This study was partly supported by the Basic Science and Platform Technology Program for Innovative Biological Medicine, no. 17am0301014, from the Japan Agency for Medical Research and Development (AMED), Research Grant from MEXT to the RIKEN Center for Life Science Technologies and a Research Grant from MEXT to the RIKEN IMS. We thank members of the PC lab and of the SINEUP network (SISSA, University of Eastern Piedmont and RIKEN) for thought-provoking discussions. We thank Dr. Matthew Valentine for proofreading.

1. Design of BDs of SINEUP Constructs for Target mRNAs
<ol>
	<li>Check transcription starting site (TSS) and translation starting site of target mRNAs in the cells of interest. Acquire TSS data from both the ENCODE and FANTOM projects (cap analysis of gene expression, CAGE) (ZENBU: http://fantom.gsc.riken.jp/zenbu/).</li>
	<li>Open the browser, search genes of interest and check TSS by CAGE peaks.</li>
	<li>Consult the example analysis of cell and tissue specific TSS of Parkinson disease protein 7 (PARK7) mRNA shown in Figure 2.</li>
	<li>Design BD sequences of several different lengths corresponding to 40 bases upstream and 32 bases downstream of the first methionine (AUG), 72 nt in total.</li>
	<li>Custom order the designed BDs in SINEUP expression vector (see Table of Materials). 
	NOTE: Check the sequence specificity by basic local alignment search tool (BLAST) to avoid off-target effects26.</li>
</ol>
2. Cell Culture and SINEUP Transfection
<ol>
	<li>Seed cells of interest in a 6 well-plate or 24 well-plate for 24 h before transfection of SINEUPs. In the case of human embryonic kidney cell line (HEK293T/17) (see Table of Materials), seed 0.5 x 106 cells per well of a 6 well-plate or 1.5 x 105 cells per well of a poly-D-lysine coated 24 well-plate (see Table of Materials). It becomes 70% confluent after 24 h.</li>
	<li>After 24 h, change the medium to 1.5 mL of fresh medium for a 6 well-plate or 0.4 mL of fresh medium for a 24 well-plate. In case of SINEUP-GFP, transfect 0.6 &#181;g of pEGFP-C2 (see Table of Materials) and 3.4 &#181;g of SINEUP-GFP in one well of a 6 well-plate or 130 ng of pEGFP-C2 and 670 ng of SINEUP-GFP in one well of a 24 well-plate with transfection reagent (10 &#181;L in 6 well-plate and 3 &#181;L in 24 well-plate) by following the manufacturer&#8217;s instructions (see Table of Materials), and incubate at 37 &#176;C in a 5% CO2 incubator for 24 h.</li>
	<li>Wash cells with 2 mL of phosphate buffer saline (PBS) (37 mM NaCl, 8 mM Na2HPO4, 2.6 mM KCl and 1.5 mM KH2PO4) in each well of a 6 well-plate or 0.5 mL of PBS in each well of a 24 well-plate. Only for poly-D-lysine coated 24 well-plate, add 25 &#181;L of 0.05% weight per volume Trypsin, incubate in a 5% CO2 incubator for 5 min and add 275 &#181;L of cell medium per well. In case of 6 well-plate, add 2 mL of PBS in each well. Pipet up and down to harvest 3/4 of cells (1.5 mL for a 6 well-plate or 225 &#181;L for a 24 well-plate) from 1 well for protein extraction (go to protocol 3 for protein extraction) and 1/4 of cells (0.5 mL for a 6 well-plate or 75 &#181;L for a 24 well-plate) for RNA extraction and&#160; centrifuge at 6,000 x g for 5 min at 4 &#176;C (go to step 5 for RNA extraction). 
	NOTE:&#160;Analyze the effect of SINEUP-GFP in a poly-D-lysine coated 24 well-plate by imaging. Go to step 7 (imaging analysis).</li>
</ol>
3. Protein Extraction
<ol>
	<li>Carefully aspirate 1.5 mL of PBS and add 140 &#181;L of lysis solution (20 mM Tris-HCl (pH 7.5), 150 mM NaCl, 1 mM Na2EDTA, 1 mM EGTA, 1% (w/v) Triton, 2.5 mM sodium pyrophosphate, 1 mM &#946;-glycerophosphate, 1 mM Na3VO4, 1 &#956;g/mL leupeptin, and 0.005% (w/v) phenylmethylsulfonyl fluoride (PMSF)) (see Table of Materials) for a 6 well-plate or 60 &#181;L for a 24 well-plate to the cell pellets.</li>
	<li>Mix by pipetting and then mix thoroughly by rotating at slow speed for 1 h at 4 &#176;C. Collect supernatant by centrifugation at 14,000 x g for 10 min at 4 &#176;C.</li>
	<li>Check protein concentration by colorimetric assay (see Table of Materials). Prepare all the reactions at room temperature.
	<ol>
		<li>Prepare 5-6 times dilution of bovine serum albumin (BSA) protein standard in ultrapure water with concentrations ranging from 0.2-1.5 mg/mL protein. Prepare fresh standards each time.</li>
		<li>Prepare working reagent A&#697; by mixing 1 mL of reagent A (alkaline copper tartrate solution) with 20 &#181;L of reagent S (surfactant solution).</li>
		<li>Load 5 &#181;L of water (negative control), BSA standard (protein standard and positive control) or protein sample in each well of a 96-well-plate.</li>
		<li>Add 25 &#181;L of reagent A&#697; in each well. Carefully add 200 &#181;L of reagent B (Folin reagent) per well avoiding any bubble formation. Cover the plate with aluminum foil and wait for 5-10 min.</li>
		<li>Measure the protein absorbance at 750 nm with a spectrophotometer. The absorbance is stable for at least 1 h.</li>
		<li>Prepare standard curve by plotting BSA standard protein concentrations (mg/mL) on the x-axis and their respective absorbance on the y-axis. Calculate sample protein concentration by applying standard curve equation. 
		NOTE: Pause the protocol at this step if needed or go to step 4. For long-term storage, snap freeze protein samples in liquid nitrogen and store at -80 &#176;C.</li>
	</ol>
	</li>
</ol>
4. Protein Separation by SDS-PAGE and Detection of Target Proteins with Antibodies (Western-blot Analysis)
<ol>
	<li>Add one volume of 2x loading dye (0.1 M Tris-HCl (pH 6.8), 4% SDS, 20% glycerol, 1.42% 2-mercaptethanol and 0.2% bromophenol blue) to each volume of protein sample from step 3.3. Heat at 90 &#176;C for 5 min and immediately cool on ice for 1 min.</li>
	<li>Load 10-20 &#181;g of protein samples to 10% SDS poly-acrylamide gel and separate at 100-150 V) (see Table of Materials).</li>
	<li>Transfer protein from gel to 0.45-&#181;m nitrocellulose membrane (see Table of Materials) by semi-dry transfer instrument with transfer buffer (25 mM Tris, 192 mM glycine and 20% methanol) at 25 V for 30 min.</li>
	<li>Add blocking solution (5% non-fat dry milk in 1x TBST buffer (137 mM NaCl, 20 mM Tris-HCl (pH 7.6), 0.1% Tween-20)) (see Table of Materials) to the container until the membrane is completely soaked and incubate it at room temperature for 30 min.</li>
