Design of a light-conditioned nuclear localization signal

To control nuclear import with light we engineered a conditional Nuclear Localization Signal (cNLS) that would be allosterically blocked in the dark but available for binding to importin in the light (Fig 1A). Previously, the AsLOV2 domain from Avena sativa has been successfully used to control the binding of short, linear sequence epitopes [14–16] and does not contain an endogenous nuclear localization signal. Therefore, to generate an allosterically caged NLS, we first attached the human Myc NLS at the end of the AsLOV2 domain after residue 546, aligning the proline residue from the NLS sequence to the proline residue of AsLOV2. This fusion protein (AsLOV2cMyc) bound importin α5 with low nanomolar affinity and showed no light-dependence (supplemental). Next, we decided to embed the Myc NLS further into the Jα helix, aligning the alanine residues present in both sequences (Fig 1B). To eliminate the conserved proline residue at the beginning of the NLS, which could disrupt the helicity of the Jα, we performed design simulations with the modeling program Rosetta using the karyopherin-Myc NLS complex structure (PDB: 1EE4). We allowed only the proline residue of the Myc NLS to vary and identified a favorable methionine substitution (Fig 1B and S1 Fig). Rosetta was then used to build a model of the designed NLS sequence, grafted onto the AsLOV2 structure (PDB: 2v0u) creating AsLOV2cNLS. The designed methionine pointed towards solvent, not clashing with any residues from the AsLOV2 domain, and the remaining hydrophobic residues present in the NLS were well packed against the core PAS domain (S1 Fig).

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Fig 1. Design and biophysical characterization of light conditioned nuclear localization signal.

(A) Schematic of the Light Activated Nuclear Shuttle (LANS) design for light activated nuclear import (B) Sequence alignment of the wild type AsLOV2 and the designed AsLOV2cNLS (sequence identity and homology is marked according to CLUSTALW scheme). (C) Fluorescence polarization competitive binding assay of AsLOV2cNLS against human importin α5 and importin α7.

https://doi.org/10.1371/journal.pone.0128443.g001

The switch binds similarly to two distinct importins

Nuclear import efficiency is directly correlated to the binding affinity of a nuclear localization signal for importin α [17]. To determine the binding affinities of the conditioned NLS for human importin α, we adopted a competition-based fluorescence polarization assay [14]. We expressed the AsLOV2cNLS construct and human importins in bacteria, purified them and measured nanomolar affinities for both importins α5 and α7 under blue light irradiation (250 nM and 340 nM, respectively). Their affinities in the absence of light decreased to 1.5 μM for importin α5, and 2 μM for importin α7, which represented a 6-fold change in light/dark affinities (Fig 1C and S2 Fig). Since efficient nuclear localization requires an importin binding affinity tighter than 1 μM [17], these affinity ranges were predictive of efficient nuclear import upon light stimulus and reduced translocation in its absence. The similar binding affinities to two distinct importin α proteins implies that the switch’s nuclear translocation could be mediated by more than one importin in vivo. Lastly, we tested whether the chimeric sequence affects the AsLOV2 photocycle. We observed that the dark reversion rate of the AsLOV2cNLS does not deviate from that of wild type AsLOV2, with an activated state half-life of 29.5 sec (S2 Fig).

