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  • Research article
  • Open Access

Transcripts within rod photoreceptors of the Zebrafish retina

BMC Genomics201819:127

https://doi.org/10.1186/s12864-018-4499-y

  • Received: 25 July 2017
  • Accepted: 28 January 2018
  • Published:

Abstract

Background

The purpose of this study was to identify transcripts of retinal rod photoreceptors of the zebrafish. The zebrafish is an important animal model for vision science due to rapid and tractable development, persistent neurogenesis of rods throughout the lifespan, and capacity for functional retinal regeneration.

Results

Zebrafish rods, and non-rod retinal cells of the xops:eGFP transgenic line, were separated by cell dissociation and fluorescence-activated cell sorting (FACS), followed by RNA-seq. At a false discovery rate of < 0.01, 597 transcripts were upregulated (“enriched”) in rods vs. other retinal cells, and 1032 were downregulated (“depleted”). Thirteen thousand three hundred twenty four total transcripts were detected in rods, including many not previously known to be expressed by rods. Forty five transcripts were validated by qPCR in FACS-sorted rods vs. other retinal cells. Transcripts enriched in rods from adult retinas were also enriched in rods from larval and juvenile retinas, and were also enriched in rods sorted from retinas subjected to a neurotoxic lesion and allowed to regenerate. Many transcripts enriched in rods were upregulated in retinas of wildtype retinas vs. those of a zebrafish model for rod degeneration.

Conclusions

We report the generation and validation of an RNA-seq dataset describing the rod transcriptome of the zebrafish, which is now available as a resource for further studies of rod photoreceptor biology and comparative transcriptomics.

Keywords

  • Rod photoreceptor
  • Retina
  • Transcriptome
  • RNA-Seq
  • Zebrafish
  • Regeneration

Background

Within the vertebrate neural retina, photoreceptor cells are the sensory neurons that detect photons and convert this physical information into electrochemical signals. Rod photoreceptors contain the visual pigment rhodopsin, are highly sensitive to light, and provide predominantly convergent information to downstream neurons to maximize light detectability in low-light situations. Cone photoreceptors contain cone visual pigments (cone opsins) with distinct peak spectral sensitivities, and provide convergent and divergent information to downstream neurons, which process differential input to discriminate color and provide high acuity vision. Photoreceptors display distinctive morphologies with specialized apical projections, the outer segments, which are highly modified nonmotile cilia [1]. Outer segments include membranous disks to increase surface area for containing opsins and other phototransduction proteins, and photoreceptors maintain these outer segments with a high rate of protein synthesis, together with mechanisms for selective protein targeting and trafficking [2]. Rod photoreceptors in humans are particularly sensitive to genetic changes in structural and functional components; such defects cause hereditary retinal degenerations, which typically involve rod cell death, followed by cone cell death and loss of vision [3]. There is therefore great interest in increasing our depth of understanding of rod photoreceptor biology, health, the factors leading to cell death, and the discovery of strategies for promoting rod survival and/or rod replacement.

The zebrafish, an important animal model in vision research, is an example of a vertebrate with the endogenous capacity for rod replacement [4]. The zebrafish retina grows throughout its lifespan through the addition of new neurons at the retinal periphery, called the circumferential germinal zone (CGZ) or ciliary marginal zone (CMZ) [57]. In addition, Müller glia throughout the growing retina divide at a slow rate, generating a transiently-amplifying population of rod progenitors that migrate to the photoreceptor layer, and divide to generate rod photoreceptors [8]. The zebrafish retina therefore accumulates rods over its lifespan from these dedicated rod lineages. In zebrafish models of rod degeneration, either the most immediate precursors within the photoreceptor layer accelerate the production of new rods [9, 10], or the progenitor lineage is stimulated to increase rod neurogenesis to replace rods lost to damage [10]. In response to more widespread retinal damage due to chemical trauma, the progenitors generated by cell division of Müller glia gain the capacity to regenerate other types of retinal neurons [1114], ultimately resulting in restoring visual function [11, 15]. The existence of the rod lineage is well-documented in zebrafish [8, 16, 17], and in other teleosts [1820], and holds promise to inform the development of rod replacement strategies to treat human retinal disease. However, our knowledge of rods, and the rod lineage, within the zebrafish remains limited to a small number of rod-specific markers (primarily phototransduction components) [21], and a network of transcription factors important for rod determination and differentiation [5, 16, 2225]. A single, distinctive marker for cells of the dedicated lineage that generates new rods, other than incorporation of S-phase markers, remains surprisingly elusive.

In the present study, we begin to fill this knowledge gap through RNA-sequencing (RNA-seq) analysis of the transcriptome of isolated rod photoreceptors, in comparison with non-rod retinal cells. In the transgenic line xops:eGFP, rod photoreceptors exclusively express high levels of GFP [26], permitting enrichment of rods from other retinal cells by fluorescence-activated cell sorting (FACS). This approach revealed transcripts that were upregulated in rods vs. other retinal cells, those that were present in rods but not differentially expressed, and those that were downregulated in rods vs. other retinal cells. Quantitative PCR (qPCR) studies suggested that this transcriptome is remarkably stable over the zebrafish lifespan from larval to adult ages, and appeared similar in rods that had regenerated following a chemical lesion. The zebrafish rod transcriptome is now a resource that can be mined for the identification of novel structural and functional components of rods, and possibly their progenitors, and for future comparative analyses with transcriptomes of rods and/or cones from key model organisms.

Methods

Animals and tissue preparation

All procedures involving animals were carried out in compliance with protocols approved by the University of Idaho Animal Care and Use Committee. Zebrafish (Danio rerio) were maintained on a 14:10 light:dark cycle in recirculating, monitored system water, housed and propagated according to [27]. For this study we used the xops:eGFP transgenic line, in which the Xenopus rod opsin promoter drives expression of eGFP exclusively in rod photoreceptors [26], the gift of James Fadool, and a wild-type strain originally obtained from Scientific Hatcheries (now Aquatica Tropicals). In addition we used the xops:mCFP transgenic line, the gift of Ann Morris. In this line, the presence of mCFP in retinal rods leads to rapid rod degeneration, and a proliferative response to this degeneration by the rod precursor population [9].

To obtain retinal tissues for fluorescence-activated cell sorting (FACS), xops:eGFP fish were dark-adapted for 10–12 h to facilitate removal of retina from the RPE, anaesthetized with MS-222, and eyes enucleated with fine forceps. Corneas and lenses were removed, and retinas were peeled free from the RPE and whole eyecup in saline. In some cases, as indicated in Results, we used whole adult (1.5 yrs), juvenile (1 month), or larval (14 days post-fertilization; dpf) retinas for FACS and quantitative RT-PCR (qPCR). In all cases, animals were dark-adapted prior to retina removal, and in all cases, RNA isolation was performed immediately following tissue collection or FACS.

Tissues for in situ hybridization were fixed in phosphate-buffered, 4% paraformaldehyde containing 5% sucrose for 1 h at room temperature, and washed in phosphate-buffered 5% sucrose, and then a graded series ending in 20% sucrose for overnight cyroprotection at 4 °C. Tissues were embedded in a 1:2 solution of OCT embedding medium (Sakura Finetek) and phosphate-buffered, 20% sucrose, and frozen in isobutane supercooled with liquid N2. After freezing solid, tissues were sectioned at 5 μm on a Leica CM3050 cryostat [15, 28].

Cell dissociation and FACS

Whole retinas were dissociated into cell suspensions by incubating with 0.225% trypsin (Fisher ThermoScientific) and 0.001% papain (Worthington Biochemical) for 10 min at 37 °C. Dissociation was stopped by the addition of heat-inactivated fetal bovine serum (10% v/v final concentration). Suspended cells were pelleted and incubated with DNAseI at room temperature for 15 min. Cells were pelleted and resuspended in 100 μL phosphate-buffered (pH 6.5) saline (PBS) and immediately FACS-sorted.

GFP+ vs. GFP- retinal cells were sorted using a BD FACSAria flow cytometer, using the 488 nm laser and FITC fluorescence filter, and the 70 μm nozzle. Some cells were collected for fluorescence microscopy, or for post-sort FACS analysis. For RNA-seq or qPCR, GFP+ and GFP- cells were collected separately in the FACS sheath fluid, and RNA was immediately extracted.

