Transcription factors bind low-affinity DNA sequences for only short durations. It is not clear how brief, low-affinity interactions can drive efficient transcription. Here, we report that the transcription factor Ultrabithorax (Ubx) utilizes low-affinity binding sites in the Drosophila melanogaster shavenbaby (svb) locus and related enhancers in nuclear microenvironments of high Ubx concentrations. Related enhancers colocalize to the same microenvironments independently of their chromosomal location, suggesting that microenvironments are highly differentiated transcription domains. Manipulating the affinity of svb enhancers revealed an inverse relationship between enhancer affinity and Ubx concentration required for transcriptional activation. The Ubx cofactor, Homothorax (Hth), was co-enriched with Ubx near enhancers that require Hth, even though Ubx and Hth did not co-localize throughout the nucleus. Thus, microenvironments of high local transcription factor and cofactor concentrations could help low-affinity sites overcome their kinetic inefficiency. Mechanisms that generate these microenvironments could be a general feature of eukaryotic transcriptional regulation.https://doi.org/10.7554/eLife.28975.001
Genomic regions near coding genes, called enhancers, direct specific patterns of gene expression (Spitz and Furlong, 2012; Reiter et al., 2017; Long et al., 2016). Enhancers contain short DNA sequences that bind sequence-specific activating and repressive transcription factor proteins, and the integration of these positive and negative signals directs gene expression (Crocker et al., 2016a). Protein-DNA binding is often an ephemeral event; studies in mammalian cells demonstrate that transcription factors disassociate within seconds of binding to DNA (Liu et al., 2014; Chen et al., 2014; Izeddin et al., 2014; Voss et al., 2011; Normanno et al., 2015; Morisaki et al., 2014). Furthermore, recent studies in animals ranging from fruit flies to mammals have revealed that low-affinity DNA-binding sites are critical to confer specificity between related transcription factors having binding sites with similar DNA sequences (Crocker et al., 2015; Farley et al., 2015; Farley et al., 2016; Lorberbaum et al., 2016; Antosova et al., 2016; Rister et al., 2015; Crocker et al., 2010; Crocker et al., 2016b; Tanay, 2006; Lebrecht et al., 2005; Rowan et al., 2010; Gaudet and Mango, 2002; Jiang and Levine, 1993). Increasing the affinity of binding sites to more stably recruit transcription factors activates promiscuous gene expression (Farley et al., 2015; Ramos and Barolo, 2013), which leads to developmental defects. It is unclear how brief protein-DNA contacts can mediate efficient transcription from enhancers containing low-affinity binding sites.
One possible mechanism that could mitigate their kinetic inefficiency is to increase the local concentrations of transcription factors. At the scale of a single enhancer over a few hundred base pairs long, multiple low-affinity binding sites for the same transcription factor in close proximity could increase the frequency of binding events by trapping the protein. Furthermore, interactions between transcription factors and cofactors with multiple binding sites within an enhancer could generate ‘microenvironments’ (Reiter et al., 2017) of high factor concentrations.
We have explored this problem using the shavenbaby (svb) locus, which contains multiple enhancers that drive specific patterns of svb gene expression in developing Drosophila embryos. Each of three characterized svb enhancers contains clusters of low-affinity binding sites for the Hox gene Ultrabithorax (Ubx). These enhancers also require a Ubx cofactor Homothorax (Hth) to function (Crocker et al., 2015). We have exploited robust transgenic tools in Drosophila, new fluorescent dyes, and new approaches to prepare embryos for microscopy to systematically perturb these svb enhancers and directly image the results at a sub-nuclear level. We find that microenvironments of high Ubx and Hth concentrations mediate transcription from low-affinity enhancers.
We first examined whether nuclei in Drosophila melanogaster embryos possess Ubx microenvironments by performing immunofluorescence (IF) staining in fixed embryos and high-resolution confocal imaging using Airyscan (Carl Zeiss Microscopy, Jena, Germany). We found that Ubx protein was not distributed uniformly, but rather exhibited regions of high and low Ubx intensities (Figure 1A,B). To observe Ubx distribution at higher resolution, we expanded the size of the embryos (Tillberg et al., 2016) by approximately four-fold in each dimension (Figure 1C). Nuclei of expanded embryos revealed distinct regions of high Ubx intensity separated by regions of low Ubx intensity. We observed, on average, 185 ± 25 (n = 12, three embryos) clusters per nucleus that were stronger than one-quarter of the maximum Ubx intensity within that nucleus (Figure 1D,E, and Figure 1—figure supplement 1).
One explanation for the observed distribution of Ubx is that transcription factors localize generally to accessible regions of the nucleus that have high levels of transcriptional activity. This mechanism, if shared by transcription factors in general, should yield Ubx distributions that mostly overlap with that of other transcription factors. Engrailed (En), a transcription factor unrelated to Ubx, displayed non-uniform sub-nuclear concentrations, but its distribution only partially overlapped with that of Ubx (Figure 1—figure supplement 2A–C, white regions indicate overlap). We similarly observed only partial overlap between Ubx and Even-skipped (Eve) (Figure 1—figure supplement 2D–F). Abdominal-A (AdbA), a paralog of Ubx that is expressed mainly in separate cells from Ubx and that has similar DNA-binding specificity as Ubx, was excluded from Ubx regions in the few nuclei where both were expressed (Figure 1—figure supplement 2G–I). These results indicate that the distributions of these transcription factors do not result from a shared mechanism that limits the distribution of all transcription factors to the same sub-nuclear regions.
