Structural Characterization of DDX23 5’ UTR Regulatory Elements and Their Targeting by LNA-Modified Antisense Oligonucleotides

1. Introduction

DDX23, a DEAD-box helicase family member, exhibits versatile regulatory functions in genome stability maintenance, RNA processing, and translational control [1,2]. The protein is an integral component of the U5 small nuclear ribonucleoprotein complex, facilitating spliceosomal conformational alterations through RNA duplex unwinding [2,3]. DDX23 maintains genomic stability via R-loop resolution [4] and participates in antiviral immunity through viral dsRNA detection and subsequent IRF3/NF-kB pathway activation [5,6,7].

DDX23 dysregulation is implicated in both cancer development and neurological disorders. Notable upregulation occurs in ovarian, pancreatic, and glial neoplasms, correlating with aggressive phenotypes and unfavorable clinical outcomes. In ovarian cancer, E2F1-driven DDX23 overexpression modulates FOXM1 splicing, promoting oncogenic FOXM1C isoform generation [8]. DDX23 activates Notch pathway in non-small cell lung cancer enhancing linc00630 expression [9]. In pancreatic ductal adenocarcinoma, METTL3-mediated m6A methylation stabilizes DDX23 mRNA, promoting gemcitabine resistance through PI3K/Akt pathway activation [10]. Glioma progression involves DDX23-mediated miR-21 biogenesis regulation [11]. Conversely, DDX23 deficiency or mutations compromises antiviral responses and neurological function, manifesting as developmental delay, autism spectrum disorder, seizures, and dysmorphism [7,12,13]. Current therapeutic approaches targeting DDX23 lack selectivity and include an antiparasitic drug and pan-helicase inhibitor ivermectin as well as estrogen receptor (ER) antagonists endoxifen and fulvestrant [11,14].

An approach to modulate gene expression with high specificity and effectiveness explores antisense oligonucleotides (ASOs) that are designed to bind to specific RNA sequences. A number of ASOs have been approved for commercial use [15], and they are increasingly recognized as powerful tools for uncovering the biological functions of genes. The main antisense mechanisms include RNase H1-dependent mRNA degradation and pre-mRNA splicing regulation for down- and up-regulation of gene expression, respectively [16]. However, ASOs can also utilize other mechanisms such as translation inhibition due to steric hindrance or no-go decay degradation [17,18,19]. To increase gene expression, ASOs are designed to disrupt mRNA 5’ UTR secondary structures or mask upstream open reading frames (uORF) that negatively affect translation of the coding sequence (CDS) [20,21].

Chemical modifications of ASOs have significantly enhanced their therapeutic potential through the improvement of target hybridization, stability, and cellular uptake. Striking examples include phosphorothioate (PS) backbones, 2′-O-methoxyethyl (2′-MOE) nucleotides, and locked nucleic acids (LNAs) that have proven effective in the treatment of genetic diseases [15]. LNAs represent ribonucleotide analogs featuring a methylene bridge between the 2’-O and 4’-C atoms of the ribose ring [22]. This structural constraint favors a 3’-endo conformation of the ribose moiety that results in optimization of hybridization characteristics and a context-dependent increase in melting temperature (T_m) up to 10 °C per modified nucleotide [23]. Additionally, LNA incorporation at ASO termini can enhance nuclease resistance, thus improving their therapeutic efficacy.

ASOs targeting 5’ UTR can interact with regulatory structural elements, such as hairpins and G-quadruplexes (rG4s) [21,24]. rG4 structures can fold within guanine (G)-rich sequences and consist of stacked G-quartets stabilized by a network of Hoogsteen hydrogen bonds and monovalent cations such as K⁺ [25]. In most cases, hairpins and rG4s function as translation inhibitors by acting as steric hindrances to the scanning pre-initiation complex (PIC) [25,26,27]. Previous transcriptomic analyses and bioinformatic predictions have indicated that DDX23 mRNA 5’ UTR contains putative rG4s [28,29]. Furthermore, RNA fold analysis suggests the presence of hairpin structures within the 5’ UTR [30,31]. Here, we employ spectroscopic analysis and LNA-based functional probing to characterize these structural elements and evaluate their regulatory capacity and targetability using dual luciferase assay.