RNA isolation and quantitative real-time PCR (qPCR)

RNA was extracted from tissue samples using the NucleoSpin® RNA kit (Macherey-Nagel) using the manufacturer’s protocol, quantified and quality-checked on a Nanodrop spectrophotometer, and cDNA was synthesized using the SuperScript® kit (New England Biotech) using random hexamer primers. Gene-specific primers used for qPCR were designed using AlleleID7/84 (Premier Biosoft), and are provided in Table 1. Amplification was carried out using a model 7900HT Fast Real-Time PCR System and SYBR-Green PCRMaster Mix (Applied Biosystems, Inc.). Relative quantitation of gene expression between GFP+ and GFP- samples was determined using the 2^-ΔΔCt method with 18S as the reference transcript [29], and five technical replicates per biological replicate. For samples from adult fish, retinal cells from a single adult fish constituted a biological replicate (3–5 replicates); for samples from juvenile fish, retinal cells from 10 to 15 juveniles were pooled for each biological replicate (3 replicates); for samples from larvae, retinal cells from 15 to 20 larvae were pooled for each biological replicate (3 replicates).
Table 1

Primers used for qPCR

Gene

Sense Primer 5′ - > 3′

Anti-sense Primer 5′- > 3′

aipl1

TCCAGTCAGTCTTTACAC

CCTTAGTTCCAGTCACAA

ajap1

GGAGTAAGGTGTCTAACT

TTCCTGATATTCGTCCAT

apoc1l

CCCAATTACCTTGTGTTT

ACAGTGTGACTTTGTATTG

atat1

CTAATGTGAATCTGCTATA

ACTCAAGTTACTATCCAA

bbs4

ACCACATTAGGACTGCTG

TCATAGGTCAGAGCGTTTC

cabp4

AGTTCGTTATGATGTTGTCTCT

CTATGATGATCCGCCACTG

cobl

TCTAACCATACAGCAGAATCCA

GTCCAGGCGACAACATTG

cry3

TTACTCTTCTGGATTTCC

ATATAAACACACCGTACA

dscamb

AAGAAGATGGTCTGACTC

CAAGGGAAAGCAAGTATT

egf

TAAGTGAGTGGACAATGTT

GTCTTCGTGTTCCATCTA

enc1

ACGAGTCAGTATATTTCT

GTAAGTAACGAGCCTATA

esrrb

CGTCTCCTCATACTTCAG

TCCTCCACTCTATTAGCA

esrrd

CATGACCTTATGTGACCTT

CAGAAACCTGGTATGTGT

gc2

CTGTGTTAATTGGTGGAA

AGAGTATCGTAGGACATAA

gc3

CTCTATTCACTGCCATAT

CATGGTTACTGTTAAGAC

gngt1

AATCCATTCATTCAACACAACAT

ACTTCCATCTTCGCCTTATC

gucy2f

TAGCATTACACTATGGATT

GCCTATGATTCCTACTTT

kcnv2a

GCAGGAGTTAAGTAAGGATAT

TAGGAGTGGAGAACAGTC

kita

AATAAGCTTGCCGCCACCATGGAATATCACTGCGTTCT

CAAATATTTGTAGGTGAGCACAATCAGGATGAGAAC

lingo1a

TGCTTGTACGGATTGAAT

ATGTTGAGGAAACGAAGA

Lplastin

GCAGTGGGTGAACGAAACAC

TCGAGATCGCATACTTGGCG

mef2ca

TGTAATCATTCAGCGTAGTG

TCTAAGGTGTGCCGTTAT

mef2cb

CCCGTGAATAACCAGATC

GTGACATGCTGTTTCTTT

mpeg1.1

CGGGTTCAAGTCCGTAACCA

TGGCGTCAGCGATTTCTTCT

msi1

CGAGCCCAGCCTAAGTTG

ATCTTCAATAGTCGTGTTCACTGA

ncam1b

AGTTTGATAAAGATGTTCGTTTC

TTAATGCTGCGGAAGTCA

ngf

GAGAAGACTACAAGCGAAT

CGACAACAATAAGGAGGAT

nr1d4a

AATCATCTTATCGCACAAC

ATAGTAGTAGGTAGTAGGAGTA

nr1d4b

AACGGTCACTATAACTTC

GAATAGCTGTTGTGTTTAG

nr2f1b

TGAGAAGAACACAGAGTAA

AGGATTGCTGACTATAACA

nrl

GATGGTCAGAGGAGAATG

GGTTGTAACGAGTGCTTA

nucb2b

ATGATATGGTGGAGATGGA

CTTGTTCGTGGCAGTAAT

panx1b

GCAGAGTGATTCTAAGTA

GAGTGAGATGAGTAACAA

pdca

TGCCGATGTGGAATAATCAGA

ACAGCGTCATTACTCATTCTATCT

ppdpfa

TAGCGTTTACCCGACCAA

TTTCCCCGTCCTCTAAAG

prom1b

CAGTTGGAGTGACAGTTG

TCAGGTCTCTTATGTTGGT

rtn2a

GGACACATAGACACAGACAA

CCTTCCAGTAGACCAGGT

rho

ACTTCCGTTTCGGGGAGAAC

GAAGGACTCGTTGTTGACAC

rhol

GCTGTGAGATGCTGGATT

GTTGTTGTTGTTGTTGTTGTC

rims3

AGAGGAGGTCAGTTAGAG

TATATGTTGCTGGAATGTTC

rxrga

TTCACACTGGTCATTCAA

AAGGCATTATAGAGCGATT

rxrgb

ACATAATACAGACAGAGACT

TAATAGCACAAGACAGAATC

thrb

TCTGGTCTGATGAGTCTA

GTATTAGCCTGGTGATGA

tprn

CAAACAACAAACATATAATCAAGT

TCTGAATGGTCGTGAATG

tulp1b

CAAGGAATCAACAGAGAAG

CATCATCATCATCGTCATC

sept8b

CTATCGTGGACTACATTGA

ATGAAGTACAGGCAGATG

znf536

CAATGGACAGAATTTAGGAATCA

CACAAAGAGGACAGGGATAT

18S

GAACGCCACTTGTCCCTCTA

GTTGGTGGAGCGATTTGTCT

Library construction, RNA-seq, and bioinformatics

Both quantity and quality of RNA were assessed by using an Agilent 2100 Bioanalyzer. All samples used for RNA-seq had an RNA integrity number (RIN) > 8.0, and the experimental design retained pairing information between GFP+ cells and GFP- cells derived from both retinas of a single fish, allowing us to analyze them as paired samples. At least 5 ng of RNA was available per sample, and provided to the University of Idaho’s Institute for Bioinformatics and Evolutionary Studies (IBEST) Genomics Core for RNA amplification, the generation of cDNA, sequencing, and bioinformatics. Quality and quantity of cDNA libraries were verified by Bioanalyzer. All sample preparation was achieved with Ovation® RNA-Seq System V2 (NuGEN), and sequencing performed on an Illumina (San Diego, CA) MiSeq with MiSeq Reagent Kit v3, 600 cycle kit. Four biological replicates (from four different fish) were sequenced (Fig. 1a). Reads were quality-trimmed with Sickle (https://github.com/najoshi/sickle), and paired reads were overlapped with FLASH [30]. Overlapped reads were aligned against Zv9.75 using the Burrows-Wheeler aligner [31]. BAM files were sorted with using SAMtools [32], and reads were counted by feature using HTSeq-count [33]. Counts were analyzed and differentially expressed genes were identified with R [34] and edgeR [35]. Descriptive plots were generated, and gene ontology (GO) analysis and hierarchical clustering were performed, with R and GOstats [36]. Comparison with a publicly available microarray dataset [37] was done using paralogue and probe identifier information available via Ensembl’s BioMart (http://uswest.ensembl.org/biomart/martview/83d09c7c5ff71f36d9df58ed9f566c78).
Fig. 1
Fig. 1

Dissociation, FACS separation, and RNA-seq analysis of GFP+ rod photoreceptors and GFP- retinal cells. a Experimental procedure. b Representative FACS results showing dissociated cells (inset; arrow indicates GFP+ cell), GFP+ population collected in P1, GFP- population collected in P2. Cells not in P1 or P2 are in red in the second panel. c Post-sort analysis of a sorted GFP+ population by fluorescence microscopy (inset; arrow indicates GFP+ cell) and FACS. SSC, side scatter (reflecting object complexity); FSC, forward scatter (reflecting object size)