We also examined whether Ubx simply occupies regions containing actively transcribed DNA. Both active RNA Polymerase II (Pol II, Ser5 phosphorylated CTD) and the methylated histone H3K4me3, which marks actively transcribed DNA, only partially overlapped with Ubx (Figure 1—figure supplement 3A–F). In contrast, the histone mark H3K27me3, which marks regions of repressed chromatin, displayed almost no overlap with the distribution of Ubx (Figure 1—figure supplement 3G–I). Thus, Ubx is not merely restricted to regions inside the nucleus that are available to transcription factors or to regions of high transcriptional activity.
To understand if the heterogeneous distribution of Ubx is dynamic or stable over the timescale of seconds to minutes, as well as to rule out the possibility that our observations of Ubx microenvironments are an artifact of the fixation protocol (Teves et al., 2016), we examined the spatiotemporal dynamics of single Ubx molecules in live Drosophila embryos. Single-molecule imaging has been mostly performed in cell lines previously because live-imaging studies of transcription factor dynamics in embryos requires overcoming several new challenges, including imaging at lower signal-to-noise ratios, compensating for rapid morphological changes during embryonic development, and determining how to deliver fluorescent dyes. We overcame these challenges by generating a HaloTag-Ubx transgene that allowed precise control of fusion protein levels (Figure 1—figure supplement 4A) and coupling HaloTag-Ubx in vivo to new, strongly fluorescent dyes (Grimm et al., 2017). The transgene we built can be expressed either from a heat-shock promoter (hsp70) or from a 20x UAS promoter by crossing with a GAL4 driver line.
Over-expression of the HaloTag-Ubx transgene by incubating the embryos at 30°C transformed anterior segments to the fate of more posterior segments, indicated by the presence of additional trichomes. This result indicates that the HaloTag-Ubx protein retains the expected Ubx behavior (Figure 1—figure supplement 4D and E). We then expressed HaloTag-Ubx from the 20x UAS promoter with the nos::GAL4 (nanos promoter driving GAL4) driver line, which drives HaloTag-Ubx expression in all cells at early developmental stages. We injected the HaloTag ligand of Janelia Fluor 635 (JF635) (Grimm et al., 2017) into these live embryos. JF635 is minimally fluorescent in solution but its fluorescence increases by over 100-fold when bound to a HaloTag protein, allowing the detection of labeled Ubx molecules against a background of dim freely diffusing dyes. The fluorescence intensity of labeled Ubx scaled with distance from the site of dye injection (Figure 1—figure supplement 4B and C), consistent with dye diffusion from the site of injection. To measure the time-averaged density of HaloTag-Ubx in specific locations of nuclei in live embryos in early stage 5, we calculated the summed intensity over 100 s (1000 frames at 100 ms per frame). We observed regions of Ubx signal (3-10x background) similar to the high-intensity clusters observed in fixed embryos (Figure 1F). We examined the dynamics of HaloTag-Ubx in nuclei by plotting fluorescence intensity over time (Figure 1G and H and Figure 1—figure supplement 5). We found that fluorescence signals over time changed in discrete up or down steps, indicating that individual HaloTag-Ubx molecules bind to specific nuclear domains with residence times on the order of a second before dissociation. Most unbound Ubx molecules move too quickly to be captured with the 100 ms exposure time; they move in and out of a diffraction-limited region in significantly less than 100 ms on average. These timescales are consistent with transcription factor-DNA binding dynamics measured in live-cell imaging experiments using mammalian cell lines (Liu et al., 2014; Izeddin et al., 2014; Voss et al., 2011; Normanno et al., 2015; Morisaki et al., 2014; Gebhardt et al., 2013). These repeated binding events produced the high intensities observed in the time-averaged projections and indicate that Ubx concentrates and remains within specific nuclear regions.
Observation of embryos at late stage 6 showed that total HaloTag-Ubx concentration continued to increase as the embryo ages (Figure 1—figure supplement 6A and B). Embryos at late stage 6 had nuclei containing high background concentrations of Ubx that masked single-molecule events, as well as displaying larger sites (>4 × 4 pixels) that constantly remained bright, possibly indicating the presence of multiple molecules or protein aggregation (Figure 1—figure supplement 6C and D). In contrast, the embryos observed during stage 5 did not contain areas that remained constantly bright, suggesting that we observed single molecule dynamics in stage 5 embryos.
To determine whether regions of high Ubx concentration depended on DNA binding, we performed the same experiments with a version of the HaloTag-Ubx transgene where Arg3 and Asn51 of the homeodomain were mutated to Ala (R3A and N51A), abrogating DNA binding (Slattery et al., 2011b). Both the wild-type and DNA-binding deficient Ubx were expressed and imported into the nucleus (Figure 1—figure supplement 7A,B,D,E,G, and H), suggesting that the protein is stable. In contrast, an unstable HaloTag-NLS construct (NLS from H2B) serving as a negative control, neither increased JF635 fluorescence post injection nor became enriched into the nucleus (Figure 1—figure supplement 7C,F, and I). The mutant HaloTag-Ubx (R3A N51A) did not display spatial heterogeneity and exhibited only extremely brief fluctuations in intensity inconsistent with transcription-factor DNA-binding events (Figure 1I and J). These results suggest that binding of Ubx to DNA is required to generate restricted nuclear distributions of Ubx.