A Nuclear Export Signal is required for the reversible control of nuclear import

To determine whether the AsLOV2cNLS switch could control nuclear localization in live cells, we fused it to mCherry fluorescent protein and observed its sub-cellular distribution in HeLa cells (Fig 2A). In the dark the mCherry fluorescence intensity was almost evenly distributed throughout the cells (Fig 2C top leftmost panel). Incorporating a well-studied AsLOV2 point mutant (I539E) that mimics its lit conformation [18] caused the mCherry signal intensity to concentrate in the nucleus, validating the switch (Fig 2C bottom leftmost panel). Since the nuclear pore complex allows passive diffusion of proteins with molecular weight under 60 kDa [19, 20], we hypothesized that the observed dark state distribution of the 45 kDa mCherry::AsLOV2cNLS protein results from passive diffusion throughout the cell, and that adding a nuclear export sequence (NES) could shift its distribution to the cytoplasm. Hence, we needed to identify the appropriate balance between nuclear import and export signal strength, such that a constitutive NES would be sufficient to remove the switch from the nucleus in the dark but would be overpowered by the strength of the conditional NLS in the light. We screened a panel of five NES sequences that vary in export strength and are derived from human nucleocytoplasmic shuttling proteins: PKI-α [21], p53 [22], Mdm2 [23], Smad4 [24] and p120ctn [25] (Fig 2B). We cloned each of the NES sequences between mCherry and either the wild type or I539E switch variant. For each of the NES variants we quantified the nuclear/cytoplasmic distribution for either the wild type protein in the dark or the lit mimetic, which allowed us to measure steady state distributions without concerns about the precise mode and timing of light stimulation. While the switch with no NES exhibited a 2.64-fold increase in nuclear localization with the lit mimetic, some amount of protein was always present in the nucleus (Dark state = 1.35 ± 0.07 nuclear/cytoplasmic fluorescence, n = 10 and Lit mimetic = 3.57 ± 0.20 nuclear/cytoplasmic fluorescence, n = 10; Fig 2C and 2D). Three of the NES sequences provided lower nuclear fluorescence in the dark, p120ctn, PKI-α, and Smad4 (Fig 2C). However, the NES motif from p120ctn was so strong that nuclear localization was not observed with the lit mutation. The greatest change in nuclear/cytoplasmic fluorescence (6.2 fold) was observed with the NES from Smad4 (Dark state = 0.45 ± 0.02 nuclear/cytoplasmic fluorescence, n = 10 and Lit mimetic = 2.81 ± 0.19 nuclear/cytoplasmic fluorescence, n = 10).

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Fig 2. Confocal microscopy of LANS in HeLa cells.

(A) Schematic of the LANS constructs (B) List of the nuclear export signals tested. (C) Representative nuclear optical slices of cells used for the quantification of the nuclear/cytoplasmic distribution of the switch (scale bar = 15 μm). (D) Quantification of the effect of the nuclear export signal on the nuclear/cytoplasmic distribution of LANS (D—wild type construct imaged in the dark, L—lit mimetic I539E). Mean is reported ±SEM and statistical significance calculated with unpaired two-tailed t-students test; NS—Not Significant.

https://doi.org/10.1371/journal.pone.0128443.g002

To confirm that exclusion of the constructs from the nucleus required active nuclear export, we treated cells with the Crm1 inhibitor Leptomycin B [26]. Leptomycin B treatment led to loss of nuclear exclusion and restoration of the no-NES construct cellular distribution for all but the p53 and Mdm2 NES (S3 Fig), indicating that the switch constitutively shuttles between the nucleus and the cytoplasm, and confirming that its nuclear export is mediated by Crm1. We therefore named the AsLOV2cNLS switch coupled with an NES the Light Activatible Nuclear Shuttle (LANS). Here, we refer to different LANS constructs by adding a suffix that denotes the NES used: LANS0 carries no NES, while LANS1-5 use the nuclear export signals of PKI-α, p53, Mdm2, Smad4 and p120ctn, respectively (Fig 2B). LANS remains functional when short peptide or large globular proteins are fused to its C-terminus (S3 Fig).

LANS is imported and exported within minutes in a variety of mammalian cell cultures

We next sought to characterize the kinetics of nuclear import and export in response to light stimulation. We performed blue light stimulation and measured the rates of nuclear import and dark reversion for LANS4 in three types of mammalian tissue culture cells—HeLa, Cos7 and HEK293 (Fig 3A, 3B and S1–S3 Movies). Nuclear fluorescence upon activation was measured and fold changes of nuclear accumulation were fit by single exponentials with t_1/2 = 3.3 ± 0.02 minutes for HeLa (n = 4), t_1/2 = 2.7 ± 0.03 minutes for Cos7 (n = 3) and t_1/2 = 5.9 ± 0.01 minutes for HEK293 (n = 5) (Fig 3C). Upon stopping the blue light stimulation, the nuclear export kinetics were similarly measured and fit, yielding t_1/2 = 2.5 ± 0.01 minutes for HeLa, t_1/2 = 2.8 ± 0.02 minutes for Cos7 and t_1/2 = 3.2 ± 0.02 minutes for HEK293 (Fig 3C). The differences observed between the cell types may result from differential expression of importins and exportins [27]. Nuclear localization appeared fully reversible, with no significant loss in activation level after multiple cycles of blue light activation and reversion over the course of a few hours (Fig 3D).