Probe preparation and in situ hybridization

Zebrafish rho (rhodopsin) cDNA, in pBK-CMV phagemid, was the gift of T. Vihtelic. Other cDNAs were generated as follows. Total RNA was extracted from homogenized adult zebrafish retina, and cDNA was generated using random hexamers and oligo(dT) primers. Gene-specific primers (Table 2) corresponding to rhol, dscamb, rxrga, and rxrgb predicted mRNAs were designed using Primer-BLAST (https://www.ncbi.nlm.nih.gov/tools/primer-blast/), were used for PCR amplifications, and the resulting amplicons were gel-purified and ligated using TA-ligation into the pGEM-T-Easy vector (Promega), which contains T7 and SP6 promoters. cDNAs were sequence-verified (ElimBio; St. Hayward, CA), with sequencing results compared to original genomic sequence using nucleotide Blast software and viewed in Sequencher (GeneCodes). Digoxigenin (dig) –labeled cRNA probes were prepared using T7 or SP6 RNA polymerase (Roche) according to the manufacturer’s instructions. In situ hybridization was carried out according to Nelson et al. [16]. In brief, sections were rehydrated, permeabilized with proteinase K, dehydrated and incubated with probe in a solution containing 50% formamide, with hybridization temperatures optimized for each probe using PolyPro [38]. Hybridized tissues were treated with RNAse A, and the presence of dig was detected with anti-dig antibodies conjugated to alkaline phosphatase, followed by an NBT-BCIP (Roche) or BM-purple (Sigma) color reaction carried out according to the manufacturer’s instructions. In situs were imaged on a Leica DM2500 upright microscope with a Leica DFC700T camera using DIC optics. In addition to antisense probes, sense probes were also prepared and confirmed not to generate detectable signal.
Table 2

Primers used for generation of in situ probes

Primer name

Primer sequence 5′- > 3′

Probe length

rhol_probe_F

CGAAGTGACCCGAATGGTGA

764b

rhol_probe_R

GCGGAATGAACCGCCTTAAC

dscamb_probe_F

TCTGGATCCCCGGAGACAAT

757b

dscamb_probe_R

TCTGGATCCCCGGAGACAAT

rxrga_probe_F

GGAGAAGATCCTGGACGCTG

734b

rxrga_probe_R

AGTGTGCGCTGGGGTTTATT

rxrgb_probe_F

CGCGGAATGGATACTCACGA

807b

rxrgb_probe_R

TCCGCTGCATGGCAGATATT

Retinal damage and regeneration

The retinas of adult xops:eGFP fish (1 yr) were chemically lesioned to destroy all retinal neurons while sparing Müller glia [13]. Briefly, fish were anaesthetized by tricaine and an incision was made across the cornea with a sapphire blade. Using a Hamilton syringe, 0.4 μL - 0.6 μL of 200 μM ouabain was injected into the vitreal chamber of the right eye, resulting in an estimated intraocular concentration of 10 μM [11, 15, 39]. Loss of GFP+ photoreceptors was verified in sectioned retinas obtained from parallel experiments at 3 days post-injury (3 dpi), and by viewing retinas of live, anaesthetized fish with epifluorescence stereomicroscopy (Leica M165 FC), also at 3 dpi. Lesioned zebrafish were allowed to recover, and regenerate their retinas [11] until 14 dpi or 30 dpi, and were humanely sacrificed to collect retinas for cell dissociation, FACS, and qPCR, or to collect whole eyes for cryosectioning.

Indirect immunofluorescence and confocal microscopy

Histological processing and sectioning was carried out as previously described [28]. In brief, whole eyes were perforated at the cornea, to create a slit through which lenses were removed. Eyecups were immersed in phosphate-buffered (pH -7.4), 4% paraformaldehyde containing 5% sucrose and fixed at room temperature for 1 h. Eyes were subjected to sequential washes with increasing concentrations of phosphate-buffered sucrose, and cryoprotected overnight at 4 °C in phosphate-buffered, 20% sucrose. Eyes were embedded in a 1:2 mixture of OCT (optimal cutting temperature; Sakura Finetek) and buffered, 20% sucrose, and sectioned on a Leica CM3050 cryostat at 5 μm. Sections were blocked in 20% goat serum 1 h, room temperature, and then incubated with primary antibody 1D1 (1:20) (the gift of James Fadool) overnight, 4 °C, which stains zebrafish rhodopsin [40]. Sections were washed with phosphate-buffered (pH -7.4) saline containing 0.01% TritonX-100 (PBST), and then incubated with secondary antibody conjugated to Cy3 (1:200; Jackson Immunoresearch) for 2 h at room temperature. Mounted sections were imaged with a Nikon Andor spinning disk confocal microscope and Zyla sCMOS camera using 40X dry and 60X oil immersion objectives.

Results

Transcripts of rods of adult zebrafish retina

We isolated highly pure rod and non-rod retinal cell populations by FACS-sorting cell suspensions from adult xops:eGFP zebrafish retinas (Fig. 1a). GFP+ cells (P1 in Fig. 1b) made up 10–20% of all collected retinal cells and constituted a distinctive cell population as compared with the GFP- population (P2 in Fig. 1b). Visualization of samples using epifluorescence microscopy suggested that the majority of dissociated GFP+ profiles, and FACS-sorted GFP profiles, appeared to be rounded-up rod cell bodies rather than outer segments or other fragments (insets in Fig. 1b, c). To verify enrichment of our sorted populations, a separate sample from one fish was used to collect GFP+ cells using the same FACS-sorting parameters as those used for RNA-seq, and we subsequently examined the sorted population by fluorescence microscopy and by post-sort analysis (Fig. 1c). These results indicated that P1 population was highly enriched for GFP+ cells (Fig. 1c), and therefore suitable for transcriptome analysis.

We performed RNA-seq on both the rod (GFP+; P1) and the “non-rod” (GFP-; P2) populations, in order to identify transcripts enriched, present, or depleted in the rod population as compared with other retinal cells (similar to the approach of [41]). The resulting dataset is publicly available via the Gene Expression Omnibus (GEO; accession # GSE100062). Sequencing depth ranged from 2,781,516 to 3,480,515 reads per sample, and mapping percentages ranged from 97.0% to 97.4% per sample. Multidimensional scaling showed good separation of GFP+ vs. GFP- samples along the first dimension and separation by sample along the second dimension (Additional file 1: Figure S1A). A plot of estimated Biological Coefficient of Variation (BCV) indicated a trend in dispersion associated with expression (Additional file 1: Figure S1B), leading us to fit a trended model within edgeR before doing differential expression analysis. Differentially expressed transcripts were identified as those significantly upregulated or downregulated in the GFP+ population vs. the GFP- population. Those identified with a false discovery rate (FDR) of < 0.01 consisted of 1629 distinct entries (597 upregulated, 1032 downregulated); those identified with an FDR of < 0.05 consisted of 2439 entries (Additional file 1: Figure S1C). The top 50 upregulated and top 50 downregulated transcripts within the GFP+ vs. GFP- populations, based upon FDR, are provided as Tables 3 and 4, respectively. Numerous transcripts known to be expressed exclusively by rods were significantly upregulated (enriched) in the GFP+ cell population, including rho, pde6g, rom1b, and gnat1 (Table 3). Numerous transcripts known to be primarily expressed by other retinal cell types were significantly downregulated (depleted) in the GFP+ cell population, including cone transcripts opn1lw2 (long wavelength-sensitive cone opsin 2), opn1mw3 (cone opsin rh2–3), and cnga3a, and the macrophage/microglial marker mpeg1 [42] (Table 4). These outcomes further corroborated the rod (GFP+) vs. non-rod (GFP-) identities of our sample cell populations.
Table 3

Top 50 transcripts significantly upregulated (enriched) in GFP+ (rods) vs GFP- retinal cell populations

Name

Description

logFC

FDR

gc2

guanylyl cyclase 2 [Source:ZFIN;Acc:ZDB-GENE-011128-8]