The heterogeneous distributions of Ubx we observed are consistent with the hypothesis of nuclear ‘microenvironments’ (Reiter et al., 2017), whereby high local concentrations of transcription factors may drive transcription. Therefore, we examined whether these regions of high Ubx concentration co-localized with sites of active transcription. The svb gene is directly regulated by Ubx protein through binding of Ubx to low-affinity sites in multiple svb enhancers (Crocker et al., 2015). We marked sites of active svb transcription by fluorescence in situ hybridization (FISH) and compared the localization of actively transcribed svb loci to Ubx protein concentration (Figure 2A and B). We observed high local Ubx concentrations surrounding active svb transcription sites (Figure 2C–F). To quantify Ubx distributions around these sites, we calculated the radially averaged Ubx intensity as a function of distance r from the point of maximum FISH intensity for each svb transcription site (Figure 2G–I). Ubx intensity was normalized to one at r = 0 (maximum FISH intensity) and averaged across all sites measured. To adjust for background fluorescence, we located the minimum intensity in the averaged Ubx distribution (r = 2–4 μm) and subtracted that value from the distribution. The first micrometer of the radially averaged 3D distribution is shown, with the shaded area representing the variance (Figure 2J). Within the first micrometer, svb transcription sites showed a relative enrichment of Ubx. Because these sites are on average within 200 nm of a local intensity maximum, Ubx intensity decreased monotonically away from the transcription sites, leading to a relatively constant variance after 200 nm. The normalized Ubx intensity after background subtraction at the site of svb transcription was 0.60 ± 0.17 (n = 59, four embryos, uncertainty is the variance of the background) and decreased approximately 250 nm away from the site. Thus, active svb transcription sites colocalized with areas of high Ubx concentration spanning approximately a few hundred nanometers.
If Ubx protein co-localizes with actively transcribed svb loci because Ubx drives svb expression, then we would expect that transcription at a locus not regulated by Ubx should not co-localize with high Ubx concentrations. Indeed, we observed that active transcription sites driven by a synthetic enhancer containing binding sites for a TALEA transcription factor (Crocker et al., 2016a; Crocker and Stern, 2013; Crocker et al., 2017) did not show Ubx enrichment on average despite wide fluctuations in Ubx levels, with a relative enrichment of Ubx at TALEA-driven enhancers of 0.02 ± 0.63 (Figure 3A–C, n = 29, three embryos). As these transcription sites are not close to maxima of Ubx intensity, the variance in these distributions incresed with distance from the site of transcription.
In numerous nuclei actively transcribing svb on the X chromosome, we observed what appeared to be two transcription sites within 200 nm of each other (Figure 2—figure supplement 1A and B). This indicates that the svb locus on homologous X chromosomes often co-localizes to the same Ubx microenvironment. There are several possible mechanisms that could explain this observation. We consider two broad classes of mechanism. First, a unique chromosomal signature specific to the region containing the svb locus could facilitate localization of homologous alleles to the same transcriptional microenvironments. Second, microenvironments contain distinct combinations of transcription factors and enhancers localize to the relevant microenvironments to enable transcription. To distinguish between these alternative hypotheses, we examined the spatial distribution of the native svb locus, located on the X chromosome, and a single svb enhancer driving lacZ expression which we placed on chromosome 3.
Double-FISH experiments revealed that the native svb locus and the ectopic svb enhancer co-localized often in nuclei in which both were transcribed (Figure 2—figure supplement 1C and D). In contrast, the transcription sites of forkhead (fkh, also on chromosome 3) did not colocalize with the svb locus (Figure 2—figure supplement 1E). The average distance between pairs of related transcription sites (svb-svb, svb-7H, and svb-E3N) within single nuclei is approximately 250 nm, near the resolution limit of AiryScan images (Figure 2—figure supplement 1F). On the other hand, fkh and svb transcription sites are on average 1 µm apart. These results indicate that related enhancers co-localize in transcriptional microenvironments independently of their chromosomal location. This suggests that transcription factor microenvironments are highly differentiated and that related enhancers often exploit the same transcriptional microenvironments.
The experiments described so far showed that the actively transcribed native svb locus co-localizes with local concentration maxima of Ubx in the nucleus. We wondered whether the position of actively transcribed enhancers within Ubx microenvironments depended on Ubx binding site affinity. To address this question, we examined transcription driven by the individual svb enhancers DG3, E3N, and 7 hr, each of which contains a cluster of low-affinity Ubx-binding sites and can independently drive transcription of a reporter gene when moved from their native location (Crocker et al., 2015). Transcription sites driven by these relocated enhancers also colocalized with regions of high Ubx concentration (Figure 3D). The relative Ubx enrichment for each of the three enhancers was 0.56 ± 0.16 for DG3 (n = 61, three embryos), 0.51 ± 0.19 for E3N (n = 142, 11 embryos), and 0.68 ± 0.10 for 7 hr (n = 38, three embryos) (Figure 3E–H,M,N). These results indicate that low-affinity enhancers actively transcribed far from the native svb locus also co-localize with microenvironments of high Ubx concentrations.
Increasing the binding affinity of a site should increase its sensitivity to Ubx and allow transcriptional activation at lower Ubx concentrations. We found previously that replacing a single low-affinity Ubx site with one of a higher affinity led to higher levels of expression and sometimes drove promiscuous transcription (Crocker et al., 2015), suggesting that more stable Ubx-DNA interactions allowed higher transcriptional activation. Consistent with these previous results, we observed that increasing the affinity of a single low-affinity binding site in the E3N enhancer decreased Ubx enrichment near transcription sites to 0.44 ± 0.27 (Figure 3I and J, E3N High Affinity, n = 36, three embryos).
In contrast, we reported previously that deletion of low-affinity binding sites reduced transcription (Crocker et al., 2015). Removing some Ubx-binding sites should lower the effective affinity of the enhancer, and we hypothesized that this might result in transcription only when genes are localized to areas of higher Ubx concentrations. Consistent with this model, when we deleted two low-affinity sites in E3N, active transcription was observed in regions of increased Ubx enrichment (0.65 ± 0.18, Figure 3K and L, E3N Mut23, n = 62, five embryos). Deletion of two low-affinity Ubx sites from the 7 hr enhancer did not alter Ubx enrichment around transcription sites (0.63 ± 0.37, Figure 3O and P, 7H Mut23 n = 81, six embryos). But, deletion of three Ubx-binding sites in the 7H enhancer increased relative Ubx enrichment, consistent with the pattern we observed for the E3N enhancer (0.91 ± 0.27, Figure 3Q and R, 7H Mut123, n = 52, eight embryos).