	<li>In the case of SINEUP-GFP, hybridize the protein with anti-GFP antibody (diluted 1:2000 in blocking solution) (see Table of Materials) by incubating the membrane for 30 min with shaking at room temperature. As an internal control protein, detect &#946;-actin protein by hybridizing with Anti-&#946;-Actin antibody (diluted 1:2000 in blocking solution) (see Table of Materials) for 30 min with shaking at room temperature.</li>
	<li>Add 1x TBST buffer to the container until the membrane is completely soaked and wash for 5 min at room temperature. Repeat the wash step two more times (a total of three washes).</li>
	<li>Hybridize GFP protein to diluted (1:1000 in blocking solution) anti-rabbit antibody conjugated with horseradish peroxidase (HRP), and hybridize &#946;-actin protein to diluted (1:1000 in blocking solution) anti-mouse antibody conjugated with HRP on the membrane for 30 min with shaking at room temperature.</li>
	<li>Wash membrane with 1x TBST buffer for 5 min at room temperature. Repeat the wash step two more times (a total of three washes).</li>
	<li>Mix equal volume of HRP-enhanced chemiluminescence (ECL) detection reagent 1 and 2 (see Table of Materials). Transfer the membrane to 2 mL ECL reagent mix, cover the box with aluminum foil and let it incubate for 1-2 min at room temperature. Carefully remove the membrane from ECL reagent mix and expose using a luminescence imaging instrument.</li>
</ol>
5. RNA Extraction and DNase Treatment
<ol>
	<li>Extract total RNA following the standard protocol for RNA extraction from cells grown in a monolayer27 or alternatively use a commercially available RNA extraction kit (see Table of Materials). To state in brief, add any monophasic lysis reagent (MLR) of guanidine isothiocyanate and phenol to the harvested cells in step 2.3 (1 mL MLR per ~5 million cells)27. 
	NOTE: Change gloves frequently. Use RNase-free reagents, and diethylpyrocarbonate (DEPC)-treated plastic ware and glassware to prevent RNA degradation. Pause the protocol at this step if needed. Store extracted RNA at -80 &#176;C.</li>
	<li>Add 0.1 volume of 10x DNase buffer and 2 U of DNase to the purified RNA from step 5.1 (see Table of Materials).</li>
	<li>Set the reaction volume to 50 &#181;L with nuclease-free water and mix gently. Incubate at 37 &#176;C for 30 min.</li>
	<li>Add 0.1 volume of re-suspended DNase inactivation reagent and mix well (see Table of Materials). Incubate for 5 min at room temperature with gentle shaking.</li>
	<li>Centrifuge at 10,000 x g for 90 s. Transfer the supernatant (DNA-free RNA) to a fresh RNase-free 1.5 mL tube. Be careful not to touch the pellet because this can cause carry-over of DNase which is troublesome for downstream steps.</li>
	<li>Quantitate RNA by measuring A260 and A260/A280 ratio (for pure RNA, the range is 1.8-2.0) in a UV spectrophotometer.</li>
</ol>
6. First Strand cDNA Synthesis and qRT-PCR Analysis
<ol>
	<li>Perform first strand cDNA synthesis following a standard cDNA synthesis protocol as below (see Table of Materials).
	<ol>
		<li>Mix 0.75 &#181;M oligo dT primer, 4.3 &#181;M random primer, dNTPs (10 mM each) with 200-500 ng total RNA (from steps 5-8) in 10 &#181;L of total reaction volume. Incubate at 65 &#176;C for 5 min and then immediately put on ice.</li>
		<li>Mix 1x reverse transcriptase buffer, 1 U of RNase inhibitor, 10 U of reverse transcriptase, and add to 10 &#181;L RNA-primer mix from 6.1.1.</li>
		<li>Set the total reaction volume to 20 &#181;L with nuclease-free water if required. Mix gently and incubate the reaction mix at 30 &#176;C for 10 min, then at 42 &#176;C for 60 min, and finally at 95 &#176;C for 5 min to inactivate the enzyme. Cool the tubes on ice. 
		NOTE: Thaw RNA samples and all the reagents on ice and prepare the reaction mix on ice. If target RNAs are only polyA RNAs, use oligo dT primer only (2.5 &#181;M). Pause the protocol if needed. Store synthesized cDNA at -20 &#176;C.</li>
	</ol>
	</li>
	<li>Perform qRT-PCR in technical triplicates (n=3, C&#1090; standard deviation &#62; 0.2) and within biological replicates (n &#8805; 3) using 1 &#181;L of 10 ng cDNA, 0.4 &#181;L of reverse primer (10 &#181;M), 0.4 &#181;L of forward primer (10 &#181;M), 10 &#181;L of mixture solution of DNA polymerase, 0.4 &#181;L of double-strand DNA staining dye, 10 &#181;L of nuclease-free water (reaction volume was 20 &#181;L) to detect PCR products using following conditions; hold stage (1 cycle) for 30 s at 95 &#176;C, cycling stage (40 cycles) for 5 s at 95 &#176;C and for 30 s at 60 &#176;C, melt curve stage. Primer examples are for Human Gapdh_Fw: TCTCTGCTCCTCCTGTTC, Human Gapdh_Rv: GCCCAATACGACCAAATCC, EGFP_Fw: GCCCGACAACCACTACCTGAG, EGFP_Rv: CGGCGGTCACGAACTCCAG, SINEUP-GFP_Fw: CTGGTGTGTATTATCTCTTATG and SINEUP-GFP_Rv: CTCCCGAGTCTCTGTAGC. See Table of Materials. Analyze quantitative RNA expression with 2-&#8710;&#8710;Ct &#177; SD method28.</li>
</ol>
7. Imaging Analysis of SINEUPs by Semi-automated Detection Method
<ol>
	<li>Wash cells with 0.5 mL of PBS for one well of a 24 well-plate.</li>
	<li>Add 2.0 &#956;g of Hoechst 33342 (see Table of Materials) (dissolving in 500 &#956;L of PBS) to each well of the 24-well-plate and incubate cells at 37 &#176;C for 20 min to stain the nucleus.</li>
	<li>Measure Hoechst stained cells to count the total number of cells at a blue emission maximum of 461 nm, and intensity of green fluorescence to count number of GFP positive cells at a green emission maximum of 510 nm by using a high-throughput micro-well image cytometer (see Table of Materials). Analyze protein up-regulatory effect of the SINEUPs by calculating GFP integrated intensity, which is the sum of all pixel intensities displaying signal in segmented objects calculated for each channel, using Imaging software29.</li>
	<li>Harvest cells to check RNA expression (back to steps 5 and 6).</li>
</ol>

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The corresponding author Piero Carninci is one of the founders of TransSINE Technologies Co. Ltd. that holds intellectual property on filed patent (EP2691522A4 and JP2017169573A), and granted patent (US9353370B2) for SINEUP technology.

