated goat anti-mouse and goat anti-rabbit IgG were purchased from Molecular Probes/Invitrogen (Eugene, OR, USA).
Primary melanocyte culture and proliferation measurements
Melanocytes from all experiments were isolated from animals not exposed to tamoxifen. Skin was harvested from 3-day-old mice of both sexes and digested with Dispase II (5 U/ml, 4942078001, Roche, Switzerland) for 1.5 h at 37°C. The epidermis was mechanically separated, minced and digested with a 0.025% Trypsin/ 0.01% EDTA solution (R-001-100, Thermo Fisher, Carlsbad, CA, USA) for 10 min at 37°C, with gentle rocking. Two volumes of trypsin neutralizer solution (R002100, Thermo Fisher) were added, and a cell suspension was obtained by thorough mixing. Tissue debris and cornified envelope fragments were removed by filtration through a 100-µm pore size nylon strainer (08-771-19, Corning Inc.), and the resulting cell suspension was centrifuged (200×g, 10 min, 22°C). Pelleted cells were suspended in MBM-4 medium (CC-4435, Lonza) supplemented with endothelin-3 (260 ng/ml, final) and growth factors (CC-4435, Lonza), and seeded at a density of 1×105 cells/cm2. The growth medium was replaced one day after plating, and subsequently every 72 h. The cultures were consistently maintained at 30-90% confluence. Where indicated, cell culture surfaces were coated with rat-tail Collagen Type I (15 µg/cm2) or laminin-332 matrix obtained from 804G rat bladder squamous carcinoma cell conditioned medium (Tripathi et al., 2008). To this end, confluent 804G cultures were rinsed with PBS, and maintained in serum-free Eagle's Minimum Essential Medium for 48 h. The spent medium was filtered to remove cell debris, and used to coat culture surfaces by incubation at 37°C for 1-2 h prior to plating melanocytes. For proliferation measurements, triplicate samples from independent cell isolates were seeded at a density of 15,000 cells/well in 24-well culture dishes. Cell numbers were determined weekly from trypsinized cultures. Unless otherwise indicated, all experiments were conducted with melanocytes passaged 2-3 times.
Immunohistochemistry and immunofluorescence microscopy
Paraffin-embedded 7-µm sections of skin harvested from E20.5 embryos were deparaffinized and subjected to high-temperature antigen retrieval, with 10 mM sodium citrate (pH 6.0), followed by incubation with primary antibodies, as described (Rudkouskaya et al., 2014). For histological visualization of melanin, tissue sections were treated with Fontana-Masson stain (150669, Abcam) and counterstained with Nuclear Fast Red, following the manufacturer's instructions. For indirect immunofluorescence microscopy analyses of cultured melanocytes, cells were fixed in freshly diluted 4% paraformaldehyde (PFA), and processed as described (Ivanova and Dagnino, 2007; Sayedyahossein et al., 2015). Fluorescence and phase-contrast micrographs were obtained with a Leica DMIRBE fluorescence microscope equipped with an ORCA-ER digital camera (Hamamatsu Photonics, Hamamatsu, Japan), using Volocity 6.1.1 software (Improvision, Coventry, UK).
Light and time-lapse video microscopy
Time-lapse video microscopy images were obtained with a Leica DMIRBE fluorescence microscope equipped with an ORCA-ER digital camera (Hamamatsu Photonics), using Volocity 6.1.1 software (Improvision). Light microscopy images of tissue sections were obtained with a Leica DM-LRE2 microscope equipped with a ProgRes C5 camera (Jenoptik Optical Systems, Jupiter, Florida, USA) and ProgRes Mac CapturePro 2.7.6 (Jenoptik) imaging software.
L-DOPA reaction assays were conducted as described (Tsuchiyama et al., 2013). Briefly, cultured melanocytes were fixed in freshly diluted 4% PFA at 22°C for 20 min. The cells were rinsed thrice with phosphate-buffered saline (PBS), and were then incubated with 5 mM L-Dopa diluted in PBS (pH 6.8) at 37°C for 4 h, protected from light. After incubation, the cells were rinsed with water and mounted with Permount.
Melanin quantification was conducted as described (Flori et al., 2011). Melanocytes (5×105 cells) were trypsinized from 60-mm culture dishes. An aliquot of this cell suspension was used to determine the number of cells present, and the remainder was centrifuged (200×g, 10 min, 22°C). The cell pellet was suspended and lysed in an aqueous solution of 1 M NaOH containing 10% DMSO, which was incubated at 80°C for 1 h with vigorous shaking. The lysates were clarified by centrifugation (12,000×g, 20 min, 22°C), and the melanin content in the lysate was determined from absorbance measurements at 420 nm, interpolating the values obtained with those from a synthetic melanin standard curve. The results were normalized to cell number.