Across all manipulations, we observed an inverse correlation between binding site affinity and the distribution of Ubx intensities at transcription sites (Figure 3—figure supplement 1). Thus, the number of Ubx-binding sites and their affinities determine the response of svb enhancers to local Ubx concentration. Lower affinity enhancers require higher Ubx concentrations to drive transcription. Conversely, higher affinity enhancers can drive transcription at lower local Ubx concentrations.
Taken together, these data suggest that enhancers may be dynamically sampling local nuclear environments. A lower fraction of nuclei showing transcription from enhancers with binding site deletions (Figure 3K,O,Q) may occur because there are fewer areas of the nucleus in which peak Ubx levels are sufficient for weakened svb elements.
Co-factors can stabilize low-affinity binding interactions through cooperative and scaffolding interactions with transcription factors. A co-factor-dependent enhancer would require sufficient concentrations of both the factor and the co-factor to drive transcription. The homeodomain proteins Extradenticle (Exd)/Pbx and Homothorax (Hth)/MEIS (Slattery et al., 2011b; Rieckhof et al., 1997; Ryoo and Mann, 1999; Lelli et al., 2011) interact with Ubx during DNA binding, and Ubx and Hth regulate a partially overlapping set of genes (Choo et al., 2011; Slattery et al., 2011a). In vitro, Ubx requires Hth/Exd to bind to the low-affinity sites in 7H and E3N (Crocker et al., 2015). In vivo, Hth deficiency led to the loss of expression for both 7H and E3N (Figure 4A–D). Consistent with this requirement for both Ubx and Hth, Hth was co-enriched with Ubx around active transcription sites driven by 7H or E3N (Figure 4E–T). The relative enrichment for Ubx and Hth, respectively, was 0.58 ± 0.14 and 0.41 ± 0.16 for 7H (n = 51, seven embryos) and 0.66 ± 0.13 and 0.39 ± 0.24 for E3N (n = 74, five embryos). These results suggest that transcription from co-factor-dependent enhancers requires microenvironments that contain high concentrations of both transcription factors and their co-factors. This observation provides further support for the model that transcription factor microenvironments are present as multiple highly differentiated transcription domains containing unique combinations of transcription factors.
Biological systems often generate locally high concentrations of interacting molecules to increase the efficiency of biochemical reactions (Dueber et al., 2009; Oehler and Müller-Hill, 2010). This appears to be true also for transcription from low-affinity enhancers. Microenvironments (Reiter et al., 2017) of high local concentrations of transcription factors and their co-factors may circumvent the instability of low-affinity interactions by promoting more frequent DNA binding and cooperative interactions when enhancers are located within these domains (Farley et al., 2016) (Figure 4U and V). These microenvironments may be relatively stable domains generated by rapid dynamics of individual molecules. For example, we observed interactions between transcription factors and DNA on the timescale of seconds, with transcription factors continuously arriving to and departing from specific loci. From the perspective of gene expression, transcription likely occurs intermittently, switching on and off as the gene locus samples different nuclear regions. These rapid dynamics ensure that, once the gene locus moves outside of a microenvironment, or the conditions to form microenvironments are no longer satisfied, then the transcription factors needed to sustain expression quickly depart from low-affinity binding sites. In contrast, the fact that svb enhancers placed on the third chromosome often co-localized with the native svb locus on the X chromosome suggests that unique microenvironments may have relatively long half-lives. One challenge for the future is to determine how rapid dynamics of individual molecules generates apparently stable sub-nuclear domains.
Many mechanisms might work in concert to create these observed microenvironments. First, clustered binding sites for the same transcription factor (Crocker et al., 2016b) could lengthen the dwell time of proteins near enhancers and increase effective local protein concentrations (Yao et al., 2006; Zhang et al., 2006; Elf et al., 2007; Kabata et al., 1993; Leith et al., 2012; Ruusala and Crothers, 1992). Second, cooperative and scaffolding interactions between transcription factors and co-factors, each of which may bind independently to enhancers, can stabilize transcription factors at low-affinity sites (Farley et al., 2016; Junion et al., 2012). Finally, clustering of enhancers could trap transcription factors over longer length scales (Noordermeer et al., 2014; de Laat and Duboule, 2013; Symmons et al., 2016; Williamson et al., 2016; Giorgetti et al., 2016), perhaps generating the ~200 nm microenvironments that we observed. This last model is supported by recent findings that multiple promoters can share the same enhancer in a common local environment (Fukaya et al., 2016).
Transcription factor microenvironments may be a general feature of eukaryotic transcription, as supported by studies showing mouse and human cells exhibiting RNA polymerase II crowding (Cisse et al., 2013; Cho et al., 2016), transcription factors using local clustering to efficiently find their binding sites (Liu et al., 2014; Izeddin et al., 2014), and chromatin packaging in Drosophila cells generating distinct chromatin environments at the kilobase-to-megabase scale (Boettiger et al., 2016). Collectively, these findings are consistent with a phase-separated model of transcriptional regulation (Hnisz et al., 2017) whereby distinct microenvironments contain different combinations of proteins inside the nucleus. These localized regions impose a spatial constraint on the expression of genes, allowing transcriptional activation from enhancers only when they are physically in regions with the correct combinations of transcription factors and co-factors. Multiple enhancers acting as DNA scaffolds for protein binding could provide the anchoring interactions that form transcriptional microenvironments. These microenvironments would, in turn, provide a mechanism to allow both efficient and specific transcription from low-affinity enhancers.
D. melanogaster strains were maintained under standard laboratory conditions. All enhancer constructs were cloned into the placZattB expression construct with a hsp70 promoter (Crocker et al., 2015). Transgenic fly lines were made by Rainbow Transgenic Flies Inc. E3 and 7H were integrated at the attP2 landing site. DG3 was integrated at ZH-86Fb.