We described here a protocol to specifically enhance protein production of a target mRNA by means of a SINE-containing non-coding RNA, called SINEUPs. As a representative example, optimum synthetic SINEUP-GFP is shown to up-regulate the translation of GFP mRNA 2.6-fold as measured by Western-blot analysis.
Designing an optimum BD is crucial to ensure SINEUP specificity and potency (extent of protein up-regulation). Previously, we screened 17 BDs of SINEUP-GFP by Western-blot analysis15 and found that the optimum BD overlaps the AUG-KOZAK sequence of GFP mRNA, though it may not be the case with other mRNAs and should be verified for each case. Another independent group also screened the BD using a different method31. As screening many BDs can be quite time-consuming and cumbersome, we introduced a high-throughput SINEUP detection method here. This method measures relative changes in GFP integrated density in SINEUP transfected-cells compared to the control vector transfected-cells. To ensure that cells in a particular well of a culture plate are transfected equally and GFP signal is not concentrated to only a certain region of the well, it is very important to distribute the cells equally in the wells in step 2.1. For this purpose, gently shake the plate 10 times back and forth (&#8593;&#8595;) after seeding the cells inside a clean bench and repeat in the 5% CO2 incubator before starting the incubation.
Another critical step is the calculation of protein concentration in step 3.3. Miscalculations here can lead to the loading of an erroneous amount of protein during Western-blot analysis, consequently preventing detection of small changes in protein expression by some of the weak SINEUPs or generating false positives from overloading. It is recommended to freshly prepare the protein standard curve every time, making sure that equal amounts of standards and protein samples are measured in step 3.3.3. The protocol described here focuses on SINEUP-GFP, but Western-blot analysis can be used for any target mRNA of interest. The incubation time and concentration of antibodies should be optimized for each target to get the best result.
One of the unique features of SINEUPs is that target-mRNA expression level remains unaffected. It is important to treat RNA with DNase to avoid detection of transfected SINEUPs and genomic DNA by qRT-PCR. SINEUP RNAs and target mRNA expression should be measured by qRT-PCR to confirm the success of both transfection and SINEUP activity. SINEUPs contain a SINE sequence, which is abundant throughout both the human and mouse genomes. To avoid non-specific detection of SINE sequences, it is not recommended to design qRT-PCR primers to the SINE sequence.
In this protocol we used human cell lines, but SINEUPs are efficacious in a number of cell lines from several different species12,13,14,18,19. The cell culture and transfection conditions can be modified according to different cell lines as long as these maintain transfection efficiency of the SINEUP vectors. Moreover, alternative methods of RNA extraction, cDNA synthesis, and protein concentration checking can be employed, given that they preserve the required RNA and protein quality for qRT-PCR and Western-blot analysis. While we used a specific high-throughput micro-well cytometer, which enabled detection of GFP fluorescence across the entire well, other cytometers with a similar detection range can be used31. It is to be noted that if the distribution of cells and transfection are equal throughout a well, then it is not necessary to scan the whole well for GFP fluorescence: half or one-quarter of the area of a well might be enough to discern SINEUP effect depending on experimental skills.
Establishing a high-throughput SINEUP detection protocol allows for simultaneous screening of multiple BDs targeting a given mRNA in cultured cells. This is important as the rules governing optimum targeting by the BD are still unclear. Such a multiplex screening system allows for large-scale testing of many SINEUPs against different genes, useful for targeting multiple genes involved in a particular signaling pathway for instance. Furthermore, it can be utilized to expand the search for effective SINEUPs targeting several mRNAs, designing different SINEUP BDs around AUG-Kozak region (see Figure 1), co-transfecting full length target mRNAs (5&#697; UTR-CDS-3&#697; UTR) fused with GFP mRNA in cultured cells to find the optimum SINEUPs, and subsequently testing BD candidates against endogenous mRNA in cultured cells and in vivo model animals, from humans and mice to other animal and plant species.
This screening protocol is very fast. We do not need to fix and collect cells, but just need to place the living cell culture plate in the imaging instrument. We propose to use this high-throughput screening protocol to select optimum BDs of SINEUPs and evaluate potential candidates by Western-blot analysis. Thus, selected candidates with optimum BDs can be applied to increase antibody production18,19,21. Currently, the RNA therapeutic field is dramatically growing. For instance, siRNA, ASO, mRNA, and CRISPR RNA therapies, are widely employed to control mRNA expression of their respective targets9,32. In this context, SINEUPs are in their infancy, but so far none of the studied SINEUPs changed expression of target mRNAs. In addition, SINEUPs do not edit target mRNA, but only up-regulate translation of mRNA. Furthermore, loss-of-function diseases resulting from haploinsufficiency can be targeted by SINEUP therapy, achieving a 2-fold induction of the deficient protein17,33. Although off-target effects need to be further studied, SINEUPs potentially and specifically target a single, expressed mRNA with a complementary sequence to the BD.
A limitation of this high-throughput protocol is that it is not suitable to screen BDs of SINEUPs in in vivo mouse models because the protocol measures the GFP integrated intensity only. As SINEUPs are natural antisense lncRNAs that act post-transcriptionally, they cannot be applied when the target mRNA is missing in the cells or tissue samples.
Nevertheless, SINEUPs can be applied to gain-of-function studies, to enhance antibody production, and as an RNA therapy to up-regulate expression of deficient proteins within the range of 1.5-3.0-fold. The methods described here present a useful guide to target and detect SINEUP-induced translation enhancement of desired mRNA and provide a new tool for post-transcriptional gene regulation.