3.032892

5.22E-22

esrrd

estrogen-related receptor delta [Source:ZFIN;Acc:ZDB-GENE-040616-3]

3.642435

8.52E-17

zgc:112,334

zgc:112,334 [Source:ZFIN;Acc:ZDB-GENE-050809-120]

3.829432

3.64E-16

gngt1

guanine nucleotide binding protein (G protein), gamma transducing activity polypeptide 1 [Source:ZFIN;Acc:ZDB-GENE-030131-7596]

2.959265

4.60E-16

arhgap29a

Rho GTPase activating protein 29a [Source:ZFIN;Acc:ZDB-GENE-030131-9510]

2.653423

8.20E-16

kitb

kit receptor b [Source:ZFIN;Acc:ZDB-GENE-050916-2]

2.782837

1.06E-15

si:dkey-204f11.59

si:dkey-204f11.59 [Source:ZFIN;Acc:ZDB-GENE-040724-220]

3.212857

2.27E-15

ajap1

adherens junctions associated protein 1 [Source:ZFIN;Acc:ZDB-GENE-041210-353]

2.499397

7.05E-15

OSBPL1A (2 of 2)

oxysterol binding protein-like 1A [Source:HGNC Symbol;Acc:16,398]

2.427894

7.09E-15

pde6g

phosphodiesterase 6G, cGMP-specific, rod, gamma [Source:ZFIN;Acc:ZDB-GENE-030904-1]

3.045885

9.01E-15

UBAP1L (1 of 2)

ubiquitin associated protein 1-like [Source:HGNC Symbol;Acc:40,028]

2.868683

9.01E-15

rcvrna

recoverin a [Source:ZFIN;Acc:ZDB-GENE-050913-106]

2.719941

5.43E-14

rom1b

retinal outer segment membrane protein 1b [Source:ZFIN;Acc:ZDB-GENE-040426-1073]

2.85896

5.78E-14

rorb

RAR-related orphan receptor B [Source:ZFIN;Acc:ZDB-GENE-061204-2]

2.48207

6.19E-14

tmtops2a

teleost multiple tissue opsin 2a [Source:ZFIN;Acc:ZDB-GENE-130129-3]

2.265541

1.05E-13

cerkl

ceramide kinase-like [Source:ZFIN;Acc:ZDB-GENE-070410-38]

2.181324

1.11E-13

cobl

cordon-bleu homolog (mouse) [Source:ZFIN;Acc:ZDB-GENE-091020-11]

2.417617

1.19E-13

hcn3

hyperpolarization activated cyclic nucleotide-gated potassium channel 3 [Source:ZFIN;Acc:ZDB-GENE-060503-193]

3.197947

1.51E-13

zgc:162,144

zgc:162,144 [Source:ZFIN;Acc:ZDB-GENE-030131-7630]

2.775518

1.70E-13

gnb1b

guanine nucleotide binding protein (G protein), beta polypeptide 1b [Source:ZFIN;Acc:ZDB-GENE-040426-2855]

2.767042

1.70E-13

unc119.2

unc-119 homolog 2 [Source:ZFIN;Acc:ZDB-GENE-030131-7635]

2.116224

1.79E-13

PTPDC1 (1 of 3)

protein tyrosine phosphatase domain containing 1 [Source:HGNC Symbol;Acc:30,184]

3.253732

2.91E-13

pdca

phosducin a [Source:ZFIN;Acc:ZDB-GENE-031023-1]

2.797727

3.06E-13

rom1a

retinal outer segment membrane protein 1a [Source:ZFIN;Acc:ZDB-GENE-040426-1765]

3.176656

3.68E-13

kcnv2a

potassium channel, subfamily V, member 2a [Source:ZFIN;Acc:ZDB-GENE-091117-27]

2.625431

4.38E-13

rho

rhodopsin [Source:ZFIN;Acc:ZDB-GENE-990415-271]

3.214731

4.63E-13

cplx4c

complexin 4c [Source:ZFIN;Acc:ZDB-GENE-101018-1]

2.863052

7.98E-13

samd11

sterile alpha motif domain containing 11 [Source:ZFIN;Acc:ZDB-GENE-060428-2]

2.708617

9.40E-13

BX248120.1

Uncharacterized protein [Source:UniProtKB/TrEMBL;Acc:E7F7S5]

2.586515

1.34E-12

saga

S-antigen; retina and pineal gland (arrestin) a [Source:ZFIN;Acc:ZDB-GENE-040426-1538]

3.089512

1.44E-12

arhgef10lb

Rho guanine nucleotide exchange factor (GEF) 10-like b [Source:ZFIN;Acc:ZDB-GENE-090313-222]

2.476543

1.60E-12

guca1a

guanylate cyclase activator 1A [Source:ZFIN;Acc:ZDB-GENE-011128-5]

2.765826

1.68E-12

si:dkeyp-41f9.3

si:dkeyp-41f9.3 [Source:ZFIN;Acc:ZDB-GENE-091118-56]

2.849587

1.72E-12

TDRD7B

Tudor domain-containing protein 7B [Source:UniProtKB/Swiss-Prot;Acc:E7FDW8]

2.840789

2.06E-12

PLCH2 (1 of 2)

phospholipase C, eta 2 [Source:HGNC Symbol;Acc:29,037]

2.020111

2.30E-12

cabp4

calcium binding protein 4 [Source:ZFIN;Acc:ZDB-GENE-081104-291]

2.513244

2.77E-12

guca1b

guanylate cyclase activator 1B [Source:ZFIN;Acc:ZDB-GENE-011128-6]

2.703103

2.78E-12

grk1a

G protein-coupled receptor kinase 1 a [Source:ZFIN;Acc:ZDB-GENE-050823-1]

2.930581

1.10E-11

gnb1a

guanine nucleotide binding protein (G protein), beta polypeptide 1a [Source:ZFIN;Acc:ZDB-GENE-030131-823]

2.886447

1.19E-11

slc6a15

solute carrier family 6 (neutral amino acid transporter), member 15 [Source:ZFIN;Acc:ZDB-GENE-050420-93]

2.779643

1.45E-11

ppdpfa

pancreatic progenitor cell differentiation and proliferation factor a [Source:ZFIN;Acc:ZDB-GENE-030219-204]

2.669857

1.71E-11

pde6b

phosphodiesterase 6B, cGMP-specific, rod, beta [Source:ZFIN;Acc:ZDB-GENE-090421–2]

3.049742

2.01E-11

znf536

zinc finger protein 536 [Source:ZFIN;Acc:ZDB-GENE-030616-624]

2.683055

2.19E-11

SUSD3

sushi domain containing 3 [Source:HGNC Symbol;Acc:28,391]

2.124055

2.28E-11

gnat1

guanine nucleotide binding protein (G protein), alpha transducing activity polypeptide 1 Source:ZFIN;Acc:ZDB-GENE-011128-11]

2.967409

3.45E-11

sagb

S-antigen; retina and pineal gland (arrestin) b [Source:ZFIN;Acc:ZDB-GENE-050913-98]

3.155676

3.69E-11

asmt

acetylserotonin O-methyltransferase [Source:ZFIN;Acc:ZDB-GENE-080220-43]

1.844975

4.41E-11

pfkfb4l

6-phosphofructo-2-kinase/fructose-2,6-biphosphatase 4, like [Source:ZFIN;Acc:ZDB-GENE-031031-4]

1.93027

4.63E-11

alpl

alkaline phosphatase, liver/bone/kidney [Source:ZFIN;Acc:ZDB-GENE-040420-1]

2.701265

5.22E-11

slc24a1

solute carrier family 24 (sodium/potassium/calcium exchanger), member 1 [Source:ZFIN;Acc:ZDB-GENE-060503-191]

2.88482

7.45E-11

Table 4

Top 50 transcripts significantly downregulated (depleted) in GFP+ (rods) vs GFP- retinal cell populations

Name

Description

logFC

FDR

si:dkey-27i16.2

si:dkey-27i16.2 [Source:ZFIN;Acc:ZDB-GENE-030131-9667]

−6.03866537

1.88E-38

ptprc

protein tyrosine phosphatase, receptor type, C [Source:ZFIN;Acc:ZDB-GENE-050208-585]

−6.06476722

3.46E-31

apoc1l

apolipoprotein C-I like [Source:ZFIN;Acc:ZDB-GENE-030131-1074]

