- Research article
- Open Access
Profiling sex-biased gene expression during parthenogenetic reproduction in Daphnia pulex
© Eads et al; licensee BioMed Central Ltd. 2007
- Received: 13 May 2007
- Accepted: 18 December 2007
- Published: 18 December 2007
Sexual reproduction is a core biological function that is conserved throughout eukaryotic evolution, yet breeding systems are extremely variable. Genome-wide comparative studies can be effectively used to identify genes and regulatory patterns that are constrained to preserve core functions from those that may help to account for the diversity of animal reproductive strategies. We use a custom microarray to investigate gene expression in males and two reproductive stages of females in the crustacean Daphnia pulex. Most Daphnia species reproduce by cyclical parthenogenesis, alternating between sexual and clonal reproduction. Both sex determination and the switch in their mode of reproduction is environmentally induced, making Daphnia an interesting comparative system for the study of sex-biased and reproductive genes.
Patterns of gene expression in females and males reveal that 50% of assayed transcripts show some degree of sex-bias. Female-biased transcription is enriched for translation, metabolic and regulatory genes associated with development. Male-biased expression is enriched for cuticle and protease function. Comparison with well studied arthropods such as Drosophila melanogaster and Anopheles gambiae suggests that female-biased patterns tend to be conserved, whereas male-biased genes are evolving faster in D. pulex. These findings are based on the proportion of female-biased, male-biased, and unbiased genes that share sequence similarity with proteins in other animal genomes.
Some transcriptional differences between males and females appear to be conserved across Arthropoda, including the rapid evolution of male-biased genes which is observed in insects and now in a crustacean. Yet, novel patterns of male-biased gene expression are also uncovered. This study is an important first step towards a detailed understanding of the genetic basis and evolution of parthenogenesis, environmental sex determination, and adaptation to aquatic environments.
- Codon Usage
- Mature Female
- Codon Usage Bias
- Juvenile Female
- Relative Synonymous Codon Usage
Differences between males and females have fascinated biologists and stimulated research for many years, yet detailed molecular explorations of sexually dimorphic phenotypes are available for only a few organisms (cf. [1–5]). Among the insects, sex-biased gene expression is particularly well studied in Drosophila [6–13]. This research reveals that a large proportion of the transcriptome is sex-biased [2, 10, 12], and that most of these differences can be ascribed to divergence in the germ line [6, 11]. Furthermore, sex is a much stronger determinant of transcript levels than an animal's ontogeny , age, or genotype . These studies also find that, overall, male-biased genes are evolving more rapidly than female-biased genes [9, 13, 14], providing evidence that males experience stronger positive selection than females [8, 12]. In addition, male genes are under-represented on the X chromosome of D. melanogaster . To date, the generality of these findings for arthropods is not clear. Recent studies of Anopheles gambiae [3, 16] report that a large proportion of gene expression is sex-biased and shows similar functional patterns to the female-biased gene set in flies. For example, females of both insects tend to express genes involved in ribosome function, translation initiation, and DNA replication at a higher level than males . However, genes expressed at a two-fold or greater difference in Drosophila tend to be male-biased . In contrast, 71% of highly biased genes are enriched in Anopheles females . Further comparative experimental work is required to better understand the evolution of sex-biased gene expression.
Genome sequencing projects serve to underscore both the unity of eukaryotic organization as well as its amazing diversity. Functional characterization of genomes demonstrates that significant portions of gene inventories are preserved, which accounts for many of the core biological attributes defining large classes of organisms. In practice, comparative data from closely related species are a useful resource to ascribe tentative functions to conserved genomic elements, as studies of insects have begun to demonstrate [17, 18]. Yet, investigations that include species from the other major lineages of arthropods (chelicerates and crustaceans) are equally important to discern insect-specific and arthropod-specific differences, and to infer ancestral versus derived conditions. Crustaceans are an amazingly varied group encompassing over 38,000 known species , and constitute a significant portion of animal communities in aquatic environments. Amongst crustaceans, the "water flea" Daphnia is arguably the best studied and has traditionally been an important model for ecology, population genetics, evolutionary biology, and toxicology . Although these studies have focused on a variety of aspects of Daphnia biology, including phylogeography, functional morphology, physiology and life history evolution, genomic investigations have begun only recently . A few large-scale studies of gene expression patterns in Daphnia have been published [22, 23], but molecular studies have mostly been confined to a limited number of allozymes, sequence-tagged sites (STS), or genes [24, 25]. Interest in crustacean biology per se, as well as their phylogenetic position as an outgroup to other well studied arthropods (Drosophila, Apis, Anopheles), emphasize the relevance of Daphnia in comparative genomic studies.
Several features of Daphnia biology make them an interesting subject of investigation in comparative functional genomics. Females typically reproduce by apomixis (parthenogenesis), depositing multiple embryos into a dorsal brood pouch that develop and hatch within about 48 hours . Adverse environmental conditions such as crowding, lowered temperature or food scarcity can induce either male production (males are genetic copies of their mothers), or haploid gametes that are fertilized and overwinter in a state of diapause. Male production is known to be under the control of endocrine factors during oocyte maturation, and can be induced by juvenile hormone analogs such as the insecticides pyriproxyfen and fenoxycarb . The ability to produce either males or haploid (sexual) eggs has been lost independently in multiple lineages of Daphnia, suggesting a simple genetic mechanism. In D. pulex, current data support the existence of a dominant allele conferring obligate asexuality in females but not in males , which has been spreading into North America from the northeast to the midwest . As a step towards understanding these processes at a molecular level, here we specifically address the question of conservation of gene expression patterns and protein evolution in sex-biased genes.