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Fig 3. Real time light induced nuclear translocation of LANS4 in mammalian tissue culture cells.

(A) Representative images for light activation and reversion in HeLa cells and Cos7 (B) (scale bar = 25 μm); (c) Plotting the fold change of nuclear accumulations in HeLa, Cos7 and HEK293 (n = 4 each, mean reported ± SEM with dashed line). See also S1, S2 and S3 Movies. The blue shaded region indicates pulsed blue light activation (see Supplemental experimental procedures). (C) Multple activation reversion cycles in Cos7 (n = 2, mean reported ± SEM with shaded grey area). The blue shaded regions indicate pulsed blue light activation.

https://doi.org/10.1371/journal.pone.0128443.g003

LANS enables robust transcriptional control in yeast

To determine whether LANS could be used to control protein function in cells, we sought light-mediated control of transcription in yeast. We used the NMY51 yeast strain (Fig 4A) and an NLS reported plasmid system [28] to which we fused LANS4 to its C-terminus (Fig 4B). Colony growth assays showed light-dependent survival when grown on media lacking histidine and adenine with no background detected for the vector (Fig 4C). Normal yeast growth was not affected by blue light (Fig 4C, left panel: growth minus leucine). We then grew liquid cultures in light and dark and performed β-galactosidase assays to quantify the levels of transcriptional activation. A 21-fold change in signal was observed (8.8 ± 0.7 Miller Units (n = 3) in the dark and 187 ± 24 Miller Units (n = 3) in the light). No detectable transcription was seen for a construct with a mutated conditional nuclear localization signal where all lysines and arginines were substituted with alanines (MAAAAVALD). These data demonstrate that LANS can be used to control the activity of a transcription factor by regulating its nuclear localization.

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Fig 4. Light induced transcription via light mediated nuclear translocation in yeast.

(A) NMY51 contains his3, ade2 and lacZ genomic reporter genes under the control of LexAop. (B) Schematic of the LANS controlled artificial transcription factor in yeast (C) Growth assay of LANS controlled transcription factor in NMY51. The left panel shows growth on media lacking leucine, which confers plasmid resistance and demonstrates that the light used does not affect regular yeast growth. The right panel demonstrates light dependent growth on media lacking leucine, histidine and adenine. (D) β-galactosidase activity measurements upon blue light induced transcription activation with LANS4 n = 3 each, mean reported ± SEM and statistical significance is calculated with unpaired two-tailed t-student’s test (p = 0.0019).

https://doi.org/10.1371/journal.pone.0128443.g004

LANS can be used to precisely control nuclear translocation in C. elegans embryos

To test whether LANS can be used to regulate protein nuclear localization in vivo, we took advantage of the optical clarity and ease of genetic manipulation of the C. elegans embryo. We fused LANS4 to the red fluorescent protein mKate2 (Fig 5A) and expressed it in C. elegans embryos under the control of the his-72 promoter and tbb-2 3’UTR. This promoter and 3’UTR support ubiquitous expression throughout development, with the strongest expression in developing embryos ([29] and D.J.D., unpublished observations). The fusion protein was cytosolic in embryos kept in the dark, but translocated rapidly (< 2 minutes) into the nucleus upon blue light activation (Fig 5B and S4 Movie). It returned fast (< 3 minutes) to the cytosol after the illumination was stopped. Expression and photoactivation of LANS did not appear to cause toxicity, since the embryos continued developing normally and hatched into viable L1 larvae after the experiment (n = 8 embryos from 2 separate experiments). We next tested whether we could achieve precise spatial control of nuclear translocation by targeting photoactivation to a single cell. For these experiments, we used embryos expressing mKate2::LANS4 in mesodermal precursors of the MS cell lineage under the control of the ceh-51 promoter [30]. Illumination of a cell expressing mKate2::LANS4 resulted in rapid nuclear translocation, which was reversed when the illumination was stopped (Cell 1 in Fig 5C and 5D and S5 Movie). No change in mKate2::LANS4 localization was detectable in a neighbouring cell that was not illuminated (Cell 2 in Fig 5C and 5D and S5 Movie). The activation and recovery curves were well fit by single exponentials with t_1/2 = 49 ± 9 seconds for activation and t_1/2 = 67 ± 9 for recovery (n = 11 experiments). We conclude that LANS can be used to control nuclear localization with high temporal and spatial precision in a living C. elegans.