In the post-genomic era, many insights have been gained into the gene regulatory roles of non-coding antisense transcripts owing to the development of next-generation sequencing technologies1,2,3 and gene-editing tools. This category of transcripts, which was previously considered to be &#34;transcriptional trash&#34;, is now established as a key player of genetic regulation. Antisense transcripts are reported to modulate chromatin and control stability and expression of their cognate protein-coding sense mRNA4,5. In most cases, this mode of regulation is negative and antisense transcripts silence their sense counterparts through RNA-RNA interactions6,7. This trait of natural antisense transcripts has been utilized to downregulate desired genes in the form of synthetic small interfering RNA (siRNA), microRNA (miRNA), and antisense oligos (ASO)8,9,10,11 leaving a technological void for targeted gene up-regulation.
One intriguing study changed the perspective of the antisense RNA field by demonstrating that antisense long non-coding RNAs (AS lncRNAs) of the genes Uchl1 (ubiquitin C-terminal hydrolase L1) and Uxt (ubiquitously-expressed transcript) positively regulate translation of their cognate sense mRNA at the post-transcriptional level in mice12. The 5&#697; end of these AS lncRNAs overlaps with several bases in the 5&#697; untranslated region (5&#697; UTR) of their corresponding sense transcripts, and the non-overlapping 3&#697; end contains an inverted repeat of a retrotransposon belonging to the short interspersed nuclear element (SINE) family. Interestingly, we found that the main driving force behind this translational up-regulation is the embedded SINE repeat and it is not limited to mouse SINE repeats only. Human Alu repeat-containing AS lncRNAs also enhanced translation of target sense mRNAs, reinforcing the idea of a novel class of SINE-driven regulatory antisense non-coding RNAs, appropriately named SINEUPs13. Recent studies showed that the potential of natural SINEUPs is preserved in synthetic SINEUPs designed to specifically target various endogenous and exogenous genes14,15. SINEUPs have two important features: first the &#34;binding domain&#34; (BD) which is generally the 5&#697; end region complementary to the sequence encompassing the primary start codon of a protein-coding mRNA, and second the &#34;effector domain&#34; (ED) as it incorporates an inverted repeat of SINE which is a prerequisite for SINEUP function14 (Figure 1). SINEUPs can be customized to design a BD specifically targeting a gene of choice. This can then be harnessed to dissect the function of a particular gene involved in a biological pathway, as a better alternative to a conventional mRNA overexpression strategy. In addition, this versatile tool can be applied to boost antibody production, and as a drug to treat haploinsufficient diseases caused by insufficient dosages of functional proteins16,17,18,19,20,21.
The advantages of SINEUP technology are manifold. It does not alter the expression of the target at the transcriptional level. Longer BDs provide more specificity to SINEUPs, while not inducing a dsRNA-dependent stress response15. The protein induction is maintained within the normal physiological range of the cell, preventing any deleterious effect due to aberrant or excessive protein expression. SINEUPs are compatible with a wide variety of mouse, human, and hamster cultured cell lines, for instance, HEK293T/17, HepG2, HeLa, CHO, MN9D, and many more12,13,14,15,18,19. SINEUPs can efficiently target endogenous genes, transiently overexpressed genes, and FLAG-tagged or luciferase-fusion genes, eliminating the need of gene-specific antibodies14,18. The basic SINEUP analysis requires routine cell culture, transfection, sodium dodecyl sulfate-polyacrylamide gel electrophoresis (SDS-PAGE), real time quantitative reverse transcription-polymerase chain reaction (qRT-PCR) instruments and settings, and expertise can be gained in a short time.
Here, we describe a method for targeting genes with synthetic SINEUPs to up-regulate translation, an effect contrary to other technologies such as RNA interference9 and ASO gapmers11,22,23. A widely-used method for RNA-guided gene activation is clustered regularly interspaced short palindromic repeats-based activation (CRISPRa), where the gene expression is triggered at the transcriptional level24. This method, though simple and fast, requires multiple single guide RNAs (sgRNAs) targeting the same gene for higher efficiency, thereby increasing the chances of off-target binding25. In addition, the key enzyme of the CRISPRa system, the catalytically dead CRISPR-associated protein 9 (dCas9) has low binding specificity and sgRNAs targeting bi-directional promoter regions can non-specifically up-regulate nearby genes25. Conversely, SINEUPs bind to target mRNA at a single binding region with high specificity and do not affect expression of nearby genes. We discuss the basic steps involved in SINEUP design, transfection, protein and RNA expression analyses. Furthermore, we present a semi-automated, high-throughput imaging system to screen multiple SINEUPs at once, which is useful for detection of optimum SINEUPs.