2. Results and Discussion

2.1. Analysis of Potential Regulatory G-quadruplex Elements in 5’ UTR of DDX23 mRNA

The rG4 structure was previously identified in the ENST00000551468 transcript of DDX23 during investigation of its translation regulation by predominately rG4-resolving DEAH-box helicase DHX36 [28]. Although this finding is important, the later annotation (GENCODE release 48) implies that this specific isoform has a truncated 3’ end without the full coding sequence and 3’ UTR. Moreover, the sequence of the studied rG4 does not map to any other transcripts. Therefore, this rG4 has no influence on the isoforms coding full-length DDX23 proteoforms. Thus, we searched for rG4s in the MANE Select [32] isoform of DDX23 (ENST00000308025), which is more functionally relevant.

Computational analysis using QGRS software identified putative rG4-forming motifs within the DDX23 mRNA 5’ UTR exclusively (14-36 nt and 51-77 nt) and including proximal region of the coding sequence (14-36 nt and 76-96 nt) [33]. Transcriptomic techniques DMS-seq and G4RP-seq corroborated the formation of rG4 structures within 14-36 nt and 76-96 nt sequences (Figure S1) [29,34,35]. To study the putative rG4-folding in vitro, we synthesized RNA sequences that contain these rG4-forming motifs and 3-nt flanks, as well as control mutants with guanine-to-uridine substitutions (Figure 1A, Table S1): G1 (11-39 nt), G2 (48-80 nt) and G3 (73-99 nt).

We began the structural characterization of the sequences with thioflavin T (ThT)-based light-up assay [36] and used rTBA15 and BON1-2 with validated folding patterns as control rG4 and RNA duplex, respectively (Figure 2A) [37]. Only G3 sequence exhibited an enhancement in fluorescence intensity comparable to control rTBA15 that suggests rG4 formation.

Since the results of ThT light-up assay usually require additional validation due to possible false-positive outcomes [38], circular dichroism (CD) spectroscopy was used for additional structural analysis (Figure 2B). rG4s are typically parallel-stranded [26] and display characteristic CD spectra with positive and negative peaks at 263-267 nm and 240 nm, respectively [39,40,41]. However, the characteristic signals for RNA duplex also appear in the same spectral region, typically with maximum at 260-270 nm and with or without minimum at 230-240 nm [42,43,44,45]. This complicates the unambiguous assignment of secondary structure. The CD signal pattern of G3, with a maximum at 265 nm and a minimum at 237 nm, is most consistent with rG4. Furthermore, only the G-to-U mutant of G3 exhibited a decrease in ellipticity. This again indicates that G3 is the most probable rG4-forming sequence. For G1 and G2, the ellipticity of the mutants was higher, which reinforces doubts about their ability to form G4s, and we did not observe perfect alignment of signals with the characteristic peaks of rG4. Thus, among the three sequences, G3 has the highest probability of forming the rG4 structure; however, the slight increase in ellipticity compared to the mutant cast doubt on this conclusion and necessitate further verification.

Comparative CD analysis of native and mutated sequences was performed in potassium and lithium-containing buffers (Figure S2) [46,47]. K⁺ cations typically stabilize rG4 structures by coordinating the guanine O6 atoms within G-quartet, whereas Li⁺ cannot provide such stabilization due to its smaller ionic radius [48,49]. Only G3 exhibited modest spectral alterations upon K⁺-to-Li⁺ replacement, with peaks shifting towards characteristics of RNA A-form helix (positive and negative peaks at 268 nm and 235 nm, respectively). The minimal spectral changes observed for all other sequences, both wild type and mutant, further supported the inability of the G1 and G2 sequences to fold into rG4 structures.