−4.46320866

2.75E-30

cd74a

CD74 molecule, major histocompatibility complex, class II invariant chain a [Source:ZFIN;Acc:ZDB-GENE-000901-1]

−4.67633439

1.65E-28

bzw1b

basic leucine zipper and W2 domains 1b [Source:ZFIN;Acc:ZDB-GENE-040426-2881]

−3.66358803

9.06E-28

si:dkey-25o1.6

si:dkey-25o1.6 [Source:ZFIN;Acc:ZDB-GENE-091204-276]

−5.26240739

3.27E-27

si:ch211–260d11.1

si:ch211–260d11.1 [Source:ZFIN;Acc:ZDB-GENE-091204-40]

−6.02459793

1.05E-26

lgals3bpb

lectin, galactoside-binding, soluble, 3 binding protein b [Source:ZFIN;Acc:ZDB-GENE-040426-2262]

−5.09075533

1.25E-26

coro1a

coronin, actin binding protein, 1A [Source:ZFIN;Acc:ZDB-GENE-030131-9512]

−7.62303025

1.06E-25

hbaa1

hemoglobin alpha adult-1 [Source:ZFIN;Acc:ZDB-GENE-980526-79]

−9.74873113

1.70E-25

si:dkey-25o1.5

si:dkey-25o1.5 [Source:ZFIN;Acc:ZDB-GENE-091204-344]

−9.53659867

7.14E-23

sla2

Src-like-adaptor 2 [Source:ZFIN;Acc:ZDB-GENE-080204-98]

−9.56172956

2.35E-22

inpp5d

inositol polyphosphate-5-phosphatase D [Source:ZFIN;Acc:ZDB-GENE-100922–30]

−4.44994274

1.17E-21

mpeg1

macrophage expressed 1 [Source:ZFIN;Acc:ZDB-GENE-030131-7347]

−9.35334321

2.15E-21

ZFP36

ZFP36 ring finger protein [Source:HGNC Symbol;Acc:12,862]

−5.4525006

1.53E-20

ankrd33ab

ankyrin repeat domain 33Ab [Source:ZFIN;Acc:ZDB-GENE-100729-1]

−3.13603996

1.97E-20

pfn1

profilin 1 [Source:ZFIN;Acc:ZDB-GENE-031002–33]

−4.86406116

2.72E-20

grk7a

G-protein-coupled receptor kinase 7a [Source:ZFIN;Acc:ZDB-GENE-050824-1]

−2.77617205

5.07E-20

rcv1

recoverin [Source:ZFIN;Acc:ZDB-GENE-030131-7590]

−2.80718642

2.57E-19

tagapa

T-cell activation RhoGTPase activating protein a [Source:ZFIN;Acc:ZDB-GENE-040426-1877]

−6.39333701

1.05E-18

si:dkey-126 g1.9

si:dkey-126 g1.9 [Source:ZFIN;Acc:ZDB-GENE-030131-9862]

−2.79689496

1.53E-18

havcr1

hepatitis A virus cellular receptor 1 [Source:ZFIN;Acc:ZDB-GENE-040718-131]

−7.67482315

1.91E-18

slc1a8b

solute carrier family 1 (glutamate transporter), member 8b [Source:ZFIN;Acc:ZDB-GENE-070912-552]

−2.5380374

3.55E-18

csf1ra

colony stimulating factor 1 receptor, a [Source:ZFIN;Acc:ZDB-GENE-001205-1]

−4.24059459

1.94E-17

si:ch211–250 g4.3

si:ch211–250 g4.3 [Source:ZFIN;Acc:ZDB-GENE-060503-506]

−7.55964405

3.53E-17

arpc1b

actin related protein 2/3 complex, subunit 1B [Source:ZFIN;Acc:ZDB-GENE-030131-7414]

−4.66326368

6.41E-17

CT826376.1

Uncharacterized protein [Source:UniProtKB/TrEMBL;Acc:E7F690]

−2.34407255

7.14E-17

pdcb

phosducin b [Source:ZFIN;Acc:ZDB-GENE-031023-2]

−2.4532108

9.01E-17

opn1lw2

opsin 1 (cone pigments), long-wave-sensitive, 2 [Source:ZFIN;Acc:ZDB-GENE-040718-141]

−2.76413479

5.15E-16

ba1

ba1 globin [Source:ZFIN;Acc:ZDB-GENE-990415-18]

−6.23069882

6.15E-16

opn1mw3

opsin 1 (cone pigments), medium-wave-sensitive, 3 [Source:ZFIN;Acc:ZDB-GENE-030728-6]

−2.56365947

9.40E-16

hbaa1

hemoglobin alpha adult-1 [Source:ZFIN;Acc:ZDB-GENE-980526-79]

−6.44638081

2.14E-15

zgc:195,245

zgc:195,245 [Source:ZFIN;Acc:ZDB-GENE-081022-200]

−2.62839443

2.47E-15

arr3a

arrestin 3a, retinal (X-arrestin) [Source:ZFIN;Acc:ZDB-GENE-040718-102]

−3.02133496

2.47E-15

zgc:100,919

zgc:100,919 [Source:ZFIN;Acc:ZDB-GENE-040718-248]

−4.70079878

3.07E-15

gc3

guanylyl cyclase 3 [Source:ZFIN;Acc:ZDB-GENE-011128-9]

−2.32749631

4.00E-15

ppp1r18

protein phosphatase 1, regulatory subunit 18 [Source:ZFIN;Acc:ZDB-GENE-060503-350]

−2.29809174

5.42E-15

CD68

CD68 molecule [Source:HGNC Symbol;Acc:1693]

−3.83135448

5.42E-15

il1b

interleukin 1, beta [Source:ZFIN;Acc:ZDB-GENE-040702-2]

−4.3585252

5.67E-15

cplx4a

complexin 4a [Source:ZFIN;Acc:ZDB-GENE-060526-116]

−2.12559816

7.51E-15

cnga3a

cyclic nucleotide gated channel alpha 3a [Source:ZFIN;Acc:ZDB-GENE-090611–2]

−2.2388126

1.69E-14

ccr9a

chemokine (C-C motif) receptor 9a [Source:ZFIN;Acc:ZDB-GENE-060130-125]

−4.13641441

1.75E-14

opn1lw1

opsin 1 (cone pigments), long-wave-sensitive, 1 [Source:ZFIN;Acc:ZDB-GENE-990604-41]

−2.8443546

1.89E-14

KEL

Kell blood group, metallo-endopeptidase [Source:HGNC Symbol;Acc:6308]

−8.54223593

2.27E-14

si:ch1073-403i13.1

si:ch1073-403i13.1 [Source:ZFIN;Acc:ZDB-GENE-100921–25]

−4.50874649

2.31E-14

wasb

Wiskott-Aldrich syndrome (eczema-thrombocytopenia) b [Source:ZFIN;Acc:ZDB-GENE-030131-7098]

−5.26157912

2.52E-14

SLC24A2 (1 of 2)

solute carrier family 24 (sodium/potassium/calcium exchanger), member 2 [Source:HGNC Symbol;Acc:10,976]

−2.22076034

2.67E-14

pbxip1b

pre-B-cell leukemia homeobox interacting protein 1b [Source:ZFIN;Acc:ZDB-GENE-070112-2032]

−2.27917445

3.27E-14

CD53

CD53 molecule [Source:HGNC Symbol;Acc:1686]

−5.72855472

3.28E-14

slc25a25a

solute carrier family 25 (mitochondrial carrier; phosphate carrier), member 25a [Source:ZFIN;Acc:ZDB-GENE-040426-2396]

