- Research article
- Open Access
Enhancer of zeste plays an important role in photoperiodic modulation of locomotor rhythm in the cricket, Gryllus bimaculatus
Zoological Letters volume 2, Article number: 5 (2016)
Insects show daily behavioral rhythms controlled by an endogenous oscillator, the circadian clock. The rhythm synchronizes to daily light–dark cycles (LD) and changes waveform in association with seasonal change in photoperiod.
To explore the molecular basis of the photoperiod-dependent changes in circadian locomotor rhythm, we investigated the role of a chromatin modifier, Enhancer of zeste (Gb’E(z)), in the cricket, Gryllus bimaculatus. Under a 12 h:12 h LD (LD 12:12), Gb’E(z) was constitutively expressed in the optic lobe, the site of the biological clock; active phase (α) and rest phase (ρ) were approximately 12 h in duration, and α/ρ ratio was approximately 1.0. When transferred to LD 20:4, the α/ρ ratio decreased significantly, and the Gb’E(z) expression level was significantly reduced at 6 h and 10 h after light-on, as was reflected in the reduced level of trimethylation of histone H3 lysine 27. This change was associated with change in clock gene expression profiles. The photoperiod-dependent changes in α/ρ ratio and clock gene expression profiles were prevented by knocking down Gb’E(z) by RNAi.
These results suggest that histone modification by Gb’E(z) is involved in photoperiodic modulation of the G. bimaculatus circadian rhythm.
Most animals exhibit daily rhythms in various physiological functions that synchronize with daily environmental cycles, such as light–dark cycles (LD), which are affected by Earth’s rotation . The rhythm is generated by a circadian clock, which is an endogenous mechanism that oscillates over a period of approximately 24 h. The circadian clock’s oscillatory mechanism is based on transcriptional/translational molecular feedback loops [2–4]. In insects, the clock machinery has been studied most extensively in the fruit fly, Drosophila melanogaster, in which the major players are Clock (Clk) and cycle (cyc) [2, 3]; their product proteins, CLK and CYC, form heterodimers and activate the transcription of period (per) and timeless (tim) during the late day to early night. The translated proteins PER and TIM accumulate in the cytoplasm during the night, and in late night they heterodimerize and enter the nucleus to repress their own transcription by inhibiting CLK-CYC transcriptional activity. This feedback results in a reduction of PER and TIM levels, leading to the reactivation of per and tim transcription [2, 3].
Recent studies have revealed that circadian clock cycling is precisely controlled by mechanisms that include chromatin remodeling, recruitment of RNA polymerases, and post-transcriptional and post-translational modifications [5–8]. Chromatin remodeling plays an important role in regulating the circadian clock and in its response to environmental time cues. In both mammals and insects, CLK acts as a transcriptional activator and recruits other transcription factors by binding to E-boxes at the regulatory regions of clock-controlled genes, including per and tim [9–11].
In addition to daily time-keeping, the circadian clock plays a key role in seasonal changes in physiology, including the change in active phase to rest phase ratio (α/ρ ratio), based on seasonal change in photoperiod [12–14]. The photoperiod-dependent change in α/ρ ratio persists for many days in constant darkness and is recognized as a kind of history-dependent change in the circadian clock. History-dependent changes are also observed in the free-running period [15–17]. However, the molecular basis of photoperiod-dependent changes has remained elusive.
In the present study, we investigated the possible involvement of chromatin modification in photoperiod-dependent changes in circadian rhythm of the cricket, Gryllus bimaculatus. We used the cricket in this study for the following reasons: first, the cricket shows a clear photoperiodic response in locomotor activity rhythms [12, 14]; second, the circadian clock has been localized in the optic lobe [18, 19]; and third, cDNAs were previously obtained for major clock genes . Although number of chromatin modifiers so far known for insects including E(z), UTX, TRX, and Su(var)3-9 [21–24], we investigated the role of E(z) in photoperiodic modulation of the circadian rhythm, since its mammalian homolog EZH2 has been shown to be involved in control of the circadian clock mechanism through trimethylation of histone H3 lysine 27 (H3K27)  and we have some experimental evidence that RNA interference (RNAi) of E(z) effectively reduces H3K27 trimethylation (H3K27me3) level in our cricket . We found that knockdown of E(z) expression by RNAi prevented photoperiodic modulation. The results are discussed relative to the role of E(z) in photoperiodic modulation as well as seasonal adaptation of the circadian clock.
Materials and methods
Adult male crickets were purchased or taken from our laboratory colony, which is maintained under standard conditions of LD 12:12, at a constant temperature of 25 °C. The crickets were fed laboratory chow and water.