<table><tbody><tr><td>Synthetic SINEUP</td><td>Cell Guidance Systems Ltd. in UK and K.K.DNAFORM in Japan</td><td>https://www.cellgs.com/items/sineupand8482.html and https://www.dnaform.jp/en/information/20130320</td><td>Step 1.5</td></tr><tr><td>HEK293T/17</td><td>ATCC</td><td>ATCC CRL-11268</td><td>Step 2.1</td></tr><tr><td>Falcon Multiwell Plate For Cell Culture 6 well plate</td><td>Corning</td><td>6902A01</td><td>Step 2.1</td></tr><tr><td>Corning BioCoat Poly-D-Lysine 24 well Plate</td><td>Corning</td><td>08-774-124</td><td>Step 2.1</td></tr><tr><td>Lipofectamine 2000 Transfection Reagent</td><td>Thermo Fisher Scientific</td><td>11668027</td><td>Step 2.2</td></tr><tr><td>pEGFP-C2</td><td>Clontech</td><td>#6083-1</td><td>Step 2.2</td></tr><tr><td>Cell Lysis Buffer (10x)</td><td>Cell Signaling Technology</td><td>#9803S</td><td>Step 3.1 This is pre-mixed cell lysis solution.</td></tr><tr><td>PMSF</td><td>Cell Signaling Technology</td><td>#8553S</td><td>Step 3.1 To complete cell lysis buffer, add 0.005% (w/v) PMSF to 1x cell lysis buffer.</td></tr><tr><td>DC protein assay kit II</td><td>BIO RAD</td><td>#5000112JA</td><td>Step 3.3</td></tr><tr><td>10% Mini-PROTEAN TGX Precast Protein Gels, 12-well, 20 &amp;micro;L</td><td>BIO RAD</td><td>#4561035</td><td>Step 4.2</td></tr><tr><td>Amersham Protran Premium NC 0.45 (150 mm&amp;times;4 m)</td><td>Amasham</td><td>10600013</td><td>Step 4.3, This is a 0.45 &amp;micro;m nitrocellulose membrane.</td></tr><tr><td>Nonfat Dry Milk</td><td>Cell Signaling Technology</td><td>#9999S</td><td>Step 4.4 A component of the blocking solution.</td></tr><tr><td>GFP Tag Antibody</td><td>Thermo Fisher Scientific</td><td>A-6455</td><td>Step 4.5 Lot number: 1495850, RRID: AB_221570</td></tr><tr><td>Monoclonal Anti-&amp;beta;-Actin antibody produced in mouse</td><td>SIGMA</td><td>A5441</td><td>Step 4.5 Lot number: 026M4780V, RRID: AB_476744</td></tr><tr><td>Polyclonal Goat Anti Rabbit Immunoglobulins</td><td>Dako</td><td>P0448</td><td>Step 4.5 This is secondary antibody conjugating with HRP for anti GFP antibody. Lot number: 20017525, RRID:AB_2617138</td></tr><tr><td>Polyclonal Goat Anti mouse Immunoglobulins</td><td>Dako</td><td>P0447</td><td>Step 4.5 This is secondary antibody conjugating with HRP for anti &amp;beta;-Actin antibody. Lot number: 20019698, RRID:AB_2617137</td></tr><tr><td>ECL Western Blotting Detection Reagents</td><td>Amersham</td><td>RPN2109</td><td>Step 4.9</td></tr><tr><td>Maxwell Rapid Sample Concentrator (RSC) Instrument</td><td>Promega</td><td>AS4500</td><td>Step 5.1 This is commercially available RNA exreaction instrument.</td></tr><tr><td>Maxwell RSC simplyRNA Cells Kit</td><td>Promega</td><td>AS1390</td><td>Step 5.1 This is commercially available RNA exreaction kit.</td></tr><tr><td>TURBO DNA-free Kit</td><td>ambion</td><td>AM1907</td><td>Step 5.2 and 5.4 The kit contains DNase, DNase buffer and inactivation reagent.</td></tr><tr><td>PrimeScrip 1st strand cDNA Synthesis Kit</td><td>TaKaRa</td><td>6110A</td><td>Step 6.1 The kit contains reagents of first strand cDNA synthesis.</td></tr><tr><td>TB Green Premix Ex Taq II</td><td>TaKaRa</td><td>RR820A</td><td>Step 6.2</td></tr><tr><td>Hoechst3342</td><td>Thermo Fisher Scientific</td><td>H3570</td><td>Step 7.2</td></tr><tr><td>Celigo S</td><td>Nexcelom Bioscience</td><td>200-BFFL-S</td><td>Step 7.3 This is a high throughput micro-well image cytometer.</td></tr></tbody></table>

cell based assays of sineup non-coding rnas that can specifically enhance mrna translation

Targeted-protein enhancement is of importance not only for the study of biological processes but also for therapeutic and biotechnological applications. Here, we present a method to selectively up-regulate protein expression of desired genes in cultured cells by means of synthetic antisense non-coding RNAs known as SINEUPs. This positive control of gene expression is at the post-transcriptional level and exerted by an inverted short interspersed nuclear element (SINE) repeat at the 3&#697; end of SINEUPs that comprises its effector domain (ED). SINEUPs can specifically bind to any protein-coding mRNA of choice through its binding domain (BD), a region designed to complement the sequence within the 5&#697; untranslated region (5&#697; UTR) and around the start codon of the mRNA. Target-specific SINEUPs designed in this manner are transfected to cultured cells, and protein and RNA are extracted for downstream analyses, generally 24-48 h post-transfection. SINEUP-induced protein up-regulation is detected by Western-blot analysis and RNA expression is measured using real-time quantitative reverse transcription PCR. We have observed that BD design is critical for achieving optimum SINEUP activity and that testing different BD sizes and positions with respect to the start codon of the target mRNA is recommended. Therefore, we describe here a semi-automated high-throughput imaging method based on fluorescence detection that can be implemented to target mRNA fused with green fluorescent protein (GFP). SINEUPs specifically enhance translation within normal physiological range of the cell, without altering the target transcript level. This method has been successfully employed against a range of endogenous and exogenous targets, in a wide variety of human, mouse, and insect cell lines along with in vivo systems. Moreover, SINEUPs have been reported to increase antibody production and work as an RNA therapeutic against haploinsufficient genes. The versatile and modular nature of SINEUPs makes them a suitable tool for gene-specific translational control.

SINEUP-GFP is a synthetic SINEUP containing both an optimum BD (-28/+4 overlap to GFP mRNA) and an ED (inverted SINE B2 from AS-Uchl1) that can up-regulate GFP mRNA translation (Figure 3A and 3B) without changing the expression of GFP mRNA (Figure 3C and 3D). To screen optimum BDs and EDs for SINEUPs, we developed a protocol of semi-automated image analysis that improved detection time and increased the number of samples being simultaneously screened compared with a conventional Western-blot analysis15. As shown in Figure 4, this high-throughput imaging system took 3 days (Western-blot analysis took 2 weeks for 48 SINEUPs). Having demonstrated that SINEUP-GFP increases GFP translation, we detected GFP integrated intensity by the image cytometer. The optimum BD of SINEUP-GFP induced a 1.4-fold increase in GFP protein expression. Although we observed compression of signals from 2.6-fold (Western-blot analysis, see Figure 3A) to 1.4-fold (Imaging analysis, see Figure 5), the difference might be due to the calibration of the imaging instrument software. Nevertheless, we detected significantly higher levels of GFP fluorescence compared with the control (Figure 5A and 5B).
<img alt="Figure 1" class="xfigimg" src="/files/ftp_upload/58627/58627fig1.jpg" /> 
Figure 1: Basic design of the synthetic SINEUPs. BD = binding domain to target mRNA, ED = effector domain containing an inverted SINE sequence. <a href="https://www.jove.com/files/ftp_upload/58627/58627fig1large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 2" class="xfigimg" src="/files/ftp_upload/58627/58627fig2.jpg" /> 
Figure 2: Transcription starting sites (TSSs) of human Parkinson disease protein 7 (PARK7) mRNA in specific tissues and cells as detected by CAGE analysis. (A) A snapshot showing a TSS search result for human PARK7 mRNA using an omics data integration and interactive visualization system30. The horizontal green arrow in the Entrez gene hg19 track indicates the genomic position of the reference human PARK7 mRNA and the vertical green bars in the FANTOM5 CAGE 1 and 2 tracks indicate the sum of TSSs (measured as transcripts per million (tpm)) from 1,829 types of tissues and cells. (B) Zoom in of the marked region of the TSS in panel A (1/354 scale: 35.4 kb to 100 bp). Grey shaded area in the FANTOM5 CAGE phase 1 and 2 tracks indicates the TSS of 6 specific cells out of the total 1,829, which are listed at the bottom of the figure. The numbers (11.369, 4.998, 4.304, 3.509, 3.477, and 3.055) corresponding to these listed cells indicate transcripts per million for each specific cell at the grey shaded positions of the TSS. <a href="https://www.jove.com/files/ftp_upload/58627/58627fig2large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 3" class="xfigimg" src="/files/ftp_upload/58627/58627fig3.jpg" /> 
Figure 3: Western-blot analysis confirming up-regulation of translation by SINEUP-GFP. (A) SINEUP-GFP was examined by Western-blot with anti-GFP antibody. (B) Results were normalized to the intensity of the &#946;-actin protein band. (C) GFP mRNA and (D) SINEUP RNAs expression were detected by qRT-PCR. ***p &#60; 0.0005, n = 3, two-tailed student&#39;s t-test, error bars are standard deviation. This figure has been modified from Takahashi et al.15. <a href="https://www.jove.com/files/ftp_upload/58627/58627fig3large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 4" class="xfigimg" src="/files/ftp_upload/58627/58627fig4.jpg" /> 
Figure 4: Schematic of SINEUP semi-automated image analysis. Day 1: Seed cells of interest in a 24 well-plate. Day 2: Transfect GFP and SINEUP-GFP. Day 3: Analyze the effect of SINEUPs by measuring GFP integrated intensity. <a href="https://www.jove.com/files/ftp_upload/58627/58627fig4large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 5" class="xfigimg" src="/files/ftp_upload/58627/58627fig5.jpg" /> 
Figure 5: High-throughput analysis of translation up-regulation by SINEUP-GFP. (A) Comparison of GFP fluorescence between control and SINEUP-GFP transfected cells15. Scale bar = 2 mm. (B) GFP integrated intensity was normalized to the total cell number counted by nuclear staining with Hoechst 33342. ***p &#60; 0.0005, n = 3, two-tailed student&#39;s t-test, error bars are standard deviation. FOV: field of view. This figure has been modified from Takahashi et al.15. <a href="https://www.jove.com/files/ftp_upload/58627/58627fig5large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>