We report here on gene expression profiles of D. pulex, an emerging model for functional genomics, by measuring transcription levels in males and females at two stages of development using a custom cDNA microarray. We compare the gene expression profiles of D. melanogaster to those of D. pulex to discover conserved elements of sex-specific transcriptional regulation. Analysis of the patterns associated with sex-bias also reveals a conserved trend in male-biased genes to be evolving faster than female-biased.
Profiling sex- and parthenogenesis- biased gene expression
Our study represents the first description of global patterns of sex-biased transcription in a crustacean species, and we analyzed our results using two major approaches. First, we compared our male and female profiles to each other and to published studies of other arthropods using annotated gene ontology functions and processes. Secondly, we used an evolutionary approach to assess patterns of sequence conservation and sex bias. Furthermore we tested mature females carrying their first brood as well as juvenile females, whose ovaries are beginning the reproductive cycle, in order to examine embryogenesis as well as oogenesis.
We used the number of array elements and assembled sequences, fully described in reference , to estimate the number of unique genes differentially expressed in each comparison (Table 1). When data from the male-mature female and male-juvenile female experiments were pooled, a total of 81% (1,270) of genes shows statistically significant sex-biased gene expression with an estimated false discovery rate of 5% (Table 1). With a more conservative threshold of both at least a two-fold difference and statistical significance, a total of 45% (698) of genes, corresponding to 1,355 array elements, showed sex-biased gene expression (Table 1). This overall pattern is consistent with previous studies of other arthropods [2, 3, 12]. Additionally, there were almost three times as many male enriched genes compared to female enriched genes (957 versus 313, Table 1). However, at a two-fold or greater expression difference the proportion of male-biased transcription declined substantially (431 male biased and 267 female biased).
Differentially expressed genes in male and female D. pulex
Mature Enriched vs. Male
Mature Depleted vs. Male
Juvenile Enriched vs. Male
Juvenile Depleted vs. Male
Self vs. Self
Male enriched vs. Female
Female Enriched vs. Male
Mature enriched vs. Juvenile
Juvenile enriched vs. Mature
Estimated Non-redundant Genes†
Estimated Non-redundant Genes†
A closer examination revealed important differences between the patterns of sex-biased gene expression in juvenile and mature females. At the gross level, both males and mature females displayed a paucity of highly differentially expressed genes relative to juvenile females. Mature females expressed 21% of genes and juvenile females expressed 23% of genes at a two-fold or lower level relative to males (Table 1). By comparison, at a two-fold or higher level, males expressed 15% of genes more highly than mature females but only 0.6% of genes more highly than juvenile females. It is important to note that the arrayed cDNA libraries were made from mixed cultures comprised predominantly of females, and consequently are expected to under-represent male-specific and strongly male-biased genes. As males are a common reference, this indicates that a significant number of genes were also differentially expressed in juvenile females relative to mature females.
Functional categories of differentially expressed genes
The role of homology in inferring putative function for unknown gene sequences is well established and is the basis for annotation using a structured vocabulary such as the popular gene ontology, or GO [34, 35]. One reason for this popularity is the ability to statistically test associations between GO annotations and gene expression measurements, although unfortunately no ontological or methodological approach can be considered optimal [36–38]. To investigate whether differentially expressed genes have a non-random representation of functional categories with respect to each other, we analyzed the occurrences of GO terms in each of the classes of differentially expressed genes (using assembled sequences only, so redundant sequences were not counted twice). We extracted the GO terms of the best Blast match in the GenBank NR database, and analyzed the relative frequency of differentially expressed genes to the reference set of all data using Fisher's exact test implemented in Blast2GO .
Analysis of GO term enrichment in juvenile compared to mature females reveals differences that can be ascribed to embryogenesis. Specifically, while juvenile females show a paucity of categories enriched vs. mature females, mature females are enriched for a number of GO terms (5C, 5D). Over-represented GO terms in juvenile females include lytic vacuole, lysosome, vacuole, structural molecule activity, carbohydrate metabolism, and structural constituent of cuticle (Fig. 5C). Both males and juvenile females, which are approximately half the size of mature females, are significantly enriched for exoskeletal-associated gene function. This enrichment may be a simple consequence of larger surface area/volume ratios, which presumably require a higher concentration of cuticular proteins per unit mass. For mature females, enriched GO categories include those related to DNA packaging as well as transcription (Fig. 5D). Other GO terms are associated with amino acid metabolism and organelle function. In addition, various types of regulation are associated with mature females, including regulation of nucleic acid metabolism, primary metabolism, transcription, and physiological process.
GO term comparisons between males and mature females further illustrate important differences related to embryogenesis. Juvenile-enriched categories represent a subset of the female-enriched vs. male comparison (not shown). In contrast, mature-enriched GO terms include some categories not seen in other comparisons (Fig. 5E). For instance, many terms associated with purine nucleotide functions are overrepresented, such as GTPase activity and purine binding. Another set of terms involves microtubule function, such as microtubule binding and polymerization, and to transcriptional regulation (Fig. 5E).