Measurement of mRNA levels
Quantitative real-time RT-PCR (qPCR) was used to measure mRNA levels. Total RNA was extracted from optic lobes of 4–6 adult males using ISOGEN (Nippon Gene, Japan) or TRIzol Reagent (Invitrogen, California). The total RNA was treated with DNase I to remove any traces of genomic DNA. Approximately 250 ng of total RNA of each sample was reverse transcribed with random 6mers using PrimeScript RT Reagent Kit (Takara, Japan). qPCR was performed with an Mx3000P Real-time PCR System (Stratagene, California) using Fast Start Universal SYBR Green Master (Roche, Japan) including SYBR Green with the following primers for respective genes: 5′-AAGGTGCGAAAACAGGCATC-3′ and 5′-TCGTCGTTTTGGTGGATGTG-3′ for Gb’E(z) (GenBank Accession No. LC012934), 5′-AAGCAAGCAAGCATCCTCAT-3′ and 5′-CTGAGAAAGGAGGCCACAAG-3′ for Gb’per (GenBank Accession No. AB375516), 5′-GATTATGAAGTCTGTGATGATTGG-3′ and 5′-AGCATTGGAGAGAACTGAA-GAGGT-3′ for Gb’tim (GenBank Accession No. AB548625), 5′-GGCCGAAGCTCATAAAGTGG-3′ and 5′-AACCGCACAAAGGAACCATC-3′ for Gb’cyc (GenBank Accession No. AB762416), 5′-AATGACCGTAGTCGAGAAAGTGAAG-3′ and 5′-TTGCGATGATTGAGGTTGTTG-3′ for Gb’Clk (GenBank Accession No. AB738083), and 5′-GCTCCGGATTACATCGTTGC-3′ and 5′-GCCAAATGCCGAAGTTCTTG-3′ for Gb’rpl18a (GenBank Accession No. DC448653). Standard curves for the transcripts were generated by serial dilutions of amplified cDNAs and included in each qPCR run. After 40 PCR cycles, samples were subjected to melting curve analysis, and a single expected amplicon was confirmed in each sample. The results were analyzed using software associated with the instrument: quantification of mRNA levels was performed by the standard curve method, and the values were normalized to the values of rpl18a at each time point.
Double-stranded RNAs (dsRNAs) were synthesized using the MEGAScript T7 Kit (Ambion, California) and adjusted to 20 μM for DsRed2 and 2 μM for Gb’E(z) for RNAi. For dsRNA synthesis, we used the T7 primer, 5′-TAATACGACTCACTATAGGG-3′, for Gb’E(z) and an exogenous gene, DsRed2; dsRNA lengths were 431 bp and 660 bp, respectively. In total, 700 nL of dsRNA was injected into the abdomens of the adult male crickets. As a negative control, we injected dsRNA for DsRed2.
Heads of adult males were fixed at zeitgeber time (ZT) 10 (ZT 0 corresponds to lights-on) with 2 % paraformaldehyde (PFA) in phosphate-buffered saline with 0.1 % Tween 20 (PBT) for 17 h at 4 °C. The brain and optic lobe complex was extracted using a fine razor knife, tweezers, and micro scissors under dissecting microscope, then fat bodies and associated nerves were removed. The tissues were refixed in 4 % PFA/PBT and dehydrated in 25 %, 50 %, 75 % EtOH/PBT and 100 % EtOH. Dehydrated samples were rehydrated in 75 %, 50 %, and 25 % EtOH/PBT, washed with PBT, and blocked with 1 % normal goat serum (NGS) in PBT for 1 h. Blocked samples were incubated overnight at 4 °C with rabbit polyclonal anti-trimethylated H3K27 antibody (EMD Millipore, Germany; 1:500 diluted in 1 % NGS in PBT). The samples were then washed with PBT and incubated for 3 h with secondary anti-rabbit IgG antibody conjugated with Alexa Fluor 488 (Molecular Probes, Massachusetts; 1:500 diluted in 1 % NGS/PBT). Samples were washed with PBT and incubated with DAPI at 1:1000 in PBT for 15 min. The samples were mounted on a glass slide with 50 % glycerol/PBT, observed and optical digital images were captured with a confocal laser scanning microscope (LSM-780, Zeiss, Germany).
To quantify the staining intensity of H3K27me3 and DAPI, the fluorescence intensities were quantified from digital images of six optic lobes for each treatment using the ImageJ software (freely available at http://rsb.info.nih.gov/ij/). The H3K27me3 staining indices were shown as the ratio of staining intensity of H3K27me3 to that of DAPI.
Recording of locomotor activity
Locomotor activity of individual animals was recorded with an actograph made of a transparent plastic box (18 × 9 × 4.5 cm) with a rocking substratum, as previously described . A magnetic reed switch sensed rocking movements of the substratum caused by a moving cricket. The number of movements was recorded every 6 min by a computerized system. Water and food were provided ad libitum. The activity chambers were placed in an incubator in which temperature was kept at 25 ± 0.5 °C and desired lighting regimens were provided by a cool white fluorescent lamp connected to an electric timer. The light intensity was 600–1000 lux, which varied based on the animal’s proximity to the lamp.