Flies were reared at 25°C and embryos were fixed and stained according to standard protocols (Crocker et al., 2015). Primary antibodies were detected using secondary antibodies labeled with Alexa Fluor dyes (1:500, Invitrogen). In situ hybridizations were performed using DIG or biotin-labeled, antisense RNA-probes against a reporter construct RNA (lacZ) or the first intron of svb or fkh. DIG-labeled RNA products were detected with a DIG antibody: Invitrogen, 9H27L19 (1:200 dilution) and biotin-labeled RNA products are detected using a biotin antibody: Pierce, PA1-26792 (1:200).
The following primary antibodies for proteins were used at the indicated concentrations:
Ubx: Developmental Studies Hybridoma Bank, FP3.38-C (1:20)
Hth: Santa Cruz Biotechnology (dN-19), sc-26186 (1:50)
Eve: Developmental Studies Hybridoma Bank, 2B8-C (1:20)
AbdA: Santa Cruz Biotechnology (dN-17), sc-27063 (1:50)
En: Santa Cruz Biotechnology (d-300), sc-28640 (1:50)
RNA PolII RPB1 (Ser5 phosphorylated): BioLegend, (920304), (1:200)
Histone H3K27me3: Active Motif, 39157 (1:200)
Histone H3K4me3: Cell-signaling technology C42D8 (1:200)
LacZ: Promega anti-ß-Gal antibody (1:1000)
Fixed Drosophila embryos mounted in ProLong Gold mounting media (Molecular Probes, Eugene, OR) were imaged on a Zeiss LSM 880 confocal microscope with Airyscan (Carl Zeiss Microscopy, Jena, Germany) using 3D Airyscan in SR mode to obtain images with 1.7-fold higher resolution compared to diffraction-limited confocal imaging (Sheppard et al., 2013) (method supplements: imaging setup for Airyscan). Images presented in the figures were processed with ImageJ (Schindelin et al., 2015).
To expand embryos, after fixation and staining, embryos were embedded into poly-acrylate gels and expended according to a previously published protocol (Tillberg et al., 2016) (method supplements: handling expansion gels).
Expanded gels containing embryos were imaged in 6-well glass bottom plates (Cellvis, Mountain View, CA) using a Zeiss LSM 800 confocal microscope (Carl Zeiss Microscopy, Jena, Germany) using standard settings (method supplements: imaging setup for expanded embryos).
Transgenic fly lines containing HaloTag-Ubx under the control of both a hsp70 and a 20x UAS promoter was made by Rainbow Transgenic Flies Inc. The lines were made homozygous for the transgene.
Embryos resulting from crossing the homozygous line with the HaloTag-Ubx transgene with a nos::GAL4 driver line were injected following previously established protocols (Rubin and Spradling, 1982) with the HaloTag ligand of JF635. Briefly, embryos were collected for 30 min at 25°C and placed in oxygen permeable Halocarbon 27 oil. The stock dye solution of 1 mM JF635 with a HaloTag ligand in DMSO was diluted 1:100 into fly injection buffer and injected into the posterior end of the embryos. The embryos were then aged to stage 5 or late stage 6 and imaged in oxygen permeable Halocarbon 27 oil.
Injected embryos were imaged on a customized inverted Nikon Ti-Eclipse (Nikon Instruments, Tokyo, Japan) with the appropriate settings (method supplements: imaging setup for live embryos).
Embryos from the homozygous HaloTag-Ubx transgene line were exposed to 30°C to induce the heat shock promoter and cuticle preps were prepared following previously established protocols (Crocker et al., 2015).
To obtain the distributions of Ubx and Hth around a transcription site, the processed Airyscan stacks obtained from the Zeiss LSM 880 confocal microscope were analyzed in Fiji (Schindelin et al., 2012) using native functions and the 3D ImageJ Suite plugin (Schmid et al., 2010). Radially averaged distributions for individual transcription sites were computed using the 3D ImageJ Suite Plugin. Distributions for all sites were averaged and background offset in Matlab (MathWorks, Natick, MA) using a custom script (method supplements: settings for extracting radially averaged distributions).
All Airyscan images were acquired using a Zeiss Plan-Apochromat 63x/1.4 Oil DIC M27 objective due to its well-characterized point spread function. First an embryo at the appropriate developmental stage (stage 15 for most embryos) and proper orientation was located. The band of mRNA expression in high Ubx regions of the first abdominal (A1) segment was then found. Within that band, areas containing transcription sites in nuclei of high Ubx expression were imaged. Images with both Ubx and Hth were acquired in the same manner by locating the proper area using the mRNA and Ubx. When Ubx was imaged together with RNA polymerase II, a histone marker, or other transcription factors, Ubx expression levels were used to locate the region of interest.
The optimal setting suggested by Zeiss for the number of pixels in the x-y direction (40 nm per pixel) and displacement in the z-stack (190 nm) were used for all Airyscan images. The images from different fluorophores were acquired sequentially with the appropriate laser lines (405 nm, 488 nm, 561 nm, or 633 nm) and spectral filters. The laser power and gain were adjusted to maximize the signal to noise ratio within the dynamic range of the Airyscan detector. The acquired stacks were processed with Zen 2.3 SP1 (Carl Zeiss Microscopy GmbH, Jena, Germany) in 3D mode to obtain super-resolved images.