Conservation of sex-biased gene expression
Rapid evolution of male-biased genes may be due to either relaxation of selective pressure, or to increased positive selection favoring sequence divergence. One prediction of the former hypothesis is increased codon usage bias in slowly evolving genes , which could cause a spurious correlation between transcription and rate of evolution. To test this idea, we used correspondence analysis  to analyze codon usage statistics for male-biased, female-biased, and unbiased genes, using a conservative cutoff of four-fold difference for biased genes. We found no difference in codon usage bias between these classes as measured by frequency of optimal codons (Fop), codon bias index (CBI), codon adaptation index (CAI), or relative synonymous codon usage either at a four-fold cutoff, or at a more relaxed two-fold cutoff (data not shown). Additionally, correlations between third position GC content and Fop (r2 = 0.47; p < 0.05) or CBI (r2 = 0.56; p < 0.01) indicate GC content is likely to be causing major trends in codon usage among these genes . These observations show that for the genes in our data set, selection on codon usage is not a cause of the relationship between protein evolution and expression bias.
Gene expression analysis of males and females
Sexual reproduction is a core biological function and recent genome-wide studies of sexual dimorphism and gametogenesis in model metazoans have revealed several recurring patterns. (i) A very large proportion of the transcriptome shows some level of sex-biased gene expression [4, 5, 11]. (ii) The most profound sex-biased gene expression is found in the germ line [1, 4, 6, 11]. (iii) Sex-biased genes are non-randomly distributed among sex-chromosomes and autosomes [15, 47]. (iv) Male-biased genes show accelerated patterns of evolution [9, 13]. Two features of D. pulex make it particularly interesting for a comparative study of sex-biased and reproductive genes. First, D. pulex are cyclically parthenogenetic, alternating sexual and asexual rounds of reproduction. Second, sex determination is environmentally induced, as males are genetically identical to their mothers (sexual reproduction results in female offspring). Thus in D. pulex, we expect to find the patterns of sex-biased gene expression common to the arthropods overlaid with changes associated with parthenogenetic oogenesis and environmental sex determination.
As a first step in understanding the genetic basis of the D. pulex reproductive system, we profiled the expression of genes differentially expressed in males compared to parthenogenetically reproducing females. Daphnia oogenesis proceeds with a clutch of oocytes undergoing development in the ovaries, while embryos develop in the brood chamber . Shortly after molting, which releases young from the brood chamber, newly vitellogenic eggs from the ovary are deposited into the brood chamber. In the intervening intermolt period, embryonic development and vitellogenesis proceed in the brood chamber and ovary, respectively. Thus, females reproducing parthenogenetically contain both developing egg chambers as well as developing embryos. In contrast, juvenile females generally contain pre-vitellogenic oocytes but no embryos . Therefore, we compared males to both juvenile females and females carrying embryos in order to partition the embryonic component from the two female types, while simultaneously ensuring a comparison with reproductively capable females.
Males used in these experiments were treated identically and showed no systematic differences in the two experiments, so the low level of two-fold differential expression in the male-juvenile female comparisons must reflect a higher level of transcript present in juvenile vs. mature females. The paucity of highly differentially expressed genes in males vs. juvenile females is likely due in part to having few male-specific transcripts on the arrays. Gene expression due to oogenesis, occurring in both juvenile and mature females, and embryogenesis, which occurs only in mature females, also shows an important contribution from embryos. Of the functional annotations of embryo-associated genes, the most prominent are related to DNA metabolism and transcription, and to microtubule function. It is interesting that in other arthropod male-female comparisons, microtubule function is male-enriched, presumably due to spermatic function . It is not clear why Daphnia embryos are so highly enriched for this ubiquitous protein. Future studies of gene expression across the life cycle of D. pulex should shed light on specific embryonic genes and pathways, and provide useful insights into comparative developmental genomics of arthropods.
Patterns of sequence conservation and sex-biased gene expression in D. pulex are broadly similar to those seen in comparable studies of Anopheles gambiae and D. melanogaster. In particular, we found a high proportion (roughly 50%) of sex-biased expression among genes on our array, similar to other reports [3, 7, 12, 16], with large numbers of both male- and female-biased genes. It is interesting that, in spite of potential bias toward discovering female-enriched genes on our arrays due to the nature of the arrayed cDNA library, we found a large number of genes to be male-biased. Functional categories overrepresented in males were associated with cuticle metabolism and protease function, which contrasts to the situation seen in adult mosquitoes . We speculate that increased cuticle metabolism in males and juvenile females is a result of allometry (mature females being roughly double the size), although we cannot rule out the possibility of differences in cuticular composition or structure. Higher expression of proteases in males also differs from A. gambiae, in which female transcripts were enriched for genes associated with blood feeding, such as salivary gland proteins . In mice, immune-related gene expression is also lower in testes than ovaries, although the reason for this difference is unknown . Some proteases with higher expression in D. pulex males are homologous to digestive enzymes, but there are also clear examples of homologs of defence response proteins, as well as non-proteolytic members of these signaling pathways. It is not clear whether male Daphnia have a greater need for protease activity for defence, immune signaling, or metabolism. Finally, although males have higher mass-specific metabolism than females , females rather than males are enriched for energy metabolism-annotated GO categories.