The raw data were displayed as conventional double-plotted actograms to judge activity patterns, and free-running periods were calculated using the χ 2 periodogram  in ActogramJ . If a peak of the periodogram was above the 5 % confidence threshold, the peak period was designated as statistically significant. The duration of the active phase, or subjective night, (α) was estimated with ActogramJ: the boundary of the active phase was defined at the time point where the moving average of activity exceeded or fell below 70 % of daily average activity; then, a linear regression line was fitted to the points for consecutive days. The rest of the time was designated as the rest phase, or subjective day, (ρ).
The one-way analysis of variance (ANOVA) followed by a post hoc Tukey-test was used to compare the differences in means of free-running periods, α/ρ ratios, and immunostaining intensity of H3K27me3 between the control and experimental groups. Significance of daily cycling of clock gene mRNA levels and difference of mRNA levels among three groups of crickets treated in different ways were tested by ANOVA followed by Tukey-test. To compare the means of two groups, t-test was used. In all statistical tests, the significance level was set at P < 0.05.
Expression profile of Gb’E(z) in the optic lobe and its suppression by RNAi
We first examined whether Gb’E(z) was expressed in the optic lobe, which is known to harbor the circadian clock in the cricket, by using qPCR to measure Gb’E(z) mRNA levels in the tissue. Under LD 12:12 Gb’E(z) mRNA was fairly consistently expressed throughout a day in intact crickets (Fig. 1a), and no daily fluctuation was observed (ANOVA, F5, 41 = 0.34, P > 0.88).
To estimate the effects of Gb’E(z)RNAi, we measured Gb’E(z) levels in the optic lobe of Gb’E(z)RNAi crickets and control (DsRed2 RNAi) crickets, which were treated with dsDsRed2. DsRed2 RNAi crickets showed similar Gb’E(z) expression to that of intact crickets (Fig. 1a) and no daily rhythm was observed (ANOVA, F5, 37 = 0.52, P > 0.76). The value at each time point did not differ from that of intact crickets (Tukey-test, P > 0.05). In Gb’E(z)RNAi crickets, Gb’E(z) expression was greatly reduced compared with the control and intact crickets at all time points (Tukey-test, P < 0.01). Expression reduced to approximately 53 % of that of intact and control crickets at ZT 10. These results indicate that Gb’E(z) is expressed rather constitutively in the optic lobe and could be knocked down by RNAi against Gb’E(z), and that DsRed2 RNAi crickets can be used as a control.
Expression profile of clock genes in the optic lobe under LD 12:12
Expression profiles of the clock genes Gb’per, Gb’tim, and Gb’cyc were investigated in the optic lobe of DsRed2 RNAi and Gb’E(z)RNAi crickets under LD 12:12 by qPCR. The results are shown in Fig. 1b–d. In the control crickets, the mRNA levels of Gb’per and Gb’tim showed a significant daily fluctuation, which peaked at ZT 18 under LD 12:12 (ANOVA: F5, 36 = 9.01, P < 0.01 for Gb’per, F5, 17 = 67.97, P < 0.01 for Gb’tim) (Fig. 1b, c). Gb’cyc also showed a significant daily cycling, with a peak at ZT 10 (ANOVA: F5, 41 = 3.62, P < 0.01) (Fig. 1d). Similar rhythmic expression profiles were observed for the three genes in Gb’E(z)RNAi crickets (ANOVA: F5, 20 = 15.47, P < 0.01 for Gb’per; F5, 17 = 24.25, P < 0.01 for Gb’tim; F5, 22 = 4.45, P < 0.01 for Gb’cyc), but with slight changes in pattern or phase compared with those in DsRed2 RNAi crickets (Fig. 1b-d): Gb’per showed a significant reduction at ZT 6 and ZT 10 (t-test, P < 0.01), and Gb’tim showed a slight increase at ZT 2, a slight reduction at ZT 10 (t-test, P < 0.05), and a reduction at ZT 18 (t-test, P < 0.01) that resulted in a phase advance of the peak by 4 h. Moreover, Gb’cyc showed a significant increase at ZT 2 (t-test, P < 0.05).