To allow easier handling of expanded gels, the gels containing embryos were cast into eight-well silicone isolators without adhesives (eight round chambers with a diameter of 9 mm and a thickness of 0.5 mm, Grace Bio-Labs (Bend, OR)) and allowed to polymerize. The gels were transferred into a six-well glass-bottom cell culture plate (Cellvis, Mountain View, CA) and expanded using ultrapure water containing 500 nM DAPI. Before imaging, the water was removed and the gel encased in 3% low melting temperature agarose (NuSieve GTG Agarose, Lonza Group Ltd, Basel, Switzerland), taking care not to allow the agarose to flow under the gel and float the gel away from the cover glass bottom. Water was then added back into the wells to prevent drying.
A long working-distance water immersion objective, the Zeiss LCI Plan-Neofluar 25x/0.8 Imm Korr DIC M27, was selected for index-matching with the gel and its ability to image up to 400 µm above the surface of the coverslip. Stage 15 embryos in the correct orientation were located using the DAPI and Ubx staining. Regions of low to high Ubx expression were imaged sequentially using the appropriate laser lines (405 nm, 488 nm, or 561 nm) with the proper spectral filters. The laser power settings and the gain were selected to maximize signal to noise within the dynamic range of the detector. The full field of view of the microscope was imaged with 2048 × 2048 pixels and with a z-step of 1 μm. The final images presented were processed in ImageJ (Schindelin et al., 2015).
All videos were collected under a Nikon CFI Plan Apo NCG 100X Oil NA 1.41 objective with an Andor iXon 897 EMCCD camera (Andor Technology Ltd., Belfast, UK). Embryos at stage 5 and late stage 6 in the correct orientation were found and imaged. We selected an area in the middle of the embryo with enough dye-labeled Ubx molecules to observe single molecules and we avoided regions close to the injection site to avoid oversaturating the camera (compare with Figure S5A-D where there are too many labeled Ubx). The samples were illuminated with a 633 nm laser to image the JF635 tagged Halo-Ubx molecules with laser power and camera gain set to maximize signal from individual Ubx molecules without oversaturating the EMCCD detector. The 512 × 512 pixel videos were acquired at an exposure time of 100 ms per frame for up to 200 s. Images were processed using ImageJ to generate the time-averaged images and the intensity-over-time traces presented in the figures.
To extract radially averaged protein distributions, we used Fiji to identify transcription sites inside nuclei by thresholding at a level that is roughly 50-fold above the background intensity. The center of a transcription site was defined as the pixel of maximum intensity in 3D in the mRNA channel inside a nucleus with high levels of Ubx expression. The radially averaged distribution out to a radius of 4 μm from transcription site for the transcription factor in 3D was computed using the 3D ImageJ Suite. The suite generates the distribution by computing the average intensity on the surface of a sphere with a radius r from the center in three dimensions for all the values of r ranging from zero to a desired outer limit (4 μm in this case).
The individual distributions from each transcription site were normalized to have the intensity at the center (r = 0) equal to 1. The distributions were averaged and background offset in Matlab. To adjust for background Ubx intensity outside of the nucleus, the entire averaged distribution was offset by a constant value to bring the minimum intensity present in the distribution to zero to generate the distribution plots. The shaded area around the line represents the variance. The first μm of the distributions, where contributions from outside of the nucleus were minimal, are shown in the figures. The relative enrichment of Ubx or Hth for each enhancer variant is the intensity at r = 0 in the distribution and the cited uncertainty is the variance at the location of zero Ubx or Hth intensity (the site of minimum intensity before offsetting, between 2 and 4 μm from the transcription site).
The initial dataset for 7H enhancers contained only a part of the deletion series. A subsequent dataset contained all the 7H deletion mutants. The 7H mutants present in both sets were compared and the distributions of Ubx intensity between the sets were found to differ by a multiplicative factor. When such factor was computed for each overlapping 7H mutant present in both datasets, the results were similar, indicating that there was a systematic shift in background noise. This could have resulted from differences in embryo handling during fixation, antibody staining, and other steps in sample preparation. Other characteristics such as the functional form of the distributions between the two sets and the trends between 7H mutants within each set remained unchanged after correcting for the difference in intensity. The wild-type 7H data from the first set with a correction factor and the rest of the deletion series uncorrected from the second set were used to minimize the normalization employed.
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David N ArnostiReviewing Editor; Michigan State University, United States
In the interests of transparency, eLife includes the editorial decision letter and accompanying author responses. A lightly edited version of the letter sent to the authors after peer review is shown, indicating the most substantive concerns; minor comments are not usually included.
Thank you for submitting your article "Nuclear microenvironments modulate transcription from low-affinity enhancers" for consideration by eLife. Your article has been favorably evaluated by Jessica Tyler (Senior Editor) and four reviewers, one of whom is a member of our Board of Reviewing Editors. The following individuals involved in review of your submission have agreed to reveal their identity: Robert P Zinzen (Reviewer #2); Stephen J. Small (Reviewer #3).
The reviewers have discussed the reviews with one another and the Reviewing Editor has drafted this decision to help you prepare a revised submission.
The reviewers of your manuscript found that the observations on the inhomogeneity of intranuclear Ubx transcription factor concentration and the activation of homologous enhancers with different Ubx affinities were highly significant and convincingly demonstrated. A strength of this study is that the authors use complementary techniques on fixed and living cells to observe the distribution of Ubx and other TF, and see similar trends. The use of svb regulatory elements with carefully "tuned" Ubx affinities and output is another powerful tool that reveals the importance of the different Ubx domains. Overall, the reviewers found that this study uses a set of advanced imaging methods to fundamentally reshape our view of the nuclear environment in the context of developmental gene regulation.
Essential points to be addressed:
1) There was some uncertainty whether the authors are proposing that the change in affinity of the Ubx motifs reshapes the intranuclear concentration gradients, or whether they are just responding differently to the existing inhomogeneities in the nucleus. The statement "Manipulation of binding site number and affinity changes the level of Ubx enrichment around svb enhancers" might be interpreted to mean that the selected enhancers are shaping the nuclear gradients. A clearer understanding of the authors' interpretation is necessary, and better statement of what they propose is establishing the different concentration of Ubx. Another related point: are the authors proposing that the enhancers get "stuck" in areas of appropriate concentration, or do they randomly sample the different intranuclear environments, activating when they are experiencing sufficient Ubx levels?