Some of the biological processes overrepresented in female D. pulex are similar to those in other arthropods, such as translation elongation, ribosomal function, and DNA packaging. In comparing conserved sex-biased genes in D. pulex and D. melanogaster, we found 31 male-biased, 86 female-biased and 32 genes with opposite bias. These differences are on the same order as differences found in comparing D. melanogaster to D. simulans , where 20% of the genes studied had changed sex-biased expression between species. In marked contrast, Hahn and Lanzaro  found only 4 orthologs that had sex-biased expression in both Anopheles and Drosophila. Discrepancy between this finding and our study probably reflects the two-fold cutoff used in the Anopheles study , and difficulty in assigning orthologs to rapidly evolving male-biased genes. However, it is clear that proteins involved in translation and DNA packaging are female-biased in expression among flies, mosquitoes and Daphnia.
We found a difference in the degree of conservation between female and male-biased genes, similar to studies showing that female-biased genes tend to be better conserved than male-biased genes [9, 14]. Data from population genetic studies indicate an increase in positive selection on male biased genes, which also have a significantly lower level of codon bias than female-biased genes. These findings were recently extended by Zhang and colleagues , who analyzed polymorphism levels for sex-biased and unbiased genes in several Drosophila species. Their results demonstrate an accelerated rate of evolution for male-biased genes, and that these genes are more often subject to positive selection . It is clear that for genes in our data set, selection on codon usage is not driving differences in evolutionary rates, nor is it causing a spurious correlation between bias and rate. However, it is possible that our data set was too small to detect codon usage differences.
Future studies should focus on examining differences in population polymorphism and species divergence, for example in the nonsynonymous/synonymous polymorphism ratio in biased genes between populations of D. pulex and D. magna, a congener for which cDNA data are accumulating rapidly. This comparison would distinguish between relaxed selective constraints or increased positive selection on male genes. The ability to control for chromosomal effects makes a useful comparison to chromosomally-determined systems, in distinguishing whether linkage or some other mechanism is responsible. Another central question is whether male-biased genes are mutationally degenerating in non-male producing obligate asexual lines, and we identify candidate genes for such research. Finally, comparing parthenogenetic reproduction to sexual reproduction in this species should also yield interesting candidates for molecular evolutionary studies, and provide clues as to the mechanisms involved in these processes. The public release of the assembled D. pulex genome, combined with genetic mapping studies , should provide insight into the roles of recombination rate, chromosomal context, demographic history, and selection on shaping sequence divergence in sex-biased genes.
In this study, we analyze patterns of gene expression differences in D. pulex males, juvenile females, and pregnant females. We find patterns of sex-specific and pregnancy-specific expression across a substantial proportion of genes. Results suggest that patterns of female-biased expression are similar to those reported for D. melanogaster and A. gambiae, indicating conserved functional requirements across arthropods. Specifically, females express transcripts relating to protein metabolism, primary metabolism, and organelle function at a higher level than do males. Embryonic gene expression is enriched for processes related to DNA metabolism, transcription, and microtubule function. Male-biased transcription is over-represented with cuticle and protease functions, in contrast to other arthropods. We also find that male-biased genes are less likely to have identifiable homologs in sequence databases, consistent with faster evolution of male-biased genes.
We constructed the first D. pulex microarray. The arrays were printed with 3,602 PCR amplified cDNA clone inserts and 240 positive and negative controls, corresponding to 787 clusters of nuclear-derived genes as described . cDNA libraries were constructed as described elsewhere . The printed array elements were from a mixture of anonymous clones and clones with single pass 5' EST sequence reads. Fabrication of microarrays was conducted concurrently with EST sequencing, and we have sequenced 1,546 high-quality clones on the array to date. A detailed description of this platform has been submitted to the Gene Expression Omnibus at NCBI under the accession number GPL4349, series GSE5908. Not all of the arrayed clones were sequenced, and many genes were represented by multiple clones. Therefore, we define redundancy on the array as the proportion of unique sequences among our clones. Given approximately 57% redundancy among the sequenced clones , we estimate that the array contains 1,560 distinct D. pulex genes. From each library, 384 samples were PCR amplified from plasmid purified using the PerfectPrep kit (Eppendorf) and sequenced using BigDye (ABI; v.2) on an ABI 3730 sequencer. These samples served as a random sample for quality control in further analysis. Remaining samples (3,168 in all) were PCR amplified from colony picks of transformed bacterial cells. Template was generated by growing colonies in 1.2 ml of 2× YT and 0.005% chloramphenicol in 96-deepwell plates for 24 hours at 37°C. Reactions were run in 100 μl containing: 1× Taq buffer (Eppendorf), 0.2 mM dNTPs, 0.2 μM primers (Fwd. 5'-GTGTAAAACGACGGCCAGTAG 3' and Rev. 5'-AAACAGCTATGACCATGTTCAC 3'), 5 U Taq (Eppendorf), and 5 μl fresh bacterial growth or 2 μl purified plasmid. Quality of PCR amplifications was verified by gel electrophoresis and number and size of bands was recorded using Kodak's 1D imaging software (v.3.6). Concentration of samples was determined by 96-well microplate spectrophotometer (Molecular Devices SpectraMax 190) and adjusted to 50–200 ng/μl for printing.