Effects of Gb’E(z)RNAi on circadian locomotor rhythms in LD 12:12 and ensuing DD
To examine the role of Gb’E(z) in regulation of circadian rhythms, we recorded the locomotor activity in Gb’E(z)RNAi, intact and control crickets. Both intact and control crickets showed nocturnal activity rhythms that peaked just after lights-off under LD 12:12, and the rhythm persisted with a free-running period slightly shorter than 24 h in constant darkness (DD) (Fig. 2a, b, Table 1). We measured the duration of active phase (α) and rest phase (ρ), and calculated α/ρ ratio to characterize the daily activity profile. The α/ρ ratios of intact and control crickets were approximately 1.0 both in LD 12:12 and DD (Table 1). These results were consistent with those of our previous study . The Gb’E(z)RNAi crickets showed nocturnal locomotor rhythms similar to those of control crickets under LD 12:12 (Fig. 2c); their α/ρ ratios were approximately 1.0 both in LD 12:12 and DD (Table 1), and were not significantly different from those of the intact and control crickets (ANOVA followed by Tukey-test, P > 0.05). However, their average free-running period was significantly longer than that of intact and control crickets (ANOVA followed by Tukey-test, P < 0.01, Table 1), which suggests that methylation of H3K27 is involved in regulating the free-running period in DD.
Role of Gb’E(z) in photoperiodic modulation of locomotor rhythms
In the cricket, the α/ρ ratio in DD has been shown to change depending on the preceding photoperiodic conditions . We used LD 20:4 to examine the photoperiodic modulation of the rhythm because it has been shown to reduce the α/ρ ratio most effectively . To examine the effects of Gb’E(z)RNAi on this photoperiodic effect on the α/ρ ratio, we recorded locomotor activity rhythm of intact, DsRed2 RNAi, and Gb’E(z)RNAi crickets under LD 12:12, followed by LD 20:4 for 9 cycles, and then by DD. The representative records are shown in Fig. 3, and the locomotor rhythm parameters are summarized in Table 1. The intact and control crickets showed that locomotor activity was confined to a short dark phase under LD 20:4, and the shortened active phase persisted under subsequent free-running conditions (Fig. 3a, b).
The α/ρ ratios of intact and DsRed2 RNAi crickets under LD 20:4 and the ensuing DD were both significantly smaller than those in LD 12:12 and the ensuing DD (Table 1). There was no significant difference in the α/ρ ratio between intact and DsRed2 RNAi crickets under DD (ANOVA followed by Tukey-test, P > 0.05). These results are consistent with those of Koga et al. . Under LD 20:4 some Gb’E(z)RNAi crickets (6/23) showed similar changes in α/ρ ratio (Fig. 3c). However, the remaining crickets (17/23) exhibited an activity pattern that consisted of a strong activity bout after lights-on in addition to the light-off peak under LD 20:4; the average α/ρ ratio was 0.84 ± 0.28 (n = 23) (Table 1). Interestingly, the α/ρ ratio was maintained in the ensuing DD, and was significantly greater than those of the intact and control crickets (ANOVA followed by Tukey-test, P < 0.01, Table 1). The free-running period of the Gb’E(z)RNAi crickets was again significantly longer than that of the control crickets (Tukey-test, P < 0.01). These results suggest that Gb’E(z) is involved in photoperiodic modulation and regulation of free-running period in the circadian locomotor rhythm.
Involvement of Gb’E(z) in photoperiodic modulation of clock gene expression profiles
Because Gb’E(z) is the chromatin modifier that controls gene expression through H3K27 methylation, we predicted that Gb’E(z) is involved in photoperiodic modulation of α/ρ ratio through alteration in clock gene expression. Consequently, we examined whether endogenous Gb’E(z) mRNA levels in the optic lobe altered with a change of photoperiodic condition (Fig. 4a). In the control crickets, Gb’E(z) showed no significant daily change in its expression, but a significant reduction was found at ZT 6 and ZT 10 in LD 20:4 when compared with that in LD 12:12 (Tukey-test, P < 0.01). Gb’E(z)RNAi highly reduced Gb’E(z) levels compared with the control at all the points in LD 20:4 (Tukey-test, P < 0.01). The reduced levels were significantly less at ZT 2–10 and ZT 18 than those with same treatment under LD 12:12 (Tukey-test, P < 0.01 for ZT 2–10 and P < 0.05 for ZT 18). These results indicate that Gb’E(z) expression level is affected by photoperiod and may be involved in photoperiodic modulation of locomotor rhythm.