Watch this Scientific Journal Video about Cell Based Assays of SINEUP Non-coding RNAs That Can Specifically Enhance mRNA Translation at JoVE.com

Cell Based Assays of SINEUP Non-coding RNAs That Can Specifically Enhance mRNA Translation

SINEUPs are synthetic antisense non-coding RNAs, which contain a binding domain (BD) and an effector domain (ED) and up-regulate translation of target mRNA. Here, we describe detection methods for SINEUPs in cultured cell lines, analysis of their translation-promoting activity by Western-blot and a semi-automated high throughput imaging system.

Targeted-protein enhancement is of importance not only for the study of biological processes but also for therapeutic and biotechnological applications. ...

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Genetics

8.3K Views.  RIKEN Center for Integrative Medical Sciences. SINEUPs are synthetic antisense non-coding RNAs, which contain a binding domain (BD) and an effector domain (ED) and up-regulate translation of target mRNA. Here, we describe detection methods for SINEUPs in cultured cell lines, analysis of their translation-promoting activity by Western-blot and a semi-automated high throughput imaging system.

Video: Cell Based Assays of SINEUP Non-coding RNAs That Can Specifically Enhance mRNA Translation

Quantitative Immunofluorescence to Measure Global Localized Translation

The mechanisms regulating mRNA translation are involved in various biological processes, such as germ line development, cell differentiation, and organogenesis, as well as in multiple diseases. Numerous publications have convincingly shown that specific mechanisms tightly regulate mRNA translation. Increased interest in the translation-induced regulation of protein expression has led to the development of novel methods to study and follow de novo protein synthesis in cellulo. However, most of these methods are complex, making them costly and often limiting the number of mRNA targets that can be studied. This manuscript proposes a method that requires only basic reagents and a confocal fluorescence imaging system to measure and visualize the changes in mRNA translation that occur in any cell line under various conditions. This method was recently used to show localized translation in the subcellular structures of adherent cells over a short period of time, thus offering the possibility of visualizing de novo translation for a short period during a variety of biological processes or of validating changes in translational activity in response to specific stimuli.

This manuscript describes a method to visualize and quantify localized translation events in subcellular compartments. The approach proposed in this manuscript requires a basic confocal imaging system and reagents and is rapid and cost-effective.

The mechanisms regulating mRNA translation are involved in various biological processes, such as germ line development, cell differentiation, and ...

Biochemistry

Biotin-based Pulldown Assay to Validate mRNA Targets of Cellular miRNAs

MicroRNAs (miRNAs) are a class of small noncoding RNAs that post-transcriptionally regulate cellular gene expression. MiRNAs bind to the 3&#39; untranslated region (UTR) of target mRNA to inhibit protein translation or in some instances cause mRNA degradation. The binding of the miRNA to the 3&#39; UTR of the target mRNA is mediated by a 2&#8211;8 nucleotide seed sequence at the 5&#39; end of miRNA. While the role of miRNAs as cellular regulatory molecules is well established, identification of the target mRNAs with functional relevance remains a challenge. Bioinformatic tools have been employed to predict sequences within the 3&#39; UTR of mRNAs as potential targets for miRNA binding. These tools have also been utilized to determine the evolutionary conservation of such sequences among related species in an attempt to predict functional role. However, these computational methods often generate false positive results and are limited to predicting canonical interaction between miRNA and mRNA. Therefore, experimental procedures that measure direct binding of miRNA to its mRNA target are necessary to establish functional interaction. In this report, we describe a sensitive method for validating direct interaction between the cellular miRNA miR-125b and the 3&#39; UTR of PARP-1 mRNA. We elaborate a protocol in which synthetic biotinylated-miRNA mimics were transfected into mammalian cells and the miRNA-mRNA complex in the cellular lysate was pulled down with streptavidin-coated magnetic beads. Finally, the target mRNA in the pulled-down nucleic acid complex was quantified using a qPCR-based strategy.

This report describes a fast and reliable method for validating mRNA targets of cellular miRNAs. The method uses synthetic biotinylated Locked Nucleic Acid (LNA)-based miRNA mimics to capture target mRNA. Subsequently, streptavidin-coated magnetic beads are employed to pulldown the target mRNA for quantification by qPCR polymerase chain reaction.

MicroRNAs (miRNAs) are a class of small noncoding RNAs that post-transcriptionally regulate cellular gene expression. MiRNAs bind to the 3&#39; ...