A Genemachines Omnigrid 100 was used to print the D. pulex cDNA on GapsII aminosilane slides (Corning). The cDNA was printed in 3× SSC and 1.5 M Betaine buffer and deposited with Stealth Micro-Spotting Pins (Telechem) at 20°C and 65% humidity. The cDNA was fixed to the microarray slides by baking at 85°C for 3 hours. Slides were processed by agitating in 0.2 % SDS for 5 min. and in HPLC-grade water, 5 min at 21°C., followed by 2 min. in 95°C water, rinsing briefly in ice-cold 100% isopropanol, and centrifuging at 500 × g for 5 min. Five types of negative controls were printed, including printing buffer, failed PCR reaction with template DNA but no primers, ORFs from Arabidopsis and lambda phage, and bacterial PCR spikes (Ambion). Positive controls of D. pulex genes were printed next to printing buffer to assure no carryover, and included cytochrome c (subunits I, II, and III), cytochrome b, actin, and ferritin.
Animal Culturing and Experimental Design
Daphnia were reared in lake water at 20°C and a 10:14 light/dark cycle at a density of approximately 1 individual per 5 ml. Animals were fed Scenedesmus algae at approximately 0.1 mg ml-1 each day. Twenty animals of a single clone were exposed to 400 nM methyl farnesoate in methanol (60 μl L-1) to induce male production, while another 20 individuals were given a sham control of methanol and produced female offspring. Progeny were raised under conditions described above in eight beakers each for males and females, with about 25 individuals per beaker and inspected by microscopy to verify healthy appearance and correct sex. After six days, beakers containing juvenile females were sacrificed. After eight days, males and the remaining females (now carrying embryos in their brood pouches) were harvested as well. Total RNA was isolated using Trizol (Invitrogen) and RNeasy columns (Qiagen), including a DNase treatment performed on-column. Quality of total RNA preparations was assayed by spectrophotometry and electrophoresis through denaturing agarose gels.
Four biological replicates of juvenile females and adult females were compared to eight biological replicates of males. Two samples of each female replicate were labeled with red and two with green dye, and no technical replicates were performed. Eight total hybridizations were therefore performed.
Microarray Hybridization, Analysis, and Validation
Isolated total RNA (15 μg) was reverse-transcribed into first-strand cDNA using the SuperScriptIII indirect labeling kit (Invitrogen), and coupled to Alexa dyes 555 and 647 (Invitrogen). Incorporation was assessed by spectrophotometry and gel electrophoresis followed by image quantitation on a Typhoon phosphorimager (Molecular Dynamics). Results showed good incorporation of fluor, a size range of cDNA into the 1 kb range, and negligible amounts of unincorporated dye. Equal masses of cDNA from males and females were combined in a 1:3 volume with hybridization buffer (50% formamide, 5× SSC, 0.1% SDS, 10 μg calf thymus DNA) and denatured at 90°C for 4 min, quick chilled, and injected into a Lucidea Slidepro automated hybridization chamber (Amersham) containing a microarray slide pre-hybridized according to manufacturer's instructions. Following overnight hybridization, slides were washed twice at 60°C in 2× SSC + 0.2% SDS (15 min), once in 0.2× SSC + 0.2% SDS (10 min), once in 0.1× SSC (10 min) and once in 0.05× SSC (10 min). Slides were dipped briefly in 100% isopropanol, centrifuged 5 min at 500 × g to dry, and scanned using an Axon 4200B scanner.
Data were extracted using GenePix software (version 5.1) and imported into Bioconductor for normalization and analysis . Data were compared using multiple methods, including several Bioconductor packages. Data were normalized using OLIN  or limma  and differential expression was assessed with limma and EBarrays . Array elements are defined as differentially expressed in our analyses if they have a p-value less than 0.05 with a false discovery rate correction using the program linear models for microarrays (Limma)  implemented in Bioconductor .
We compared analyses using OLIN for normalization and EBarrays for differential expression, or using limma for both. Briefly, we examined assumptions of the analytical models using constant coefficient of variation and quartile-quartile plots, which showed reasonably good fits. However, certain contrasts in EBarrays were not as well fit as others for our experimental dataset, so we used the linear model framework. We performed normalizations using print-tip loess normalization with no background subtraction after genes < 2 S.D. above median background were filtered out. Gene ontology category assignment and analysis was performed using the program Blast2GO , with input data consisting of assembled sequences called as differentially expressed by Limma using a 5% false-discovery rate. Codon statistics were generated using correspondence analysis  as implemented in the program codonW . For these analyses, significantly differentially expressed genes were binned as biased if the male-female difference in both juvenile and mature comparisons was greater than 4-fold (arithmetic scale).
For clarity, we describe gene expression patterns in terms of (i) the number of array elements (to distinguish from spots, which are printed in duplicate), (ii) the number of sequenced, non-redundant genes (which we also call "assembled" sequences) and (iii) the estimated number of unique genes represented by those elements.
Quantitative PCR assays were performed with the SuperScript III Real-time PCR kit (Invitrogen) following manufacturer's protocol for 2-step amplification, using BioRad's I-cycler. Briefly, DNase-treated total RNA (200 ng) was reverse transcribed in 20 μl and amplified in duplicate samples from two separate RNA preparations. Reactions consisted of 200 μM dNTPs, 3 μM gene-specific primers, 1 μM fluorescein, and 2 U Taq. A standard curve was constructed using cDNA as template, and reactions were subjected to melt-curve analysis after amplification, which revealed a single band in each case. Reaction products were also subjected to agarose gel electrophoresis in some cases to verify amplification of a single species. Sequences of primers used were as follows: 01031D01 F 5'CGCTTCTTCTGCCTATCTGC 3';
01031D01R 5' GAAGAAAGCTGCGAATGTCC 3'; 02081H07F 5'
CGGAAATCCTTCCCACTACA 3'; 02081H07R 5'
GGGAGCGTAGTTGTCACCAT 3'; 01001A03F 5'
TTACCCATCTGCCGTCTACC 3'; 01001A03R 5'
GATTTAAACGGCAGCGAATC 3'; 02081G03F 5'
TCCACTGACATTGGCGTTTA 3'; 02081G03R 5'
CCAAATCATTGGCAAATTCC 3'; 02102C08F 5'
02102C08R 5' TCGGGCTTCATGTTATCTCC 3'.