We then examined the expression profiles of the clock genes Gb’per, Gb’tim, and Gb’cyc in the optic lobe in the control and Gb’E(z)RNAi crickets in LD 20:4 by qPCR (Fig. 4b–d). In the control crickets, Gb’per and Gb’cyc mRNA levels showed significant daily fluctuation (ANOVA: F5, 26 = 3.97, P < 0.01 for Gb’per; F5, 27 = 3.48, P < 0.05 for Gb’cyc). The peak phase occurred during the late day phase (ZT 14), which indicates that Gb’per and Gb’cyc oscillations advanced and delayed by approximately 4 h, respectively, compared with those in the preceding LD 12:12 (Fig. 4b, d). Gb’tim mRNA levels also showed significant daily cycling, with a peak at ZT 18 (ANOVA: F5, 26 = 17.50, P < 0.01), retaining the phase relationship to the lights-on similar to that was seen in LD 12:12 (Fig. 4c). In Gb’E(z)RNAi crickets, mRNA levels of the three clock genes showed significant daily fluctuation (ANOVA: F5, 27 = 12.09, P < 0.01 for Gb’per; F5, 18 = 37.93, P < 0.01 for Gb’tim; F5, 38 = 7.58, P < 0.01 for Gb’cyc). Gb’tim showed a phase relationship with LD 20:4 similar to that in the control crickets, but the mRNA levels were significantly reduced (t-test, P < 0.01). Interestingly, the peak phase of Gb’per and Gb’cyc was delayed and advanced by approximately 8 and 4 h, respectively, relative to control crickets (Fig. 4b, d). These results suggest that expression profiles of Gb’per and Gb’cyc were altered by photoperiod and that this alteration was mediated at least in part by Gb’E(z).
Methylation levels of histone H3K27
Since expression levels of Gb’E(z) were lower in LD 20:4 than in LD 12:12, we examined the level of histone H3 methylated at K27 at ZT 10 in the two photoperiodic conditions by immunohistochemistry using anti-H3K27me3 antibody. In both conditions, many nuclei were labeled by the antibody showing trimethylation of H3K27, being distributed over whole optic lobe (Fig. 5a, b). The expression levels in the optic lobe were significantly higher in LD 12:12 than in LD 20:4 (Fig. 5c). In the crickets treated with Gb’E(z)RNAi, the levels of H3K27me3 in the optic lobe were significantly reduced both in LD 12:12 and LD 20:4 (Fig. 5). These results suggest that Gb’E(z) contributes to the modulation of histone H3K27me3 levels in the optic lobe. However, no significant difference was found between Gb’E(z)RNAi crickets of the two photoperiodic conditions (Fig. 5c), although the Gb’E(z) mRNA levels significantly differed (Fig. 4a). This may be explained that the Gb’E(z) protein levels were so reduced in both cases that no significant difference was detected in H3K27me3 levels.
Using an RNAi knockdown approach, we showed that the chromatin modifier Gb’E(z) is involved in regulating the free-running period and photoperiodic modulation of the locomotor rhythm in the cricket, G. bimaculatus.
Gb’E(z) expression in the optic lobe
Our qPCR analysis revealed that the chromatin modifier Gb’E(z) is constitutively expressed in the optic lobe, which is the location of the cricket’s circadian clock , which recalls the fact that most of the chromatin modifiers involved in circadian gene expression are present on a constitutive basis and recruited as needed to regulate transcription . In mammals, for example, CLOCK plays a key role in the event and forms a transcriptional complex with BMAL1 to activate Per and Cry transcription by binding to the E-box in their upstream region . Meanwhile, CLOCK acts as a factor that opens up chromatin, which enables other transcriptional factors to act on target genes of CLOCK . Similar molecular events may occur in transcription of per and tim in Drosophila, as CLK-CYC binding to upstream and/or intronic E-boxes of per and tim controls chromatin modifications through H3K9 acetylation and H3K4 trimethylation .
Interestingly, however, Gb’E(z) mRNA levels at ZT 6 and ZT 10 were higher in LD 12:12 than LD 20:4 (Fig. 4a) and the difference was reflected in the trimethylation levels of H3K27 (Fig. 5). To our knowledge, this is the first evidence for photoperiodic regulation of a clock-related chromatin modifier in insects. Light-induced modification of chromatin is known for H3S10 in the mammalian circadian clock in the suprachiasmatic nucleus ; it is a result of phosphorylation and occurs within 5 min after lights-on, which is similar to c-fos induction. Gb’E(z) seems to be regulated by a different mechanism than immediate induction of phosphorylation, because no apparent change was observed at lights-on in Gb’E(z) mRNA levels (Figs. 1a and 4a). KISMET, a chromatin-remodeling enzyme, represents a candidate regulator for this photoperiodic regulation of Gb’E(z), as it is required for normal circadian light responses in Drosophila . Gb’E(z) was also shown to be induced by mechanical stimulation; when a leg was injured, the onset of regeneration was associated with upregulation of Gb’E(z) [24, 32]. Thus, its expression seems to be regulated by multiple pathways.