2) Pertinent to the above point, the in vivo halo-tagged imaging was found to be a very helpful complement to the analysis of fixed material, but the paper should do a better job of explicitly tying the results from the in vivo imaged spots to later work with the fixed, expanded embryos. The halo-tagged construct was not adequately described in the paper (only a brief outline in Figure 1—figure supplement 4). Finally, an important control for the in vivo expression was testing of a DNA-binding deficient form of Ubx, which did not show the inhomogeneous distributions, suggesting that DNA binding to something is essential for formation of the gradients. It was not clear that this negative control protein was expressed, however; a Western blot would demonstrate that the lack of signal is not due to trivial lack of stability.
3) An intriguing point of this paper is that as Ubx motifs are degraded, the active spots become localized only to regions of higher Ubx activity. In addition to the shown mean values that are higher for the low affinity enhancers, it is also clear from the embryo images that the weaker site enhancers are found in fewer nuclei altogether. Is this because the low affinity enhancer is able to respond to Ubx concentrations that are only found in a small percentage of nuclei? The authors are asked to show how the distribution of active enhancers in all nuclei changes as a function of Ubx motif affinity, as well as the mean values in nuclear regions where it is active. In addition, the mean levels of Ubx found in proximity to the active transcription loci have a very small variation at close range, and increase with increasing distance for a small range. Then the variation in concentration appears to be constant (and not continue to increase, as might be expected for searches of larger and larger spaces). The authors are asked to explain the shape of the Ubx distributions noted for the reporter constructs.
4) The reporter constructs with different Ubx affinities were derived from svb enhancer sequences. Do the reporters activate and colocalize with the endogenous svb locus in the fixed specimens? Double FISH with intronic probes should be able to discern this point.https://doi.org/10.7554/eLife.28975.019
Essential points to be addressed:
1) There was some uncertainty whether the authors are proposing that the change in affinity of the Ubx motifs reshapes the intranuclear concentration gradients, or whether they are just responding differently to the existing inhomogeneities in the nucleus. The statement "Manipulation of binding site number and affinity changes the level of Ubx enrichment around svb enhancers" might be interpreted to mean that the selected enhancers are shaping the nuclear gradients. A clearer understanding of the authors' interpretation is necessary, and better statement of what they propose is establishing the different concentration of Ubx.
We agree that the original statement could imply that changing the enhancer architecture changes the distribution of Ubx in the nucleus. We have modified this statement to clarify that we do not expect this to happen. Our interpretation is that the mutated enhancers respond to existing Ubx concentration gradients within the nucleus. Even if the aggregated effects of transcription factor interacting with binding sites could shape their overall distribution, changing only one to three low affinity binding sites out of the thousands of possible Ubx binding sites in the genome of D. melanogaster is unlikely to change Ubx distribution in general.
Another related point: are the authors proposing that the enhancers get "stuck" in areas of appropriate concentration, or do they randomly sample the different intranuclear environments, activating when they are experiencing sufficient Ubx levels?
Our interpretation is that enhancers sample various areas of the nuclear environment and initiate transcription only when Ubx and cofactor concentrations are sufficient, but this is only our working model. In the future, we plan to characterize the dynamics of these interactions using additional live imaging strategies, but this technology is not yet fully operational.
2) Pertinent to the above point, the in vivo halo-tagged imaging was found to be a very helpful complement to the analysis of fixed material, but the paper should do a better job of explicitly tying the results from the in vivo imaged spots to later work with the fixed, expanded embryos.
It is not entirely clear what the reviewers are requesting here. We first observed microenvironments in fixed embryos and then expanded fixed embryos to examine the microenvironments at higher resolution. We then used live imaging to characterize the temporal dynamics of transcription factor binding and found that the dynamics were consistent with the observations of fixed specimens. We explicitly state that the live imaging was performed, in part, to test whether the observations of microenvironments in fixed specimens was an artifact of fixation. The consistency between the live-imaging and fixed specimens suggests that microenvironments are real. All following experiments were performed with fixed, unexpanded embryos.
The halo-tagged construct was not adequately described in the paper (only a brief outline in Figure 1—figure supplement 4).
We have added a description of the HaloTag-Ubx construct when we first introduce it in the Results, referencing the construct diagram in the figure. We also added a more complete description in the Materials and methods section. We also updated the diagram in Figure 1—figure supplement 4 to indicate the location of the actual HaloTag-Ubx sequence to further clarify its architecture. Additionally, we will deposit the construct to Addgene to enable use by the community.
Finally, an important control for the in vivo expression was testing of a DNA-binding deficient form of Ubx, which did not show the inhomogeneous distributions, suggesting that DNA binding to something is essential for formation of the gradients. It was not clear that this negative control protein was expressed, however; a Western blot would demonstrate that the lack of signal is not due to trivial lack of stability.
The DNA-binding deficient Ubx involves only two mutations to alanine in the DNA binding pocket and has previously been reported by Richard Mann and colleagues. With the binding deficient mutant, we still observed that the mutant Ubx is labeled using JF635 with a HaloTag ligand based on the bright fluorescent signals we observed post dye injection. Without a folded and functional HaloTag domain, the dye would have remained dark. The mutant Ubx is also selectively localized into the nucleus, indicating a functional NLS that has not been degraded. We still occasionally observed single-molecules of this Ubx inside the nucleus, but their apparent dwell-time is very short (less than 100 ms). These observations suggest that the mutant protein is expressed and stable so that it is not degraded immediately post translation and can be imported into the nucleus.