This project was financed by collaborative grants from the National Science Foundation (DEB 0221837 and FIBR 0328516) and by seed funds from The Center for Genomics and Bioinformatics (CGB), supported in part by the Indiana Genomics Initiative (INGEN) under the Lilly Endowment. Computer support was provided by Phillip Steinbachs and Sumit Middha at The Center for Genomics and Bioinformatics and by Dick Repasky at the Indiana University Information Technology Services. We thank Darren Bauer, Kelley Thomas and Jim Haney (University of New Hampshire), Michael Lynch (Indiana University), Joe Shaw, Josh Hamilton, and Celia Chen (Dartmouth College) for their assistance with this project. Don Gilbert (Indiana University) and Rupali Patwardhan (CGB) provided important bioinformatics support. This work benefits from and contributes to the Daphnia Genomics Consortium.
- Li Y, Chia J, Bartfai R, Christoffels A, Yue G, Ding K, Ho M, Hill J, Stupka E, Orban L: Comparative analysis of the testis and ovary transcriptomes in zebrafish by combining experimental and computational tools. Comparative and Functional Genomics. 2004, 5: 403-418. 10.1002/cfg.418.PubMed CentralPubMedView ArticleGoogle Scholar
- Arbeitman M, Furlong E, Imam F, Johnson E, Null B, Baker B, Krasnow M, Scott M, Davis R, White K: Gene expression during the life cycle of Drosophila melanogaster. Science. 2000, 297: 2270-2275. 10.1126/science.1072152.View ArticleGoogle Scholar
- Marinotti O, Calvo E, Nguyen Q, Dissanayake S, Ribeiro J, James A: Genome-wide analysis of gene expression in adult Anopheles gambiae. Insect Molecular Biology. 2006, 15 (1): 1-12. 10.1111/j.1365-2583.2006.00610.x.PubMedView ArticleGoogle Scholar
- Reinke V, Gil I, Ward S, Kazmer K: Genome-wide germ line-enriched and sex-biased expression profiles in Caenorhabditis elegans. Development. 2004, 131 (2): 311-323. 10.1242/dev.00914.PubMedView ArticleGoogle Scholar
- Rinn J, Snyder M: Sexual dimorphism in mammalian gene expression. Trends in Genetics. 2005, 21 (5): 298-305. 10.1016/j.tig.2005.03.005.PubMedView ArticleGoogle Scholar
- Andrews J, Bouffard GG, Cheadle C, Lü J, Becker KG, Oliver B: Gene discovery using computational and microarray analysis of transcription in the Drosophila melanogaster testis. Genome Res. 2000, 10 (12): 2030-2043. 10.1101/gr.10.12.2030.PubMed CentralPubMedView ArticleGoogle Scholar
- Arbeitman M, Fleming A, Siegal M, Null B, Baker B: A genomic analysis of Drosophila somatic sexual differentiation and its regulation. Development. 2004, 131: 2007-2021. 10.1242/dev.01077.PubMedView ArticleGoogle Scholar
- Connallon T, Knowles L: Intergenomic conflict revealed by patterns of sex-biased gene expression. Trends in Genetics. 2005, 21 (9): 495-499. 10.1016/j.tig.2005.07.006.PubMedView ArticleGoogle Scholar
- Hambuch T, Parsch J: Patterns of synonymous codon usage in Drosophila melanogaster genes with sex-biased expression. Genetics. 2005, 170: 1691-1700. 10.1534/genetics.104.038109.PubMed CentralPubMedView ArticleGoogle Scholar
- Jin W, Riley R, Wolfinger R, White K, Passador-Gurgel G, Gibson G: The contributions of sex, genotype and age to transcriptional variance in Drosophila melanogaster. Nature Genetics. 2001, 29: 389-395. 10.1038/ng766.PubMedView ArticleGoogle Scholar
- Parisi M, Nuttall R, Edwards P, Minor J, Naiman D, Lu J, Doctolero M, Vainer M, Chan C, Malley J: A survey of ovary-, testis-, and soma-biased gene expression in Drosophila melanogaster adults. Genome Biology. 2004, 5: R40-10.1186/gb-2004-5-6-r40.PubMed CentralPubMedView ArticleGoogle Scholar
- Ranz J, Castillo-Davis C, Meiklejohn C, Hartl D: Sex-dependent gene expression and evolution of the Drosophila transcriptome. Science. 2003, 300: 1742-1745. 10.1126/science.1085881.PubMedView ArticleGoogle Scholar
- Zhang Z, Hambuch T, Parsch J: Molecular evolution of sex-biased genes in Drosophila. Journal Molecular Evolution. 2005, 21 (11): 2130-2139. 10.1093/molbev/msh223.View ArticleGoogle Scholar
- Davis J, Brandman O, Petrov D: Protein evolution in the context of Drosophila development. Journal Molecular Evolution. 2005, 60: 774-785. 10.1007/s00239-004-0241-2.View ArticleGoogle Scholar
- Parisi M, Nuttall R, Naiman D, Bouffard G, Malley J, Andrews J, Eastman S, Oliver B: Paucity of genes on the Drosophila X chromosome showing male-biased expression. Science. 2003, 299: 697-700. 10.1126/science.1079190.PubMed CentralPubMedView ArticleGoogle Scholar