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Fig 5. Light activated nuclear translocation in C. elegans embryo.

(A) Schematic of the mKate2::LANS construct that was expressed in C. elegans embryos (B) Confocal images of an embryo expressing mKate2::LANS ubiquitously and subjected to photoactivation with blue light. Scale bars represent 10 μm. See also S4 Movie. (C) Left: Confocal images of four mKate2::LANS expressing MS lineage cells on the ventral surface of a late gastrulation-stage embryo. The blue box in the center image indicates the region that was photoactivated with blue light. Brightness and contrast were adjusted to compensate for photobleaching. Scale bar represents 5 μm. Right: Sketches summarizing the observed localization. Numbers correspond to the cell numbers in (D). See also S5 Movie. (D) Quantification of nuclear and cytoplasmic fluorescence intensities as a function of time for the two cells labelled in (C). Cell 1 was illuminated with blue light, and Cell 2 is a neighboring cell. These measurements were corrected for photobleaching (see materials and methods).

https://doi.org/10.1371/journal.pone.0128443.g005

LANS can be used to manipulate cell fate in vivo

To test whether LANS could be used to control the activity of a protein in vivo, we sought to manipulate the development of the C. elegans vulva, a classical model system for studying cell fate specification [31]. During the third larval stage, six vulval precursor cells with equivalent developmental potential can be induced to adopt either primary or secondary vulval fates in response to an EGF signal from the nearby anchor cell. In wild type animals, a single cell called P6.p receives the strongest EGF signal and adopts the primary vulval fate. Its neighbors, P5.p and P7.p, adopt the secondary vulval fate in response to a weaker EGF signal from the anchor cell together with a Notch signal from P6.p [31]. The remaining 3 precursor cells normally adopt non-vulval fates. Activating mutations in the EGF/Ras/Raf/MAPK signalling pathway cause ectopic induction of the primary vulval fate, resulting in a Multivulval (Muv) phenotype. Loss-of-function mutations in this pathway impair vulval induction and cause a Vulvaless (Vul) phenotype [31].

The LIN-1/ETS transcription factor is a downstream target of the MAPK pathway and is thought to function as an inhibitor of the primary vulval fate (Fig 6A). Strong lin-1 loss of function mutations cause all six vulval cells to adopt primary or secondary vulval fates, independent of the activity of the MAPK pathway, resulting in a strong Multivulval phenotype [32–34]. Conversely, gain of function mutations in lin-1 result in repression of the primary vulval fate [35]. MAPK phosphorylates LIN-1 on multiple residues in its C-terminal tail (Fig 6B), which inactivates LIN-1 and allows cells to adopt the primary vulval fate [35].

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Fig 6. Control of vulval development via photoactivatable LIN-1.

(A) Simplified schematic of the role of LIN-1 in vulval fate specification. (B) Top: Schematic of the wild type LIN-1 protein. Bottom: Schematic of the LIN-1::LANS protein produced after modification of the native lin-1 locus using Cas9-triggered homologous recombination. See also S4 Fig. (C) DIC Images of the developing vulvae in mid-L4 larvae from the indicted strains and conditions. Top panel: Black arrow indicates the normal, symmetric vulval invagination. Middle panel: Black arrow indicates the main vulval invagination, and green arrowhead indicates an extra vulval invagination. Bottom panel: Orange arrowheads indicate small invaginations produced by the secondary vulval precursors, and black arrow indicates the plug of tissue derived from the failed primary cell. Scale bars represent 20 μm. (D) Quantification of phenotypes in the indicated strains and conditions. See Methods for detailed definitions of each phenotype. Numbers at the top of each bar indicate the total number of animals scored in this experiment. These data are from a single experiment; the experiment was repeated three times, using two independently isolated lin-1::lans alleles, with similar results.

https://doi.org/10.1371/journal.pone.0128443.g006

To generate a light-inducible lin-1 allele, we modified the endogenous lin-1 gene using Cas9-triggered homologous recombination [36]. We introduced three molecular changes, with the goal of eliminating the normal regulation of LIN-1 by MAPK and replacing it with optogenetic regulation (Fig 6B and S4 Fig). First, we truncated the C-terminus, mimicking the n1790 gain of function allele that eliminates the MAPK docking site and most of the predicted phosphorylation sites [35]. Second, we mutated a putative endogenous NLS. Third, we inserted sequence encoding mKate2::LANS1. We predicted that the resulting LIN-1::LANS1 fusion protein would be sequestered in the cytosol and inactive in the dark, but would localize to the nucleus and be constitutively active in the light.