RNA isolation and qPCR
Total RNA was isolated using RNeasy microkits (Qiagen, Louisville, KY, USA), following the manufacturer's instructions. RNA quality was determined with an Agilent 2100 Bioanalyzer (Agilent, Santa Clara, CA, USA). RNA samples (200 ng) with integrity numbers ≥8.5 were subjected to reverse transcription (SuperScript II RT, Fisher Scientific), following the manufacturer's protocol. Quantitative, real-time polymerase chain reactions (qPCR) were conducted on a CFX384 Real-Time PCR system (Bio-Rad, Hercules, CA, USA) operated by CFX Manager software (version 1.6). cDNA samples corresponding to 20 ng of RNA were amplified using PerfeCTa qPCR SuperMix (Quanta BioSciences, Gaithersburg, MD, USA) as described (Singh and Dagnino, 2016), and using the following primers (400 nM, final): Tyrp1 forward (F) 5′-GCCTTCTTTCTCCCTTCCTTAC-3′ and reverse (R) 5′-CTGCTGGTCTCCCTACATTTC-3′; Tyr (F) 5′-CTCTGGGCTTAGCAGTAGGC-3′ and (R) 5′-GCAAGCTGTGGTAGTCGTCT-3′; Kit (F) 5′-CCTCCTGCCCTTTATCCTTTAG-3′ and (R) 5′-GACCTCCAAACCAGCTTACTT-3′, Sox10 (F) 5′-AGCCCTCAGGACCCTATTAT-3′ and (R) 5′-GTCAGAGATGGCAGTGTAGAG-3′, Cdkn2a (F) 5′-GCTGGGTGGTCTTTGTGTA-3′ and (R) 5′TTAGCTCTGCTCTTGGGATTG-3′. The Mitf (F) 5′-GAAAGTAGAGGGAGGAGGACTAA-3′ and (R) 5′-GCACCTGGTAGTGACTGTATTC-3′ primers allow amplification of the melanocyte-specific transcript variant 2, which encodes MITF-M. The results were normalized to the expression of the Rpl16 and Rps29 genes, which encode ribosomal protein L16 and S29, respectively (de Jonge et al., 2007). Replicate cDNA samples were amplified for 40 cycles (98°C for 10 s, and 58°C for 30 s per cycle). Primer specificity and amplicon sizes were confirmed, respectively, by analysis of melt curves conducted between 65°C and 95°C, in 0.5°C increments and agarose gel electrophoresis. Relative mRNA levels were calculated using the ΔΔCq method. RNA preparations obtained from three different cell isolates were analyzed.
For single-cell motility analyses, melanocytes were seeded at 2×104 cells/35-mm μ-Dish culture dish (81156; Ibidi USA, Madison WI, USA). Time-lapse video microscopy images were obtained 24 h after plating, and cells were manually tracked using the Manual Tracking plugin for ImageJ software (version 1.49v, Fiji, NIH). The velocity, accumulated and Euclidean distances of each cell were calculated using the ‘Chemotaxis and Migration Tool’ plugin for ImageJ (version 1.01). At least 20 cells/condition were tracked in individual experiments. To assess directional migration, scrape-wound assays were conducted as described (Vi et al., 2011), with minor modifications. Melanocytes were seeded onto 24-well culture dishes with no exogenous ECM, or coated laminin-332 matrix, at a density of 1×105 cells/ well. Alternatively, the cells were seeded at a density of 1.5×105 cells/well on Collagen Type I-coated dishes (15 µg/cm2). 24 h later, a scrape wound was created with a sterile 200-µl pipette tip. The cell monolayer was rinsed with PBS to remove cell debris and cultured in growth medium. Changes in gap surface area were determined from phase-contrast micrographs obtained at timed intervals following wounding, using ImageJ software.
Data were analysed using one- or two-way ANOVA, as indicated in individual experiments, with post hoc Tukey's correction. Significance was set at P<0.05. Experiments with cultured melanocytes were conducted in triplicate samples, and at least three times with independent cell isolates.
We thank K. Barr for expert technical assistance, and Dr I. Ivanova for critical reading of the manuscript.
Conceptualization: M.C., L.D.; Methodology: M.C., V.L., L.D.; Validation: L.D.; Formal analysis: M.C., L.D.; Resources: L.D.; Data curation: L.D.; Writing - original draft: M.C., L.D.; Writing - review & editing: L.D.; Supervision: L.D.; Project administration: L.D.; Funding acquisition: L.D.
During portions of this work, M.C. was supported by an Internal Grant (grant no. F0588) from the Lawson Health Research Institute, awarded to M.C. and L.D. V.L. was supported by a ‘Dean's Undergraduate Research Opportunities Program’ studentship from the Schulich School of Medicine and Dentistry (The University of Western Ontario). This work was supported by funds to L.D. from the Canadian Institutes of Health Research and the Natural Sciences and Engineering Research Council of Canada (grant nos FRN 119303 and RGPIN-2017-04765, respectively).
The authors declare no competing or financial interests.