Gb’E(z) may be involved in photoperiodic modulation of the circadian rhythm
Involvement of chromatin modifiers in regulating the circadian clock has been shown in animals. In Drosophila, Brahma chromatin-remodeling protein regulates CLK binding to target promoters, and hence the free-running period of the rhythm . Mice that lacked Mettle3, a factor that regulates RNA methylation, showed a delay in RNA processing that leads to circadian period elongation . However, our results revealed that Gb’E(z) plays a different role from those previously described regulatory models. Gb’E(z) knockdown significantly lengthened the free-running period in DD after LD 12:12 and LD 20:4 (Table 1). Another important effect of Gb’E(z)RNAi was elimination of the photoperiod-dependent change in α/ρ ratio. In control crickets, the active phase was usually compressed during the dark phase in LD 20:4; consequently, the α/ρ ratio became much smaller (0.69 ± 0.22) than that in LD 12:12 (0.97 ± 0.09) (Table 1). The α/ρ ratio further decreased when transferred to DD (0.55 ± 0.19) (Table 1). These results are consistent with our previous results . However, compression of the active phase was only observed in a few Gb’E(z)RNAi crickets, and the majority of them showed no compression; the average α/ρ ratio was 0.84 ± 0.28 and 0.83 ± 0.25 in LD 20:4 and in the ensuing DD, respectively (Table 1). These results strongly suggest that regulation by E(z) is required in the response to a changing photoperiod through modulating the duration of the active phase. The link between regulatory mechanisms and circadian waveform or free-running period should be investigated in future studies.
Gb’E(z) may contribute to response to photoperiodic changes via clock genes
This study revealed that temporal expression profiles of clock genes change in response to LD cycle. Under a long-day condition of LD 20:4, the circadian expression profile of the clock gene Gb’tim showed a similar pattern to that in LD 12:12, whereas Gb’per and Gb’cyc expression was advanced and delayed by 4 h, respectively (Fig. 4). Gb’E(z)RNAi prevented the shift of Gb’per and Gb’cyc rhythms in response to LD 20:4 (Fig. 4), which suggests the involvement of Gb’E(z) in photoperiod-dependent phase setting of daily clock gene expression. This function of Gb’E(z) may be mediated by trimethylation of histone H3K27 because H3K27me3 levels are dependent on Gb’E(z) mRNA levels (Fig. 5) and H3K27me3 is known to regulate expression of Per1 and Per2 in the mammalian circadian clock . In the mammalian clock, EZH2, a homologous protein of E(z), is recruited by the CLOCK/BMAL1 complex to bind to H3 in the promoter regions of Per1 and Per2 and causes di- and trimethylation of H3K27 . The phase shift of Gb’cyc cycling caused by Gb’E(z)RNAi might be attributable to indirect effects through the change of Gb’per rhythm, because Gb’per is involved in the transcriptional regulation of Gb’cyc .
The photoperiodic regulation of daily clock gene expression may be caused by a change in Gb’E(z) mRNA levels (Fig. 4a). Because no daily rhythm is known in binding ability of EZH2 to CLOCK: BMAL1 and H3 at the promoter regions of Per1 and Per2 , quantity of E(z) may affect the binding and eventually daily expression profiles of the clock genes. The change in Gb’E(z) levels may not be a simple response to a given photoperiod, because the α/ρ ratio established in a photoperiod is maintained for a long period in DD . The mechanism of this long-lasting change is an important issue that should be addressed in future studies.
The long-lasting response to photoperiod is reminiscent of photoperiodism regulating the seasonal physiological adaptation in insects. Many cricket species also show photoperiodic responses . For example, nymphal development of Modicogryllus siamensis is photoperiodically regulated; nymphs grow faster under long-day conditions and become adults after seven moltings, whereas under short-day conditions, the nymphal period is elongated and the number of molts to adulthood increases . Interestingly, developmental time course is determined within about 10 days after hatching , which indicates a long-lasting effect of photoperiod. This is consistent with the finding in this study suggesting that the long-lasting change in the clock is caused by an epigenetic mechanism, and photoperiodic response is most likely underlain by the circadian clock [37, 38]. In addition to the histone modification, we also have to consider the role of DNA methylation, because a recent study showed that maternal transfer of photoperiodic information to offspring is attributable to DNA methylation in Nasonia vitripennis .
The means by which changes in molecular oscillation are reflected in overt activity rhythms are still being elucidated. There are lines of evidence that molecular oscillation of the circadian clock changes in a photoperiod-dependent manner. In Drosophila, daily per expression, i.e., phase and ratio of splicing variants, changes in response to photoperiod [40–42]. In other insects, the expression profiles of clock genes also reportedly changed based on photoperiod [43, 44]. In the present study, we showed that Gb’per and Gb’cyc responded differently so that the peak phases of their daily expression rhythms became closer in the long photoperiod (Fig. 4). Although additional studies are necessary, this phase change might be somehow related to the shortening of the active phase under long-day conditions.