We examined the phenotypes of lin-1::lans1 animals raised in the dark or under blue light. Continuous illumination for two days had no effect on the development of wild type animals (Fig 6C and 6D and DJD, unpublished observations), indicating that the light levels used in this experiment were non-toxic. A substantial fraction (38%) of lin-1::lans1 animals raised in the dark exhibited a Multivulval phenotype, consistent with our prediction that LIN-1::LANS1 should have reduced activity in the dark (Fig 6C and 6D). However, it is important to note that this phenotype is less severe and less penetrant than that of lin-1 null alleles [32–34], suggesting that LIN-1::LANS1 retains some activity in the dark. This residual activity may be due to shuttling activity of LANS (see above), which results in the LIN-1::LANS1 transient nuclear localization even in the dark.

Illumination with blue light efficiently suppressed the Multivulval phenotype of lin-1::lans1 animals (5% Muv; p = 0.001, Fisher’s exact test), indicating that LIN-1::LANS1 was activated by blue light. In addition, we observed animals that had, instead of a normal vulval invagination, a plug of tissue flanked by two smaller-than-normal invaginations (Fig 6C). We interpret this as a weak Vulvaless phenotype, in which specification of the primary cell fails, but the secondary cells still invaginate. This phenotype was observed significantly more frequently in animals raised under blue light (Fig 6D; 42% vs. 3%; p = 0.0002, Fisher’s exact test), suggesting that light-activated LIN-1::LANS1 repressed the primary vulval fate, as predicted. Consistent with our interpretation of the weak Vulvaless phenotype, a small fraction (5%) of lin-1::lans1 animals raised under blue light were completely Vulvaless (Fig 6D). It is important to note that the n1790 mutation, on which lin-1::lans1 was modelled, produces a similarly mild Vulvaless phenotype, with 54% of n1790 animals showing vulval defects [35]. The penetrance of Vulvaless / weak Vulvaless phenotypes in lin-1::lans1 animals raised under blue light (54%) is similar to the penetrance of vulval defects in n1790 animals. Taken together, these data indicate that insertion of the LANS1 coding sequence into the lin-1 gene allowed optogenetic control of an endogenous transcription factor and manipulation of cell fate decisions in a living animal.

DNA cloning

All cloning PCR amplifications were performed using high-fidelity Q5 polymerase and all preliminary construct screens were carried out by colony PCR using Taq polymerase. All enzymes were purchased from New England Biolabs (NEB). All plasmids were verified by DNA sequencing (GeneWiz).

Light illumination setup

The illumination setup for the fluorescence polarization assays was as described in Lungu et al, 2012. Briefly, collimated blue LED with maximum emission at 455 nm (Thorlabs) provided 6 mW/cm² illumination to a sample in a 1 cm quartz cuvette.

For the S. cerevisae and C. elegans experiments, a LED strip with maximum emission at 465 nm (Mouser Electronics, cat. #: 901-SB-0465-CT) was placed in an array 25 x 35 cm, 15 cm above the samples in an incubator set at 30°C for yeast and 20°C for C. elegans, thus obtaining even illumination of ± 500 μW/cm² for yeast and ± 250 μW/cm² for C. elegans.