We also performed an experiment with just an H2B-derived NLS fused to the HaloTag, which is unstable, and we observed no fluorescence signal beyond background noise and auto-fluorescence. There was no enrichment in the nucleus. This control experiment demonstrates the effect of an unstable protein that is degraded immediately, in sharp contrast with the Ubx binding-deficient mutant. We have added Figure 1—figure supplement 7 and accompanying text in the Results section summarizing this point.
3) An intriguing point of this paper is that as Ubx motifs are degraded, the active spots become localized only to regions of higher Ubx activity. In addition to the shown mean values that are higher for the low affinity enhancers, it is also clear from the embryo images that the weaker site enhancers are found in fewer nuclei altogether. Is this because the low affinity enhancer is able to respond to Ubx concentrations that are only found in a small percentage of nuclei? The authors are asked to show how the distribution of active enhancers in all nuclei changes as a function of Ubx motif affinity, as well as the mean values in nuclear regions where it is active.
We agree with the interpretation that weaker enhancers require higher Ubx concentration to activate transcription. As a result, fewer microenvironments within a nucleus would contain sufficient concentrations of Ubx to activate transcription, lowering the probability that an enhancer exploring different areas within a nucleus would be transcriptionally active at any given moment. However, due to the heterogeneous distributions of Ubx in the nuclei of embryos at stage 15, the average concentration of Ubx over an entire nucleus is a poor representation of the specific conditions within microenvironments. While we observed that these weakened enhancers are active in microenvironments with higher Ubx concentrations, transcription sites are not preferentially located in nuclei of high average Ubx concentration. In fact, we did not observe transcription sites in most nuclei with some of the highest average levels of Ubx. It is known that other transcriptional inputs, both positive and negative, regulate svb transcription (Stern and Orgogozo, 2009). In this case, transcriptional repression may prevent svb expression at peak Ubx concentrations. It would be of interest to explore in greater detail the mechanisms of this activity as a part of our future work.
In addition, the mean levels of Ubx found in proximity to the active transcription loci have a very small variation at close range, and increase with increasing distance for a small range. Then the variation in concentration appears to be constant (and not continue to increase, as might be expected for searches of larger and larger spaces). The authors are asked to explain the shape of the Ubx distributions noted for the reporter constructs.
The convergence of the variance in Ubx intensity to zero at the transcription site is an effect of intensity normalization. The intensity of Ubx directly over the transcription site is normalized to one for each of the transcription sites. We average the distributions for all observed nuclei and then subtract the residual Ubx intensity 4 μm from the transcription site as the average background to generate the plots in Figures 2–4. Because the Ubx intensity at the transcription site is the point of normalization, its variance is zero.
The reviewers made an important observation concerning the relatively constant variance in the Ubx distributions after an initial increase. Because a transcription site may sit slightly off from the local maximum of Ubx concentration, the Ubx intensity distribution close to each site fluctuates within the first 200 nm (which is near the optical resolution of our images taken using AiryScan). This leads to an initial increase in variance as the distributions move away from the transcription sites. However, most transcriptions sites are close to a maximum of Ubx concentration, so Ubx intensity decreases monotonically after initial fluctuations. Because of the relatively uniform shapes of the individual distributions, the variance stops increasing after a short distance from the transcription site. We believe that there is no a priori reason that this must be the case. For example, the individual Ubx distributions around the transcription sites of the synthetic enhancer, which is not under the control of Ubx, fluctuate at random out to the full distance plotted in Figure 3C (out to 1 μm), leading to a variance that increases throughout the plot. We have added this observation into the Results.
4) The reporter constructs with different Ubx affinities were derived from svb enhancer sequences. Do the reporters activate and colocalize with the endogenous svb locus in the fixed specimens? Double FISH with intronic probes should be able to discern this point.
We conducted double FISH experiments and measured the distances of transcription sites between the endogenous svb locus (on the X chromosome) and other transcription sites (on chromosome 3). Enhancers related to svb, which are 7H and E3N, preferentially colocalized close to the svb site in nuclei expressing both, despite being on different chromosomes. The average distance between transcription sites is about 200 nm. The transcription sites for forkhead (fkh), also on chromosome 3, did not preferentially colocalize with svb, with an average distance of 1 μm between transcription sites. In fact, nuclei showing two transcription sites from the svb locus (two bright spots next to each other) also have an average of 200 nm between those pairs of sites. We have added a new section in the Results and a new figure (Figure 2—figure supplement 1) describing this new result. We have also made additions in the Discussion highlighting this result. We would like to thank the reviewers for suggesting this experiment to improve our work.https://doi.org/10.7554/eLife.28975.020
- Albert Tsai
- Robert H Singer
- Albert Tsai
- Anand K Muthusamy
- Luke D Lavis
- Robert H Singer
- David L Stern
- Justin Crocker
- Mariana RP Alves
- Justin Crocker
The funders had no role in study design, data collection and interpretation, or the decision to submit the work for publication.
We thank Richard Mann, Timothée Lionnet, Paul Tillburg, and Brian English for advice and assistance on experimental design. We thank François Payre for advice on data presentation. We thank all members of the Stern and Singer labs for discussion. Albert Tsai is a Damon Runyon Fellow of the Damon Runyon Cancer Research Foundation (DRG 2220–15). Robert H Singer is supported by the 4D Nucleome Award U01-EB21236. Howard Hughes Medical Institute supported Albert Tsai, Anand K Muthusamy, Luke D Lavis, Robert H Singer, David L Stern, and Justin Crocker Mariana R P Alves and Justin Crocker are supported by the European Molecular Biological Laboratory (EMBL).
- David N Arnosti, Michigan State University, United States
© 2017, Tsai et al.
This article is distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use and redistribution provided that the original author and source are credited.
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