- Hahn M, Lanzaro G: Female-biased gene expression in the malaria mosquito Anopheles gambiae. Current Biology. 2005, 15 (6): R192-R193. 10.1016/j.cub.2005.03.005.PubMedView ArticleGoogle Scholar
- Whitfield C, Band M, Bonaldo M, Kumar C, Liu L, Pardinas J, Robertson H, Soares M, Robinson G: Annotated Expressed sequence tags and cDNA microarrays for studies of brain and behaviour in the honey bee. Genome Research. 2002, 12: 555-566. 10.1101/gr.5302.PubMed CentralPubMedView ArticleGoogle Scholar
- Zdobnov E, von Mering C, Letunic I, Torrents D, Suyama M, Copley R, Christophides G, Thomasova D, Holt R, Subramanian G, Mueller H, Dimopolous G, Law J, Wells M, Birney E, Charlab R, Halpern A, Kokoza E, Kraft C, Lai Z, Lewis S, Louis C, Barillas-Mury C, Nusskern D, Rubin G, Salzberg S, Sutton G, Topalis P, Wides R, Wincker P, Yandell M, Collins F, Ribeiro J, Gelbart W, Kafatos F, Bork P: Comparative genome analysis and proteome analysis of Anopheles gambiae and Drosophila melanogaster. Science. 2002, 298: 149-159. 10.1126/science.1077061.PubMedView ArticleGoogle Scholar
- Brusca G, Brusca , Thomas : Invertebrates. 2002, Sunderland, MA: Sinauer Associates, SecondGoogle Scholar
- Ebert D: Ecology, Epidemiology, and Evolution of Parasitism in Daphnia. National Library of Medicine, National Center for Biotechnology Information. 2005Google Scholar
- Eads BD, Andrews J, Colbourne JK: Ecological genomics in Daphnia: stress responses and environmental sex determination. Heredity. 2007, [Epub ahead of print]Google Scholar
- Soetaert A, Moens L, van der Ven K, van Leemput K, Naudts B, Blust R, de Coen W: Molecular impact of propiconazole on Daphnia Magna using a reproduction-related cDNA array. 2006, 142: 66-76.Google Scholar
- Watanabe H, Tatarazako N, Oda S, Nishide H, Uchiyama I, Morita M, Iguichi T: Analysis of expressed sequence tags of the water flea Daphnia magna. Genome. 2005, 48: 606-609. 10.1139/g05-038.PubMedView ArticleGoogle Scholar
- Lynch M, Pfrender M, Spitze K, Lehman N, Hicks J, Allen D, Latta L, Ottene M, Bogue F, Colbourne J: The quantitative and molecular genetic architecture of a subdivided species. Evolution. 1999, 53 (1): 100-110. 10.2307/2640923.View ArticleGoogle Scholar
- Penton E, Crease T: Evolution of the transposable element Pokey in the ribosomal DNA of species in the subgenus Daphnia (Crustacea: Cladocera). Molecular Biology Evolution. 2004, 9: 1727-1739. 10.1093/molbev/msh189.View ArticleGoogle Scholar
- Zaffagnini F: Reproduction in Daphnia. Memoirie Instituto Italiano Idrobiologia. 1987, 45: 245-284.Google Scholar
- Tatarzako N, Oda S, Watanabe H, Morita M, Iguchi T: Juvenile hormone agonists affect the occurrence of male Daphnia. Chemosphere. 2003, 53: 827-833. 10.1016/S0045-6535(03)00761-6.View ArticleGoogle Scholar
- Innes D, Hebert P: The origin and genetic basis of obligate parthenogenesis in Daphnia pulex. Evolution. 1988, 42 (5): 1024-1035. 10.2307/2408918.View ArticleGoogle Scholar
- Paland S, Colbourne J, Lynch M: Evolutionary history of contagious asexuality in Daphnia pulex. Evolution. 2005, 59 (4): 800-813.PubMedView ArticleGoogle Scholar
- Colbourne J, Eads B, Shaw J, Bohuski E, Bauer D, Andrews J: Sampling Daphnia's expressed genes: preservation, expansion and invention of crustacean genes with reference to insect genomes. BMC Genomics. 2007, 8: 217-10.1186/1471-2164-8-217.PubMed CentralPubMedView ArticleGoogle Scholar
- Rajeevan M, Ranamukhaarachchi D, Vernon S, Unger E: Use of real-time quantitative PCR to validate the results of cDNA array and Differential Display PCR technologies. Methods. 2001, 443-451. 10.1006/meth.2001.1266. 25Google Scholar
- Yuen T, Wurmbach E, Pfeffer R, Ebersole B, Sealfon S: Accuracy and calibration of commercial oligonucleotide and custom cDNA microarrays. Nucleic Acids Research. 2002, 30 (10): e48-10.1093/nar/30.10.e48.PubMed CentralPubMedView ArticleGoogle Scholar
- Smyth G: Linear models and empirical Bayes methods for assessing differential expression in microarray experiments. Statistical Applications in Genetics and Molecular Biology. 2004, 3 (1): Article 1-10.2202/1544-6115.1027.View ArticleGoogle Scholar
- Consortium GO: Gene Ontology: tool for the unification of biology. Nature Genetics. 2000, 25: 25-29. 10.1038/75556.View ArticleGoogle Scholar