The present study discovered for the first time that methylation on H3K27 by Gb’E(z) is required for photoperiodic modulation of the circadian locomotor rhythm, such as length of the active phase and free-running period, which is associated with changes in expression profiles of clock component genes. These results contribute to molecular dissection of the mechanisms of insect photoperiodism and photoperiodic modulation in circadian rhythms.
Dunlap JC, Loros J, DeCoursey PJ. Chronobiology: biological timekeeping. Sinauer: Sunderland; 2004.
Tataroglu O, Emery P. The molecular ticks of the Drosophila circadian clock. Curr Opin Insect Sci. 2015;7:51–7.
Hardin P. Molecular mechanisms of circadian timekeeping in Drosophila. Sleep Biol Rhythms. 2009;7:235–42.
Aguilar Roblero R, Díaz-Muñoz M, Fanjul-Moles ML. Mechanisms of circadian systems in animals and their clinical relevance. Heidelberg: New York, Dordrecht, London, Springer; 2015.
Ripperger JA, Merrow M. Perfect timing: epigenetic regulation of the circadian clock. FEBS Lett. 2011;585:1406–11.
Bellet MM, Sassone-Corsi P. Mammalian circadian clock and metabolism-the epigenetic link. J Cell Sci. 2010;123:3837–48.
Aguilar-Arnal L, Sassone-Corsi P. Chromatin landscape and circadian dynamics: spatial and temporal organization of clock transcription. Proc Natl Acad Sci U S A. 2015;112:6863–70.
Kwok RS, Li YH, Lei AJ, Edery I, Chiu JC. The catalytic and non-catalytic functions of the Brahma chromatin-remodeling protein collatorate to fine-tune circadian transcription in Drosophila. PLoS Genet. 2015;11:e1005307.
Doi M, Hirayama J, Sassone-Corsi P. Circadian regulator CLOCK is a histone acetyltransferase. Cell. 2006;125:497–508.
Taylor P, Hardin P. Rhythmic E-box binding by CLK-CYC controls daily cycles in per and tim transcription and chromatin modifications. Mol Cell Biol. 2008;28:4642–52.
Menet JS, Pescatore S, Rosbash M. CLOCK: BMAL1 is a pioneer-like transcrption factor. Genes Dev. 2014;28:8–13.
Tomioka K, Chiba Y. Photoperiod during post-embryonic development affects some parameters of adult circadian rhythm in the cricket, Gryllus bimaculatus. Zool Sci. 1989;6:565–71.
Tomioka K, Chiba Y. Light cycle during post-embryonic development affects adult circadian parameters of the cricket (Gryllus bimaculatus) optic lobe pacemaker. J Insect Physiol. 1989;35:273–6.
Koga M, Ushirogawa H, Tomioka K. Photoperiodic modulation of circadian rhythms in the cricket Gryllus bimaculatus. J Insect Physiol. 2005;51:681–90.
Page TL. Transplantation of the cockroach circadian pacemaker. Science. 1982;216:73–5.
Page TL. Effects of optic tract regeneration on internal coupling in the circadian system of the cockroach. J Comp Physiol A. 1983;153:231–40.
Barrett RK, Page TL. Effects of light on circadian pacemaker development. I. The freerunning period. J Comp Physiol A. 1989;165:41–9.
Tomioka K, Chiba Y. Effects of nymphal stage optic nerve severance or optic lobe removal on the circadian locomotor rhythm of the cricket, Gryllus bimaculatus. Zool Sci. 1984;1:385–94.
Tomioka K, Chiba Y. Characterization of optic lobe circadian pacemaker by in situ and in vitro recording of neuronal activity in the cricket Gryllus bimaculatus. J Comp Physiol A. 1992;171:1–7.
Tomioka K. Chronobiology of crickets: a review. Zool Sci. 2014;31:624–32.
Krauss V, Fassl A, Fiebig P, Patties I, Sass H. The evolution of the histone methyltransferase gene Su (var) 3-9 in metazoans includes a fusion with and a re-fission from a functionally unrelated gene. BMC Evol Biol. 2006;6:18.
Tie F, Banerjee R, Stratton CA, Prasad-Sinha J, Stepanik V, Zlobin A, et al. CBP-mediated acetylation of histone H3 lysine 27 antagonizes Drosophila Polycomb silencing. Development. 2009;136:3131–41.
Smith ER, Lee MG, Winter B, Droz NM, Eissenberg JC, Shiekhattar R, et al. Drosophila UTX is a histone H3 Lys27 demethylase that colocalizes with the elongating form of RNA polymerase II. Mol Cell Biol. 2008;28:1041–6.
Hamada Y, Bando T, Namamura T, Ishimaru Y, Mito T, Noji S, et al. Leg regeneration is epigenetically regulated by histone H3K27 methylation in the cricket Gryllus bimaculatus. Development. 2015;142:2916–27.