Protein expression

Avena sativa phototropin-1 gene corresponding to residues 404–546 encoding for the LOV2 domain (Uniprot: O49003) was amplified with two-step overlap extension PCR introducing the designed nuclear localization signal and clone in pQE-80L using BamHI and HindIII restriction digest. The resulting plasmid was transformed in BL21 (DE3) pLysS and bacteria grown in 1.5 L Luria Bertani media till reaching OD₆₀₀ ~ 0.6 upon which protein production was induced with 500 mM IPTG overnight (18-20h) at 25°C. Cell pellets were resuspended in 50 mM Tris pH 7.5, 1 M NaCl, 10 mM Imidazole, 10 mM β-ME and 1 mM PMSF and sonicated for 15 mins (5 sec. ON, 5 sec. OFF) on ice at 4°C. Lysed cells were then centrifuged for 30 min at 18564 RCF, then the supernatant filtered through 5 μM filter and loaded on 5 mL HisTrap IMAC columns (GE Healthcare). The columns were washed with 30 CV of 50 mM Tris pH 7.5, 1 M NaCl, 10 mM Imidazole, 10 mM β-ME and eluted on BioLogic LP (BioRad) using a gradient against 50 mM Tris pH 7.5, 100 mM NaCl, 500 mM Imidazole, 10 mM β-ME. The eluted protein was concentrated with Amicon Ultra-15 (Millipore) to 2 mL and subjected to size exclusion chromatography in 50 mM Tris pH 7.5, 100 mM NaCl and 1 mM DTT with HiLoad 16/600 Superdex 75 (GE Healthcare) run on Akta FPLC (Amersham). Importins were expressed and purified in the same way as described above. After IMAC the proteins were concentrated to 5 mL, dialyzed against 5 L of 50 mM Tris pH 7.5 overnight at 4°C and purified over HiTrap Q HP column (GE Healthcare) eluted over a gradient against 50 mM Tris pH 7.5 and 1 M NaCl. Then, the protein was were concentrated to 5 mL and subjected to size exclusion chromatography in 50 mM Tris pH 7.5, 100 mM NaCl and 1 mM DTT with HiLoad 16/600 Superdex 200 (GE Healtchare). All protein concentrations were determined using the BCA assay following manufacture protocol (Thermo Scientific Pierce).

Fluorescence polarization

Peptide of the following sequence GDMAAKRVKLD was synthesized at UNC- Chapel Hill and amine labeled using 5- and 6-Carboxytetramethylrhodamine (TAMRA) dye. Peptide concentration was determined by measuring absorbance of the TAMRA dye at 555 nm using 65,000 M^-1 cm^-1 as extinction coefficient. All fluorescence polarization measurements were performed on FluoroMax3 (Jobin Ybon Horiba) fluorescence spectrometer using 25 nM of the TAMRA labelled peptide in 3 mL of 50 mM Tris pH 7.5, 100 mM NaCl and 1 mM DTT. The dye was excited with polarized light at 555 nm and polarization of emitted light measured at 584 nm. The sample was held in a 1 cm quartz cuvette at 25°C, increasing concentrations of importin α were titrated and two polarization values for dark and lit state binding were recorded for each titration point. The polarization value for the lit state binding was collected after 2 minutes of blue light illumination and for the dark state by another measurement taken after 5 minutes in absence of light for the same titration point. Finally, the competition was fit for one-site total binding with Prism 5 (GraphPad) and IC50 values were used to determine the Kd with the online calculator [42].

Mammalian cell culture

HeLa, Cos7 HEK293T (ATCC) tissue cultures were grown at 37°C, 10% CO₂ in DMEM supplemented with 10% (v/v) HyClone Standard Fetal Bovine Serum (Thermo Scientific) and 1% (v/v) GlutaMAX (GIBCO). Cells were passaged every 2–3 days usually in Nunc T-25 or T-75 culture flasks (Thermo Scientific).

Mammalian cell imaging

Constructs consisting of mCherry and AsLOV2cNLS with or without NES signals located between mCherry and AsLOV2cNLS were cloned in pTriEx with restriction digest cloning using NcoI and HindIII restriction sites. All constructs were sequence verified.

Coverslips were washed with PBS (GIBCO) and coated with 10 μg/ml fibronectin at room temperature for a minimum of 1.5 hours. Cells were seeded for a minimum of 3 hours to overnight, then transfected using FuGENE 6 (Promega) and imaged after about 18 hours post-transfection in Ham’s F-12K medium free of Phenol red (Caisson) and containing 10% FBS buffered with 10 mM HEPES pH 8. Coverslips were mounted in an Attofluor live cell chamber (Invitrogen) placed in a microscope stage with a heated stage adaptor (Warner) and an objective temperature controller (Bioptechs).

An Olympus DSU-IX81 Spinning Disk Confocal coupled with Andor solid-state lasers (Andor) was used to perform the nuclear export signal screen. Z-stacks of 12 μm at 0.5 μm steps were acquired with a PlanApo 60× objective (Oil, N.A. 1.42) using a 561 nm laser set at 20% intensity (150 EM gain and 300 ms exposure).