- Xie H, Wasserman A, Levine Z, Novik A, Grebinskiy V, Shoshan A, Mintz L: Large-scale protein annotation through Gene Ontology. Genome Research. 2002, 12: 785-794. 10.1101/gr.86902.PubMed CentralPubMedView ArticleGoogle Scholar
- Al-Shahrour F, Diaz-Uriarte R, Dopazo J: FatiGO: a web tools for finding significant associations of Gene Ontology terms with groups of genes. Bioinformatics. 2004, 20 (4): 578-580. 10.1093/bioinformatics/btg455.PubMedView ArticleGoogle Scholar
- Hosack D, Dennis G, Sherman B, Lane H, Lempecki R: Identifying biological themes with lists of genes with EASE. Genome Biology. 2003, 4 (R70): R70-10.1186/gb-2003-4-10-r70.PubMed CentralPubMedView ArticleGoogle Scholar
- Khatri P, Bhavsar P, Bawa G, Draghici S: Onto-tools: an ensemble of web-accessible, ontology-based tools for the functional design and interpretation of high-throughput gene expression experiments. Nucleic Acids Research. 2004, W449-W456. 10.1093/nar/gkh409. 32 web serverGoogle Scholar
- Conesa A, Gotz S, Garcia-Gomez J, Terol J, Talon M, Robles M: Blast2GO: a universal tool for annotation, visualization and analysis in functional genomics research. Bioinformatics. 2005, 21 (18): 3674-3676. 10.1093/bioinformatics/bti610.PubMedView ArticleGoogle Scholar
- Lemos B, Meiklejohn C, Caceres M, Hartl D: Rates of divergence in gene expression profiles of primates, mice, and flies: stabilizing selection and variability among functional categories. Evolution. 2005Google Scholar
- Stuart J, Segal E, Koller D, Kim S: A gene-coexpression network for global discovery of conserved genetic modules. Science. 2003, 302: 249-255. 10.1126/science.1087447.PubMedView ArticleGoogle Scholar
- Nuzhdin S, Wayne M, Harmon K, McIntyre L: Common pattern of evolution of gene expression level and protein sequence in Drosophila. Molecular Biology Evolution. 2004, 21 (7): 1308-1317. 10.1093/molbev/msh128.PubMedView ArticleGoogle Scholar
- Subramanian S, Kumar S: Gene expression intensity shapes evolutionary rates of the proteins encoded by the vertebrate genome. Genetics. 2004, 168: 373-381. 10.1534/genetics.104.028944.PubMed CentralPubMedView ArticleGoogle Scholar
- Akashi H: Gene expression and molecular evolution. Current Opinion Genetics & Development. 2001, 11: 660-666. 10.1016/S0959-437X(00)00250-1.View ArticleGoogle Scholar
- Correspondence Analysis of Codon Usage. [http://codonw.sourceforge.net/]
- Sharp P, Matassi G: Codon usage and genome evolution. Current Opinion Genetics & Development. 1994, 4: 851-860. 10.1016/0959-437X(94)90070-1.View ArticleGoogle Scholar
- Wang J, McCarrey J, Yang F, Page D: An abundance of X-linked genes expressed in spermatogonia. Nature Genetics. 2001, 27: 422-426. 10.1038/86927.PubMedView ArticleGoogle Scholar
- Gilbert J, Williamson C: Sexual dimorphism in zooplankton (copepoda, cladocera, and rotifera). Annual Review of Ecology and Systematics. 1983, 14: 1-33. 10.1146/annurev.es.14.110183.000245.View ArticleGoogle Scholar
- Cristescu M, Colbourne J, Radivojac J, Lynch M: A microsatellite-based genetic linkage map of the waterflea, Daphnia pulex : On the prospect of crustacean genomics. Genomics. 2006, 88 (4): 415-430. 10.1016/j.ygeno.2006.03.007.PubMedView ArticleGoogle Scholar
- Gentleman R, Carey V, Bates D, Bolstad B, Dettlings M, Dudoit S, Ellis B, Gautier L, Ge Y, Gentry J, Hornik K, Hothorn T, Huber W, Iacus S, Irizarray R, Leisch F, Li C, Maechlers M, Rossini A, Sawitzki G, Smith C, Smyth G, Tierney L, Yang J, Zhang J: Bioconductor: open software development for computational biology and bioinformatics. Genome Biology. 2004, 5 (R80): R80-10.1186/gb-2004-5-10-r80.PubMed CentralPubMedView ArticleGoogle Scholar
- Futschick M, Crompton T: Model selection and efficiency testing for normalization of cDNA microarray data. Genome Biol. 2004, 5 (8): R60-10.1186/gb-2004-5-8-r60.View ArticleGoogle Scholar
- Kendziorski C, Newton M, Lan H, Gould M: On parametric empirical Bayes methods for comparing multiple groups using replicated gene expression profiles. Statistics in Medicene. 2003, 22: 3899-3914. 10.1002/sim.1548.View ArticleGoogle Scholar
This article is published under license to BioMed Central Ltd. This is an Open Access article distributed under the terms of the Creative Commons Attribution License (<url>http://creativecommons.org/licenses/by/2.0</url>), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.