−2.50025348

3.72E-14

To provide broad classification of rod-enriched transcripts, we used gene ontology (GO) analysis. GO molecular function categories significantly overrepresented in GFP+ samples included those related to cyclic nucleotide metabolism, intermediary metabolism, and ion transport (Fig. 2a), and GO biological processes that were overrepresented included intracellular transport processes, photoreceptor cell development, and the kit and notch signaling pathways (Fig. 2b). GO biological process categories related to cell stress or apoptosis were not overrepresented, suggesting that, although the GFP+ rods did not maintain their morphologies during the dissociation and sorting procedures (insets in Fig. 1a, b), these procedures likely did not cause differential upregulation of genes related to stress and cell death in the rods. These findings are consistent with the recent report by Richardson et al. [43] showing that FACS does not perturb gene expression. GO cellular component categories significantly overrepresented in the GFP+ samples included those related to cytoskeletal components and those related to cilia (Fig. 2c). These categories reflect the underlying structure, function, and very likely the ongoing developmental programs engaged for maintaining rod structure and function. It was surprising, however, that some of these categories were overrepresented considering the large number of cones likely to be present in the GFP- retinal cell population that were also expected to demonstrate similar molecular functions, biological processes, and cellular components. Hierarchical clustering of the rod-enriched transcripts returned only three, highly similar clusters (Fig. 2d), suggesting very little sample heterogeneity within the GFP+ samples and within the GFP- samples. Our experimental design included sex as a potential biological variable, such that we could analyze a sex X rod interaction. This analysis returned only five entries with an FDR < 0.05 (Table 5).
Fig. 2
Fig. 2

Gene ontology (GO) and hierarchical cluster analysis. a-c Molecular functions (a), biological processes (b), and cellular components (c) overrepresented in the GFP+ (rod photoreceptor) cell population (p < 0.01). d Hierarchical clustering of rod-enriched transcripts reveals only three, highly similar clusters. F, female; M, male

Table 5

Sex X rod interaction

Name

Description

logFC

FDR

Comment

pmela

premelanosome protein a [Source:ZFIN;Acc:ZDB-GENE-030131-9818]

15.0198

6.05E-06

Absent in female rods; Present in male rods

slc6a6b

solute carrier family 6 (neurotransmitter transporter, taurine), member 6b [Source:ZFIN;Acc:ZDB-GENE-030131-3077]

−4.06708

3.31E-05

Enriched in female rods; depleted in male rods

naa35

N(alpha)-acetyltransferase 35, NatC auxiliary subunit [Source:ZFIN;Acc:ZDB-GENE-030131-306]

−5.25565

0.025774

Enriched in female rods; depleted in male rods

si:ch211-89f7.1

si:ch211-89f7.1 [Source:ZFIN;Acc:ZDB-GENE-060526-180]

−2.75147

0.025774

Enriched in female rods; less enriched in male rods

ush2a

Usher syndrome 2A (autosomal recessive, mild) [Source:ZFIN;Acc:ZDB-GENE-060503-794]

−2.65862

0.025941

Enriched in female rods; not enriched in male rods

The analyses described above focused upon transcripts that were differentially expressed in GFP+ vs. GFP- cells, therefore identifying enriched transcripts in either population. To identify additional transcripts present in rods, but not necessarily enriched in comparison with other retinal cells, we generated a list of transcripts for which all GFP+ samples returned a non-zero value. This list of transcripts present in rods amounted to 13,324 distinct entries (not shown), approximately 23% of the total number of predicted transcripts (58,549; Ensembl GRCz10) encoded by the zebrafish genome. This list included numerous photoreceptor (but not rod-specific) genes such as irbp, neurod, crx, and rx1, and some genes not previously known to be expressed in rod photoreceptors, such as opsin 4.1, a zebrafish melanopsin [44], and several nuclear hormone receptor genes including rxrga. The latter is noteworthy because the mouse orthologue (RXRγ) was reported to be cone-specific [45].

Forty-five transcripts were selected for validation analysis by qPCR in independently sorted GFP+ vs. GFP- cells from adult xops:eGFP zebrafish. Transcripts were prioritized for validation based upon predicted or know functions as transcription factors (e.g. esrrb, nrl, nr2f1b, rxrga), as components of cell signaling pathways (e.g. ngf, kita), or as cell adhesion molecules (e.g. dscamb, ncam1b), because future analysis of such components stands to reveal new insights into regulation of rod development, maturation, and/or maintainance. We also selected some transcripts known to have structural (e.g. prom1b, bbs4) or functional requirements in photoreceptors (e.g. rhol, gngt1, pdca). Finally, we selected transcripts that were detected as enriched in rods, as well as some that were detected as present in rods, but not enriched, to more thoroughly validate the RNA-seq dataset.

Selected transcripts that were detected by RNA-seq as significantly enriched in rods, were all determined to be significantly enriched in rods by qPCR, at similar relative magnitudes (Fig. 3a). Selected transcripts that were detected by RNA-seq as present, though not enriched in rods, were all detectable by qPCR (see first five genes in Fig. 3b). Some of these were detected by qPCR to be significantly enriched (the first three genes in Fig. 3b), a minor discrepancy perhaps related to the larger number of biological replicates used for qPCR. Transcripts detected by RNA-seq as significantly depleted but still present in rods, were nearly all determined to be significantly depleted in rods by qPCR, with the exception of mef2cb, where qPCR did not detect a significant difference (see last six genes in Fig. 3b), but nevertheless detected the presence of this transcript in rods. These qPCR results provide strong validation that the RNA-seq dataset generated in this study will serve as a reliable resource for many future applications.
Fig. 3
Fig. 3

Quantitative PCR (qPCR) validation of transcripts enriched in GFP+ (rod photoreceptor) cells (a), and present or depleted in GFP+ cells (b). Top panel in each shows RNA-Seq results; bottom panel shows qPCR. **, p < 0.01; *, p < 0.05; ns, not significantly differentially expressed, for GFP+ vs. GFP- (three biological replicates)

Rod photoreceptor transcripts over the lifespan and in a genetic model for rod degeneration

As zebrafish grow, they continue to generate new rods throughout the retina from a dedicated rod lineage [4, 16], the apex of which (stem cell for rod lineage) has been identified as the Müller glial cell [8]. Therefore we wished to determine whether the rod transcriptome remained consistent over the zebrafish lifespan, or if the rod population of larval zebrafish would be distinct from the accumulated (and generally older) rod population of adult zebrafish. A subset of the selected transcripts that were qPCR validated in adult zebrafish, were therefore evaluated further by qPCR in GFP+ vs. GFP- retinal cell populations obtained from larval zebrafish sacrificed at 14 dpf (days post-fertilization), and juvenile zebrafish sacrificed at 30 dpf. Rod photoreceptors are considered morphologically mature at 15 dpf [46], but do not contribute to adult-like scotopic (rod-driven) electroretinogram responses until 29 dpf [47], and so these sampling times were also selected to represent stages in the functional maturation of rods. The xops:eGFP transgenic line is known to show rod-specific transgene expression throughout the zebrafish lifespan [26], and so was considered appropriate as source material for these analyses.

In general, the relative expression levels of selected rod-enriched transcripts within the GFP+ vs. GFP- cell populations were remarkably stable from larval through adult stages (Fig. 4a). However, rho transcripts appeared more highly enriched in rods of adult zebrafish than in rods of larval or juvenile zebrafish, suggesting that rods of adults may accumulate transcript at higher levels than rods of younger fish. Rhol (rhodopsin-like) transcripts showed the opposite trend (Fig. 4a), consistent with the recent findings of Morrow et al. [48], who detected limited expression of rhol in adult retina. Other transcripts more highly enriched in the rods of younger fish were gngt1, ngf, and aipl1. Transcripts present, or present but significantly depleted in adult rods, were less consistent over the lifespan; notable were rxrga and mef2ca, which were not differentially expressed in GFP+ vs. GFP- cells of larvae or juveniles, but were significantly downregulated (depleted) in rods of older zebrafish (Fig. 4b). Rod-specific functions for the encoded nuclear hormone receptor may be distinctive for rods of younger vs. older zebrafish.
Fig. 4
Fig. 4

A. qPCR of selected transcripts enriched (a), or present (and not differentially expressed) or present (and depleted) in GFP+ (rod photoreceptor) cells (b), in larval retinas (14 dpf), juvenile retinas (1 M), and adult retinas. **, p < 0.01; *, p < 0.05; ns, not significantly differentially expressed, for GFP+ vs. GFP- (three biological replicates)