Saccharomyces cerevisiae Metabolic Labeling with 4-thiouracil and the Quantification of Newly Synthesized mRNA As a Proxy for RNA Polymerase II Activity

Global defects in RNA polymerase II transcription might be overlooked by transcriptomic studies analyzing steady-state RNA. Indeed, the global decrease in mRNA synthesis has been shown to be compensated by a simultaneous decrease in mRNA degradation to restore normal steady-state levels. Hence, the genome-wide quantification of mRNA synthesis, independently from mRNA decay, is the best direct reflection of RNA polymerase II transcriptional activity. Here, we discuss a method using non-perturbing metabolic labeling of nascent RNAs in Saccharomyces cerevisiae (S. cerevisiae). Specifically, the cells are cultured for 6 min with a uracil analog, 4-thiouracil, and the labeled newly transcribed RNAs are purified and quantified to determine the synthesis rates of all individual mRNA. Moreover, using labeled Schizosaccharomyces pombe cells as internal standard allows comparing mRNA synthesis in different S. cerevisiae strains. Using this protocol and fitting the data with a dynamic kinetic model, the corresponding mRNA decay rates can be determined.

Saccharomyces cerevisiae Metabolic Labeling with 4-thiouracil and the Quantification of Newly Synthesized mRNA As a Proxy for RNA Polymerase II Activity

The protocol described here is based on the genome-wide quantification of newly synthesized mRNA purified from yeast cells labeled with 4-thiouracil. This method allows to measure mRNA synthesis uncoupled from mRNA decay and, thus, provides an accurate measurement of RNA polymerase II transcription.

Global defects in RNA polymerase II transcription might be overlooked by transcriptomic studies analyzing steady-state RNA. Indeed, the global decrease in ...

Enforced Activation of Enhancer RNAs In Situ through the dCas9 Synergistic Activation Mediator System

Enhancers are pivotal genomic elements scattered through the mammalian genome and dictate tissue-specific gene expression programs. Increasing evidence has shown that enhancers not only provide DNA binding motifs for transcription factors (TFs) but also generate non-coding RNAs that are referred to as eRNAs. Studies have demonstrated that eRNA transcripts can play significant roles in gene regulation in both physiology and disease. Commonly used methods to investigate the function of eRNAs are constrained to &#8220;loss-of-function&#8221; approaches by knockdown of eRNAs, or by chemical inhibition of the enhancer transcription. There has not been a robust method to conduct &#8220;gain-of-function&#8221; studies of eRNAs to mimic specific disease conditions such as human cancer, where eRNAs are often overexpressed. Here, we introduce a method for precisely and robustly activating eRNAs for functional interrogation of their roles by applying the dCas9 mediated Synergistic Activation Mediators (SAM) system. We present the entire workflow of eRNA activation, from the selection of eRNAs, the design of gRNAs to the validation of eRNA activation by RT-qPCR. This method represents a unique approach to study the roles of a particular eRNA in gene regulation and disease development. In addition, this system can be employed for unbiased CRISPR screening to identify phenotype-driving eRNA targets in the context of a specific disease.

Enhancer RNAs (eRNAs) are non-coding RNAs produced from active enhancers. An optimal approach to study eRNA functions is to manipulate their levels in the native chromatin regions. Here we introduce a robust system for eRNA studies by using CRISPR-dCas9-fused transcriptional activators to induce the expression of eRNAs of interest.

Enhancers are pivotal genomic elements scattered through the mammalian genome and dictate tissue-specific gene expression programs. Increasing evidence ...

An In Vitro Single-Molecule Imaging Assay for the Analysis of Cap-Dependent Translation Kinetics

Cap-dependent protein synthesis is the predominant translation pathway in eukaryotic cells. While various biochemical and genetic approaches have allowed extensive studies of cap-dependent translation and its regulation, high resolution kinetic characterization of this translation pathway is still lacking. Recently, we developed an in vitro assay to measure cap-dependent translation kinetics with single-molecule resolution. The assay is based on fluorescently labeled antibody binding to nascent epitope-tagged polypeptide. By imaging the binding and dissociation of antibodies to and from nascent peptide&#8211;ribosome&#8211;mRNA complexes, the translation progression on individual mRNAs can be tracked. Here, we present a protocol for establishing this assay, including mRNA and PEGylated slide preparations, real-time imaging of translation, and analysis of single molecule trajectories. This assay enables tracking of individual cap-dependent translation events and resolves key translation kinetics, such as initiation and elongation rates. The assay can be widely applied to distinct translation systems and should broadly benefit in vitro studies of cap-dependent translation kinetics and translational control mechanisms.

An In Vitro Single-Molecule Imaging Assay for the Analysis of Cap-Dependent Translation Kinetics

Tracking individual translation events allows for high-resolution kinetic studies of cap-dependent translation mechanisms. Here we demonstrate an in vitro single-molecule assay based on imaging interactions between fluorescently labeled antibodies and epitope-tagged nascent peptides. This method enables single-molecule characterization of initiation and peptide elongation kinetics during active in vitro cap-dependent translation.

Cap-dependent protein synthesis is the predominant translation pathway in eukaryotic cells. While various biochemical and genetic approaches have allowed ...

Real-Time Quantitative Measurement of Tumor Cell Migration and Invasion Following Synthetic mRNA Transfection

Tumor cells are highly motile and invasive and display altered gene expression patterns. Knowledge of how changes in gene expression regulate tumor cell migration and invasion is essential for understanding the mechanisms of tumor cell infiltration into neighboring healthy tissues and metastasis. Previously, it was demonstrated that gene knockdown followed by the impedance-based real-time measurement of tumor cell migration and invasion enables the identification of the genes required for tumor cell migration and invasion. Recently, the mRNA vaccines against SARS-CoV-2 have increased interest in using synthetic mRNA for therapeutic purposes. Here, the method using synthetic mRNA was revised to study the effect of gene overexpression on tumor cell migration and invasion. This study demonstrates that elevated gene expression with synthetic mRNA transfection followed by impedance-based real-time measurement may help identify the genes that stimulate tumor cell migration and invasion. This method paper provides important details on the procedures for examining the effect of altered gene expression on tumor cell migration and invasion.

Many upregulated genes stimulate tumor cell migration and invasion, leading to poor prognosis. Determining which genes regulate tumor cell migration and invasion is critical. This protocol presents a method for investigating the effects of the increased expression of a gene on the migration and invasion of tumor cells in real time.

Tumor cells are highly motile and invasive and display altered gene expression patterns. Knowledge of how changes in gene expression regulate tumor cell ...