Etchegaray JP, Yang X, DeBruyne JP, Peters AH, Weaver DR, Jenuwein T, et al. The polycomb group protein EZH2 is required for mammalian circadian clock function. J Biol Chem. 2006;281:21209–15.
Moriyama Y, Sakamoto T, Karpova SG, Matsumoto A, Noji S, Tomioka K. RNA interference of the clock gene period disrupts circadian rhythms in the cricket Gryllus bimaculatus. J Biol Rhythms. 2008;23:308–18.
Sokolove PG, Bushell WN. The chi square periodogram: its utility for analysis of circadian rhythm. J Theor Biol. 1978;72:131–60.
Schmid B, Helfrich-Förster C, Yoshii T. A new ImageJ plug-in “ActogramJ” for chronobiological analyses. J Biol Rhythms. 2011;26:464–7.
Stanewsky R. Genetic analysis of the circadian system in Drosophila melanogaster and mammals. J Neurobiol. 2003;54:111–47.
Crosio C, Cermakian N, Allis CD, Sassone-Corsi P. Light induces chromatin modification in cells of the mammalian circadian clock. Nat Neurosci. 2000;3:1241–7.
Dubruille R, Murad A, Rosbash M, Emery P. A constant light-genetic screen identifies KISMET as a regulator of circadian photoresponses. PLoS Genet. 2009;5, e1000787.
Bando T, Ishimaru Y, Kida T, Hamada Y, Matsuoka Y, Nakamura T, et al. Analysis of RNA-seq data reveals involvement of JAK/STAT signalling during leg regeneration in the cricket Gryllus bimaculatus. Development. 2013;140:959–64.
Fustin JM, Doi M, Yamaguchi Y, Hida H, Nishimura S, Yoshida M, et al. RNA-methylation-dependent RNA processing controls the speed of the circadian clock. Cell Tiss Res. 2013;155:793–806.
Uryu O, Karpova SG, Tomioka K. The clock gene cycle plays an important role in the circadian clock of the cricket Gryllus bimaculatus. J Insect Physiol. 2013;59:697–704.
Tauber TJ, Tauber CA, Masaki S. Seasonal Adaptations of Insects. New York: Oxford University Press; 1986.
Taniguchi N, Tomioka K. Duration of development and number of nymphal instars are differentially regulated by photoperiod in the cricket Modicogryllus siamensis (Orthoptera: Gryllidae). Eur J Entomol. 2003;100:275–81.
Saunders DS. Insect photoperiodism: seeing the light. Physiol Entomol. 2012;37:207–18.
Goto SG. Roles of circadian clock genes in insect photoperiodism. Entomol Sci. 2013;16:1–16.
Pegoraro M, Bafna A, Davies NJ, Shuker DM, Tauber E. DNA methylation changes induced by long and short photoperiods in Nasonia. Genome Res. 2016;26:203–10.
Majercak J, Sidote D, Hardin PE, Edery I. How a circadian clock adapts to seasonal decreases in temperature and day length. Neuron. 1999;24:219–30.
Majercak J, Chen W-F, Edery I. Splicing of the period gene 3′-terminal intron is regulated by light, circadian clock factors, and phospholipase C. Mol Cell Biol. 2004;24:3359–72.
Collins BH, Rosato E, Kyriacou CP. Seasonal behavior in Drosophila melanogaster requires the photoreceptors, the circadian clock, and phospholipase C. Proc Natl Acad Sci U S A. 2004;101:1945–50.
Syrova Z, Dolezel D, Saumann I, Hodkova M. Photoperiodic regulation of diapause in linden bugs: are period and Clock genes involved? Cell Mol Life Sci. 2003;60:2510–5.
Sakamoto T, Uryu O, Tomioka K. The clock gene period plays an essential role in photoperiodic control of nymphal development in the cricket Modicogryllus siamensis. J Biol Rhythms. 2009;24:379–90.
This work was supported in part by grants from JSPS [#14 J04731 to H.Y., #15 K06897 to B.T. and #15H04400 to K.T.]. H.Y. is a JSPS research fellow.
The authors declare they have no competing interests.
YH and AT performed the experiments and YH and KT wrote the paper. KT and YH designed the experiments. TB and HO supported molecular analysis of Gb’E(z). YH, KT, TB and HO critically read the manuscript. All authors read and approved the final manuscript.
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Hamada, Y., Tokuoka, A., Bando, T. et al. Enhancer of zeste plays an important role in photoperiodic modulation of locomotor rhythm in the cricket, Gryllus bimaculatus . Zoological Lett 2, 5 (2016) doi:10.1186/s40851-016-0042-7
- Circadian rhythm
- Photoperiodic modulation
- Histone modification
- Clock gene
- Enhancer of zeste