We next measured expression (by qPCR) of selected transcripts in whole retinas obtained from WT zebrafish and from xops:mCFP zebrafish, which show a chronic rod degeneration that stimulates proliferation of a rod precursor population [37]. We anticipated that transcripts identified in the present study as rod-enriched, would be upregulated in WT retinas (containing mature rods) vs. xops:mCFP retinas (not containing mature rods). This was true for rho, rhol, dscamb, and ngf, but not true for esrrd, nrl, and nr2f1b, which were not differentially expressed in WT vs. xops:mCFP retinas (Fig. 5a). It is possible that the latter genes may have other retinal functions in the response to the chronic loss of rods. We also tested two transcripts present (but not enriched) in rods, rxrgb and Lplastin, and these were both significantly differentially downregulated in WT vs. xops:mCFP retinas (Fig. 5b), again suggestive of roles in response to chronic loss of rods. Two transcripts depleted in rods, and known to be expressed in cones in zebrafish or other model organisms, rxrga and thrb [45, 4951], were not differentially expressed in WT vs. xops:mCFP retinas, consistent with their likely predominant localization to cones, which are unaffected in the xops:mCFP zebrafish [9]. Differentially expressed genes in WT vs. xops:mCFP retinas have previously been identified using microarray (GEO Acc # GSE22221) [37], allowing a deeper comparison of the two datasets. Using a cutoff of p < 0.01 for both datasets returned 94 shared entries (Fig. 5c; Additional file 1: Table S1), including known photoreceptor genes aanat1, pde6a, rom1a, and rom1b. We believe the number shared by the datasets is limited to 94 transcripts is in part due to the incomplete representation of zebrafish transcripts on the Agilent chip used for the microarray study.
Fig. 5
Fig. 5

qPCR of selected transcripts enriched (a), or present (and not differentially expressed) or present (and depleted) in GFP+ (rod photoreceptor) cells (b), and relative expression in WT vs. xops:mCFP retinas. **, p < 0.01; *, p < 0.05; ns, not significantly differentially expressed for GFP+ vs. GFP- cells, or for WT vs. xops:mCFP retinas (three biological replicates). c Numbers of unique transcripts upregulated in GFP+ vs. GFP- retinal cells (present study), those upregulated in WT vs. xops:mCFP retinas [37], at p < 0.01, and those shared by both sets

Selected transcripts were further examined by in situ hybridization to visualize spatial expression patterns. For these studies we selected rhol and dscamb as rod-enriched transcripts, and rxrga and rxrgb as transcripts present in rods (Fig. 6). The expression pattern of rho is shown for reference as an example of a rod-exclusive hybridization pattern (Fig. 6a). Rhol (rh1–2) was previously detected as a second rho gene in zebrafish [52] and other teleost fish [48], with demonstrated phototransduction functions and expression in the photoreceptor layer [48]. In the present study we have confirmed that rhol is expressed (and enriched) in rods, based upon RNA-seq and qPCR of purified rods (Fig. 6b). In tissues sampled at 14 dpf, rhol was expressed in the photoreceptor layer, in a subset of cells matching the distribution of rods, but restricted primarily to the peripheral retina. This predominantly peripheral pattern was evident in retinas sampled at 1 month, and in adult retina, where only very weak expression was detected in central retina (Fig. 6b). In retinas of the xops:mCFP line that displays rod degeneration, rhol was not detected by in situ hybridization, even though some developing/dying rho-expressing cells are present (Fig. 6b). In rods that express rhol, the timing of expression may be delayed as compared with rho (rho is first expressed embryonically, while rhol is first expressed in larvae [52]), and rods of xops:mCFP zebrafish may simply not survive long enough to express rhol.
Fig. 6
Fig. 6

In situ hybridization for transcripts enriched (rho, rhol, dscamb) or present (rxrga, rxrgb) in rods of adult zebrafish, using tissues sampled from larvae (14 days post-fertilization; 14 DPF), juveniles (30 DPF), and adult WT fish, and from xops:mCFP transgenics, which show a chronic rod degeneration [9]. a Expression patterns for rho. Arrows in last panel show degenerating rods in xops:mCFP retina. b Expression patterns for rhol. c Expression patterns for dscamb. d Expression patterns for rxrga. e Expression patterns for rxrgb. DPF, days post-fertilization; CMZ, ciliary marginal zone; RPE, retinal pigmented epithelium; ONL, outer nuclear layer (photoreceptor layer); INL, inner nuclear layer; IPL, inner plexiform layer; GCL, ganglion cell layer. Scale bar (applies to all) = 50 μm

Dscamb is one of two zebrafish orthologues of mammalian Dscam. Mammalian Dscam encodes a homophilic cell adhesion molecule with numerous roles in retinal cell patterning and refinement of circuitry [53, 54], but is not expressed in mouse rods [55] (although dscamlike1 is expressed in mouse rods; [56]. In larval and juvenile zebrafish retinas, dscamb was expressed in some cells of the outer nuclear layer (photoreceptor layer; ONL), in a pattern consistent with identities of rods and possibly a subset of cones, and was also seen in the inner nuclear layer (INL) and ganglion cell layer (GCL) in a pattern suggestive of amacrine cells (Fig. 6c). Expression of dscamb in adult zebrafish retinas showed similar patterns (Fig. 6c). The xops:mCFP retinas showed apparently greatly reduced expression in the photoreceptor layer, consistent with dscamb localization to rods (Fig. 6c).

In larval and juvenile zebrafish, rxrga and rxrgb were both diffusely expressed in all retinal cellular layers, and more strongly localized to the far peripheral photoreceptor layer and the stem/progenitor cell-containing CMZ (Fig. 6d, e). The former pattern suggests transient higher expression in newly-generated photoreceptors, consistent with our previous report of expression of transient expression of rxrga in photoreceptors of zebrafish embryos [57]. Juvenile and adult zebrafish WT retinas, and those of xops:mCFP fish, both showed a diffuse pattern throughout all cellular layers, although the juvenile samples showed more pronounced expression of rxrga within the GCL and inner INL (Fig. 6d, e). These findings are consistent with the lack of significant enrichment of these transcripts in rods of adult zebrafish as detected by RNA-seq and qPCR (Fig. 3).

Rod photoreceptor transcripts in regenerated retina

The zebrafish regenerates a functional retina following widespread damage due to intravitreal injection of the neurotoxin ouabain [11]. However, regenerated fish retinas display histological errors such as neuronal cell bodies present in plexiform layers [14, 15] (and see Fig. 7), and disruptions of two-dimensional patterning [58, 59]. Although microarray and other analyses have revealed transcriptional changes in whole retina in response to damage [60] and accompanying the proliferative response specifically of Müller glia [6062], the molecular signatures of identified, regenerated retinal neurons have never been compared with those of native, undamaged retinal neurons. We sampled regenerated retinas at 14 dpi, a time when all retinal layers are known to be re-established, but with some histological errors and very thin plexiform layers [11]. Another set of regenerated retinas was sampled at 30 dpi, when plexiform layers have expanded, but histological errors remain. The fidelity of xops:eGFP reporter expression as rod-specific in regenerated retina has not, to our knowledge, been established. Therefore we processed retinal cryosections for visualization of the eGFP reporter together with staining by the 1D1 (anti-rhodopsin; [40]) monoclonal antibody, using confocal microscopy. GFP+ profiles were observed in the ONL of control retinas, and of 14 dpi and 30 dpi retinas, and were associated with DAPI+ nuclei (Fig. 7a–i, asterisks). This localization to the ONL is consistent with their identities as rods. Furthermore, 1D1+ outer segments in control and regenerated retina were co-labeled with GFP (Fig. 7b-d, f-h, j-l, arrowheads), suggesting that regenerated, GFP+ cells in the xops:eGFP zebrafish retina corresponded to regenerated rods.
Fig. 7
Fig. 7