Live cell timelapse series were collected with an Olympus IX81 epifluorescence microscope equipped with a ZDC focus drift compensator and a Photometrics CoolSnap ES2 CCD camera (Roper Photometrics). A UPlanFLN 40× objective (Oil, N.A. 1.30) was used with an ET572/35x filter for mCherry detection and 1% (UVND 2.0, ET430/24x) for blue light activation of LANS.

Yeast transcription

LANS4 was amplified and cloned into pNIA-CEN-MBP plasmid [28] using EcoRI and BamHI restriction sites. The resultant plasmid was transformed via high efficiency lithium acetate transformation [43] and plated on SC-Leucine droupout agar plates.

Survival assays were performed as follows: Fresh colonies were grown overnight at 30°C in 5 ml SC-Leucine. On the next day, the cell density was measured at OD₆₀₀ and cultures diluted in 200 μl of OD₆₀₀ = 1, followed by 8 5-fold serial dilutions. Then, 5 μl of each of the dilutions were pipetted and spotted using a multichannel pipette (Gilson) onto respective dropout plates. The dark condition plates were wrapped in aluminium foil and placed in the same incubator as the lit condition at 30°C. Blue light (465 nm) at 500 μW/cm² was provided with LED strip lights attached at the incubator (look at illumination settings). Yeast plates were scanned after 72h incubation using an HP ScanJet 4850 scanner and resulting images were cropped and arranged using Adobe Photoshop.

β-Galactose assay were performed as follows: Fresh colonies were grown overnight at 30°C in 5 ml SC-Leucine. On the next day, the cell density was measured at OD₆₀₀ and 2 mL cultures were diluted to OD₆₀₀ = 0.2 in duplicates—one for a light and another for a dark condition (falcon tubes were wrapped in aluminium foil). Cultures were grown at 30°C in a shaking incubator (250rpm) till reaching OD₆₀₀ ± 0.8 in presence or absence of blue light (465 nm) at 500 μW/cm² via LED strip light wrapped around the tube rack. The resulting cultures were pelleted in triplicates and β-Galactose assay using CPRG for a substrate was performed according to the manufacturer (Clontech).

C. elegans culture and strain construction

S1 Table lists the C. elegans strains used in this study including the native N2 [44]. All strains were maintained at 20°C or 25°C on NGM medium, using E. coli strain OP50 as a food source. To express mKate2::LANS4 ubiquitously in early embryos, an mKate2::LANS4 coding sequence was designed using optimal C. elegans codons and synthetic introns [45]. This sequence was assembled from gBlocks gene fragments (Integrated DNA Technologies) using Gibson assembly (New England BioLabs) and cloned into a modified pCFJ352 vector [46] containing the his-72 promoter and tbb-2 3’UTR. This construct was inserted as a single-copy transgene into the ttTi4348 locus on LG I using MosSCI [46]. To express mKate2::LANS4 in MS cells, a construct carrying the mKate2::LANS coding sequence was cloned into a modified pCFJ151 vector [46] containing the ceh-51 promoter and tbb-2 3’UTR. This construct was injected into wild type worms (strain N2) to generate extrachromosomal arrays [47].

To insert LANS1 into the lin-1 locus, we used Cas9-triggered homologous recombination [36]. S4 Fig shows a schematic of our gene targeting strategy. We modified the Cas9–sgRNA expression plasmid pDD162 by inserting the guide sequence ATGACGTCGTGGAGGGCGATA. Next, we constructed a homologous repair template by first cloning a 3.9 kb genomic fragment, comprising the last 3.3 kb of the lin-1 gene followed by a 0.2 kb intergenic region and the first 0.5 kb of the downstream M70.5 gene, into the pCR-Blunt TOPO vector. We made 4 modifications to this construct: 1) We deleted a 1 kb fragment comprising the last 270 bp of lin-1 coding sequence and an intervening intron, and replaced this fragment with the mKate2::LANS1 coding sequence. 2) We mutated the putative NLS sequence RQCRKRSL to AQCAAASL. 3) We inserted a selection cassette, comprising a hygromycin resistance gene [48] followed by unc-58(n495), into the intergenic region downstream of the lin-1 3’UTR. We intended to use the dominant Unc-58 phenotype as a visible marker for the lin-1 allele, but animals generated using this construct do not have an Unc-58 phenotype, indicating that, although unc-58(n495) is a dominant mutation, insertion of a single extra copy of unc-58(n495) into an unc-58(+) background is not sufficient to cause the Unc-58 phenotype. 4) Finally, because lin-1 and M70.5 are close together and located on the same strand, it is possible that the lin-1 3’UTR contains sequences that function in the promoter of M70.5, and that insertion of the selectable marker in the intergenic region between lin-1 and M70.5 could disrupt M70.5 expression. To avoid this, we inserted a second copy of the lin-1 3’UTR downstream of the selectable marker. The sequence of the final homologous repair template is available upon request.