Cancer Research

In Vitro Transcribed RNA-based Luciferase Reporter Assay to Study Translation Regulation in Poxvirus-infected Cells

Every poxvirus mRNA transcribed after viral DNA replication has an evolutionarily conserved, non-templated 5&#39;-poly(A) leader in the 5&#39;-UTR. To dissect the role of 5&#39;-poly(A) leader in mRNA translation during poxvirus infection we developed an in vitro transcribed RNA-based luciferase reporter assay. This reporter assay comprises of four core steps: (1) PCR to amplify the DNA template for in vitro transcription; (2) in vitro transcription to generate mRNA using T7 RNA polymerase; (3) Transfection to introduce in vitro transcribed mRNA into cells; (4) Detection of luciferase activity as the indicator of translation. The RNA-based luciferase reporter assay described here circumvents issues of plasmid replication in poxvirus-infected cells and cryptic transcription from the plasmid. This protocol can be used to determine translation regulation by cis-elements in an mRNA including 5&#39;-UTR and 3&#39;-UTR in systems other than poxvirus-infected cells. Moreover, different modes of translation initiation like cap-dependent, cap-independent, re-initiation, and internal initiation can be investigated using this method.

We present a protocol to study mRNA translation regulation in poxvirus-infected cells using in vitro Transcribed RNA-based luciferase reporter assay. The assay can be used for studying translation regulation by cis-elements of an mRNA, including 5&#8217;-untranslated region (UTR) and 3&#8217;-UTR. Different translation initiation modes can also be examined using this method.

Every poxvirus mRNA transcribed after viral DNA replication has an evolutionarily conserved, non-templated 5&#39;-poly(A) leader in the 5&#39;-UTR. To ...

Immunology and Infection

Polysome Fractionation and Analysis of Mammalian Translatomes on a Genome-wide Scale

mRNA translation plays a central role in the regulation of gene expression and represents the most energy consuming process in mammalian cells. Accordingly, dysregulation of mRNA translation is considered to play a major role in a variety of pathological states including cancer. Ribosomes also host chaperones, which facilitate folding of nascent polypeptides, thereby modulating function and stability of newly synthesized polypeptides. In addition, emerging data indicate that ribosomes serve as a platform for a repertoire of signaling molecules, which are implicated in a variety of post-translational modifications of newly synthesized polypeptides as they emerge from the ribosome, and/or components of translational machinery. Herein, a well-established method of ribosome fractionation using sucrose density gradient centrifugation is described. In conjunction with the in-house developed &#8220;anota&#8221; algorithm this method allows direct determination of differential translation of individual mRNAs on a genome-wide scale. Moreover, this versatile protocol can be used for a variety of biochemical studies aiming to dissect the function of ribosome-associated protein complexes, including those that play a central role in folding and degradation of newly synthesized polypeptides.

Ribosomes play a central role in protein synthesis. Polyribosome (polysome) fractionation by sucrose density gradient centrifugation allows direct determination of translation efficiencies of individual mRNAs on a genome-wide scale. In addition, this method can be used for biochemical analysis of ribosome- and polysome-associated factors such as chaperones and signaling molecules.

mRNA translation plays a central role in the regulation of gene expression and represents the most energy consuming process in mammalian cells. ...

Biology

Assessment of Selective mRNA Translation in Mammalian Cells by Polysome Profiling

Regulation of protein synthesis represents a key control point in cellular response to stress. In particular, discreet RNA regulatory elements were shown to allow to selective translation of specific mRNAs, which typically encode for proteins required for a particular stress response. Identification of these mRNAs, as well as the characterization of regulatory mechanisms responsible for selective translation has been at the forefront of molecular biology for some time. Polysome profiling is a cornerstone method in these studies. The goal of polysome profiling is to capture mRNA translation by immobilizing actively translating ribosomes on different transcripts and separate the resulting polyribosomes by ultracentrifugation on a sucrose gradient, thus allowing for a distinction between highly translated transcripts and poorly translated ones. These can then be further characterized by traditional biochemical and molecular biology methods. Importantly, combining polysome profiling with high throughput genomic approaches allows for a large scale analysis of translational regulation.

The ability of cells to adapt to stress is crucial for their survival. Regulation of mRNA translation is one such adaptation strategy, providing for rapid regulation of the proteome. Here, we provide a standardized polysome profiling protocol to identify specific mRNAs that are selectively translated under stress conditions.

Regulation of protein synthesis represents a key control point in cellular response to stress. In particular, discreet RNA regulatory elements were shown ...

High-throughput Screening for Chemical Modulators of Post-transcriptionally Regulated Genes

Both transcriptional and post-transcriptional regulation have a profound impact on genes expression. However, commonly adopted cell-based screening assays focus on transcriptional regulation, being essentially aimed at the identification of promoter-targeting molecules. As a result, post-transcriptional mechanisms are largely uncovered by gene expression targeted drug development. Here we describe a cell-based assay aimed at investigating the role of the 3&#39; untranslated region (3&#8217; UTR) in the modulation of the fate of its mRNA, and at identifying compounds able to modify it. The assay is based on the use of a luciferase reporter construct containing the 3&#8217; UTR of a gene of interest stably integrated into a disease-relevant cell line. The protocol is divided into two parts, with the initial focus on the primary screening aimed at the identification of molecules affecting luciferase activity after 24 hr of treatment. The second part of the protocol describes the counter-screening necessary to discriminate compounds modulating luciferase activity specifically through the 3&#8217; UTR. In addition to the detailed protocol and representative results, we provide important considerations about the assay development and the validation of the hit(s) on the endogenous target. The described cell-based reporter gene assay will allow scientists to identify molecules modulating protein levels via post-transcriptional mechanisms dependent on a 3&#8217; UTR.

Here we describe a cell-based reporter gene assay as a valuable tool to screen chemical libraries for compounds modulating post-transcriptional control mechanisms exerted through 3&#8217; UTR.

Both transcriptional and post-transcriptional regulation have a profound impact on genes expression. However, commonly adopted cell-based screening assays ...

Cell Based Assays of SINEUP Non-coding RNAs That Can Specifically Enhance mRNA Translation

Summary

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An In Vitro Single-Molecule Imaging Assay for the Analysis of Cap-Dependent Translation Kinetics

Real-Time Quantitative Measurement of Tumor Cell Migration and Invasion Following Synthetic mRNA Transfection

In Vitro Transcribed RNA-based Luciferase Reporter Assay to Study Translation Regulation in Poxvirus-infected Cells

Polysome Fractionation and Analysis of Mammalian Translatomes on a Genome-wide Scale

Assessment of Selective mRNA Translation in Mammalian Cells by Polysome Profiling

High-throughput Screening for Chemical Modulators of Post-transcriptionally Regulated Genes