Regenerated rods in xops:eGFP transgenic zebrafish. a Undamaged retina, showing GFP+ (green); rod cell bodies in the outer nuclear layer (ONL) and GFP+, rhodopsin (1D1, magenta) outer segments (OS). Section is counterstained with DAPI (nuclei; blue). Asterisks (*) highlight some of the GFP+, DAPI+ cell bodies in the outer nuclear layer (ONL). Boxed area is shown at higher magnification in (b-d). b-d. Higher magnification views of outer segments of GFP imaging channel only (b), rhodopsin only (c), and a merged image (d), to show colabeling of outer segments (OS; some are highlighted by arrowheads). e-h Regenerated retina processed 14 days after injury (14 dpi), low magnification view with GPF, rhodopsin, and DAPI (e), and higher magnification views of GFP (f), rhodopsin (g), and merged image (h), to show colabeling of outer segments in regenerated retina (some are highlighted by arrowheads). Arrow in e shows example of histological error, with a cluster of DAPI+ cell bodies misplaced in the inner plexiform layer (IPL). i-l Regenerated retina processed 30 days after injury (30 dpi), low magnification view with GPF, rhodopsin, and DAPI (i), and higher magnification views of GFP (j), rhodopsin (k), and merged image (l), to show colabeling of outer segments in regenerated retina (some are highlighted by arrowheads). Boxed area in (i) is shown at higher magnification in (j-l). In b-d, f-h, and j-k, note that GFP fluorescence can be brighter than the corresponding 1D1 fluorescence, or vice-versa, although all OS show colabeling. Scale bar in a (applies to a, e, i) = 20 μm. Scale bar in b (applies to b-d, f-h, j-l) = 20 μm. OPL, outer plexiform layer; INL, inner nuclear layer; GCL, ganglion cell layer

Regenerated xops:eGFP retinas were dissociated, FACS-sorted, and subjected to qPCR of selected transcripts. Transcripts that were detected as significantly rod-enriched in undamaged retinas were also significantly rod-enriched in regenerated retinas at 14 and 30 dpi (Fig. 8a), providing an initial indication that regenerated rods are similar at the transcript level as the undamaged rods. Both rho and rhol were more highly enriched in the regenerating rods, and nrl was more highly enriched at 14 dpi (Fig. 8a). Rxrgb was detected, but not differentially expressed, in all samples, while rxrga was significantly depleted in rods of undamaged retina and at 14 dpi, but not 30 dpi (Fig. 8b). Thrb, important for determination of red-sensitive cones [51] was detected, but highly significantly depleted in all samples (Fig. 8b). Together these findings suggest that the rod transcriptome in regenerated retina possibly carries a molecular signature similar to that of undamaged rods.
Fig. 8
Fig. 8

qPCR of selected transcripts enriched (a), or present (and not differentially expressed) or present (and depleted) in GFP+ (rod photoreceptor) cells (b), in regenerated retinas at 14 days post-injury (dpi), 30 dpi, and in undamaged retinas. **, p < 0.01; *, p < 0.05; ns, not significantly differentially expressed, for GFP+ vs. GFP- (three biological replicates)

Discussion

We report for the first time, transcripts enriched, present, and depleted in rod photoreceptors of the adult zebrafish retina, now available as a resource for other investigators with interests in rod health, structure, function, and neurogenesis. The dataset was validated by qPCR of 45 transcripts, and many transcripts present in rods were not previously recognized as rod-enriched. Analysis of FACS-sorted fluorescent rods from transgenic zebrafish appears to be an excellent approach for expanding our knowledge of rod biology, and in the future may be applied to other photoreceptor subpopulations [63], since there are numerous transgenic tools available that selectively fluorescently label specific cone subtypes [64, 65].

The rod transcriptome appears to be remarkably stable over the zebrafish lifespan, at least for the rod-enriched transcripts studied in this manner, and at the sampling times used. The rod population of adult zebrafish, which includes the rods generated larvally – these rods are nearly as old as the zebrafish themselves – as well as the many rods that accumulated through adulthood, likely carries a molecular signature similar to that of the newly-generated rods of larval retina. The potential exceptions are the transcripts encoding the visual pigment proteins themselves, rho and rhol. Rho is more abundant in the rods from older fish, where the rod population includes many older rods. However, rhol is more abundant in those of younger fish. Interestingly, the peak spectral sensitivity of rhol is shifted 5 nm shorter than that of rho [48], although it is not known whether this difference is meaningful in the visual environment of zebrafish when rods are utilized. It is possible that the higher levels of rhol in rods of younger zebrafish are important for a visually-mediated behavior such as a prey capture strategy, that is different in larval/juvenile vs. adult zebrafish [66]. Extending the unbiased RNA-seq approach for the study of rod transcripts over the zebrafish lifespan may reveal other functional changes.

We used two approaches to evaluate rod transcripts in situations where the zebrafish retina responds to rod damage. In the first approach, we analyzed selected rod-enriched, and rod-depleted genes in WT retinas vs. those with chronic loss and attempted replacement of rods (xops:mCFP) [9]. Some of these rod-enriched transcripts were upregulated in WT retinas vs. xops:mCFP, consistent with the lack of mature rods in the xops:mCFP retinas. However, some were not, pointing to alternative roles for these transcripts in some aspect of the response to chronic damage, for example in the environment of high levels of cell death, or in upregulation of rod precursor proliferation. The second approach was to analyze selected rod-enriched, and rod-depleted genes following widespread retinal damage and a regeneration period. We found that transcripts enriched in undamaged, native rods, also were enriched in regenerated rods. Again the extension of the unbiased RNA-seq approach is likely to be even more illuminating, but this initial result suggests that regenerated rods do not differ in expression of a set of selected transcripts in comparison with undamaged, native rods. This finding implies that regenerated retinal neurons may not carry with them alternative molecular signatures, and likely recover their distinctive functions [67].

Conclusions

We report the generation and validation of an RNA-seq dataset describing the rod transcriptome of the zebrafish. This transcriptome appears stable across the zebrafish lifespan, and similar in regenerated rods as compared with undamaged rods. Future applications of this study include comparative photoreceptor transcriptomics (rods vs. each cone subtype), and comparative analysis with transcriptome information available from other model organisms including mouse [68], as well as from stem cell-derived human retinal organoids [69]. Such studies have potential to reveal further distinctions of cones vs. rods, and distinctions among vertebrates that may resolve questions of vertebrate photoreceptor evolution [25, 7072].

Abbreviations

CGZ: 

Circumferential germinal zone

CMZ: 

Ciliary marginal zone

DPF: 

Days post-fertilization

DPI: 

Days post-injury

FACS: 

Fluorescence-Activated Cell Sorting

GCL: 

Ganglion cell layer

GO: 

Gene ontology

INL: 

Inner nuclear layer

ONL: 

Outer nuclear layer

WT: 

Wild-type

Declarations

Acknowledgments

The authors are grateful to Dr. James Fadool for the xops:eGFP zebrafish, to Dr. Ann Morris for the xops:mCFP zebrafish, to Ms. Ann Norton of the UI IBEST Optical Imaging Core for assistance with FACS, to Mr. Dan New and Dr. Sam Hunter of the UI IBEST Genomics Core for RNA-Seq and assistance with bioinformatics. We thank Ruth Frey, William Thurston, Kirsie Lundholm (Stenkamp lab), and Joshua Sukeena (Fuerst lab) for technical assistance, and Dr. Diana Mitchell for retinal lesioning and for critical evaluation of earlier versions of the manuscript. The IBEST (Institute for Bioinformatics and Evolutionary Studies) Genomics Core is supported by NIH COBRE P30 GM103324.

Funding

Funding was provided by NIH R01 EY012346 (DLS), NIH R21 EY026814 (DLS), a Technology Access Grant (CS and DLS) available through Idaho’s NIH-INBRE program (supported by NIH P20 GM103408), and the Malcolm and Carol Renfrew Faculty Fellowship (DLS). These funding bodies did not have roles in the design of the study and collection, analysis, and interpretation of data and in writing the manuscript.

Availability of data and materials

The RNA-Seq dataset is available at GEO under accession # GSE100062. Other data generated or analyzed during this study are included in this article and its additional information files.

Authors’ contributions

CS performed animal husbandry, FACS-sorting, RNA isolation, and qPCR, and contributed to writing the manuscript. CG performed animal husbandry, tissue processing, probe preparation, and in situ hybridization, confocal microscopy, and contributed to writing the manuscript. DLS and CS conceived of the study, and DLS wrote the manuscript. All authors read and approved the final manuscript.

Ethics approval and consent to participate

All studies involving zebrafish were approved by the University of Idaho’s Animal Care and Use Committee.

Consent for publication

Not applicable.

Competing interests

The authors declare that they have no competing interests.

Publisher’s Note

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Open AccessThis article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated.

Authors’ Affiliations

(1)
Department of Biological Sciences, University of Idaho, 875 Perimeter Drive, MS 3051, Moscow, ID 83844-3051, USA

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