The elk-2 gene of C. elegans has >90% nucleotide sequence identity to the region of lin-1 that we wished to modify, which made it impossible to identify a Cas9 target site that was unique to lin-1. Therefore, to avoid inadvertently modifying elk-2 instead of lin-1, we performed Cas9-triggered homologous recombination in the parent strain VC2110, which carries a deletion in elk-2 that removes part of the region homologous to lin-1, including the Cas9 target site that we selected. An injection mix containing 50 ng/μL Cas9–sgRNA plasmid, 10 ng/μL homologous repair template, and co-injection markers [36] was injected into young VC2110 adults. The injected animals were allowed to lay eggs for 3 days at 25°C, and then hygromycin was added to the plates to a final concentration of 0.5 mg/mL to kill non-transformed animals. After 7 days of selection, the plates were heat shocked for 4h at 34°C to kill animals carrying extrachromosomal arrays (via PEEL-1 negative selection [46]). Candidate lin-1::lans animals that survived both rounds of selection were singled to establish lines, and correct insertion of lans was confirmed by PCR. We then outcrossed to remove the unlinked elk-2 mutation that facilitated strain construction.

Photoactivation experiments in C. elegans embryos

Embryos expressing mKate2::LANS4 were mounted on polylysine-coated coverslips and gently flattened using 2.5% agar pads. For whole-embryo photoactivation experiments (Fig 5B), we used a Nikon Eclipse Ti microscope equipped with a 100X, 1.49 NA objective and a Yokagawa CSU-X1 spinning disk head and controlled using Metamorph (Molecular Devices). Confocal images of mKate2 fluorescense were captured every 10s, and the embryos were illuminated with ~180 μW/cm² of blue light from a 488 nm laser for 5s between each pair of image acquisitions (i.e., 50% photoactivation duty ratio). For single-cell photoactivation experiments (Fig 5C), we used a Zeiss LSM710 laser scanning confocal microscope equipped with a 100X, 1.3 NA objective and controlled by Zeiss Zen software. Images were acquired at 10s intervals, and photoactivation was done between each pair of acquisitions by scanning a 458 nm laser at ~170 W/cm² over a region of interest defined using the FRAP/photoactivation function of the Zen software. Each pixel was illuminated for a total of 63 μs during photoactivation.

To measure mKate2::LANS4 nuclear localization, we made line scans across a region of the image that encompassed the nucleus and cytoplasm of each cell of interest. Pixel intensities were measured from kymographs and converted to fluorescence intensity by subtracting off-embryo background. To correct for photobleaching, we normalized each measurement to the total integrated fluorescence intensity of the entire image.

Scoring of vulval phenotypes

Animals were synchronized by allowing embryos to hatch in the absence of food and arrest as L1 larvae. Synchronized larvae were plated on NGM plates seeded with E. coli OP50, and the plates were placed under blue LED illumination (see above). Dark controls were placed in the same incubator and wrapped in aluminium foil to prevent light exposure. When the animals reached mid-L4 stage (approximately 48 hours), they were mounted on 2.5% agar pads containing 10 mM sodium azide as a paralytic. DIC images of the developing vulva were acquired using a Nikon Eclipse E800 microscope equipped with Nomarski optics and a 100X, 1.4 NA objective. Animals were scored as Normal if there was a single, symmetric vulval invagination; as Multivulval if they had at least one secondary invagination in addition to the main vulva; as “weak Vulvaless” if, instead of a fully formed vulval invagination, there were two small, equally-sized invaginations separated by apparently undifferentiated tissue; as Vulvaless if there was no vulval invagination; and as Deformed if there was a single vulval invagination that was misshapen or asymmetric, or if the morphology was too abnormal to be confidently assigned to one of the other categories. Data were plotted and p values were calculated using Graphpad Prism software.