The results obtained for G3 in vitro led us to investigate whether it influences the DDX23 mRNA translation when treated with pyridostatin (PDS), a potent G4 stabilizer [50]. Notably, rG4 structures positioned downstream of uORFs may enhance uORF translation, thus suppressing protein synthesis from CDS through synergistic inhibition [28]. To evaluate the impact of G3 stabilization, if formed in cellulo, a dual luciferase assay was conducted (Figure 3). The reporter plasmid encodes Renilla luciferase (Rluc) as a control as well as the native 5’ terminus of DDX23 mRNA, which is fused to firefly luciferase (Fluc) without AUG codon. Additionally, we utilized the same construct lacking the uORF start codon, in which ATG was mutated to AAG, and a construct with a different short 5’ UTR lacking rG4-forming motifs and uORFs (Figure 3A).

We observed that uORF induces approximately 2.5-fold translation repression, as accessed by the change in the Fluc/Rluc ratio following uORF inactivation regardless the presence of PDS or DMSO (Figure 3B). This result aligns with efficient translation of uORF according to ribosome profiling data (Figure 1C). At the same time, PDS treatment induced a similar change in relative luciferase activities across all constructs tested (as evident after normalization to DMSO), calling into question the presence of rG4 or its influence on translation (Figure 3C).

Given the results of luciferase reporters, additional CD spectra were recorded in the presence of PDS. An increase in CD ellipticity was observed only for G1 (Figure 3D). However, considering previous experimental results, rG4 formation in the G1 sequence remains unlikely. The absence of the G3 response to the PDS treatment contradicted rG4 folding, despite the ThT-based light-up assay providing encouraging results and the CD spectral changes during K⁺-to-Li⁺ substitution (Figure 2A and Figure S2).

For further structural validation of G3 folding pattern, thermal difference spectra (TDS) and UV-melting analyses were used [51,52]. These methods revealed no characteristic hypochromic shift at 295 nm during melting, typically associated with rG4 structures, although TDS displayed minor negative peak around 295 nm (Figure 4A,B).

We hypothesized that G3 may fold into an alternative structure such as a hairpin. The potential hairpin formation is supported by the sequence’s capacity to form three stable canonical GC pairs and four GU wobble pairs [30,31,53]. CD melting of G3 was monophasic with T_m of 58 °C, indicating sufficient stability of the folded structure under physiological conditions (Figure 4C). Minimal hysteresis suggests an intramolecular structure.

The G3 structure was then investigated using ¹H NMR spectroscopy (Figure 4D). A broad signal in the 10.8-11.8 ppm region may indicate rG4 formation, whereas other broad signals at 10.4, 11.9 and 13.4 ppm may correspond to the imino protons engaged in Watson-Crick base pairing. A poor signal-to-noise ratio, possibly due to aggregation or interconversion, prevented unambiguous structural assignment. The comparative analysis was conducted using two mutant sequences: mutG3 (a mutant sequence with no ability to form rG4) and h_mutG3 (designed to form exclusively rG4 structure through substitution of wobble pair-forming uridines with adenines) (Table S1). ¹H NMR spectra of both mutants yielded clear interpretable signals. The sequence h_mutG3 demonstrated formation of a two-tetrad rG4, evidenced by eight signals from guanine imino atoms in the 10.8-11.8 ppm region, with minor fraction of an alternative rG4 conformation (Figure 4D). The mutG3 spectrum corresponded to the RNA hairpin-like conformation and contained four signals from imino protons of GU wobble pairs and four signals from canonical AU and GC pairs (Figure 4D). An additional signal may stem from a GU bifurcated pair [54,55] located in the region between the two double-stranded motifs. Comparative analysis of all three spectra suggests that G3 may form both rG4 and hairpin structures, as its ¹H NMR spectrum contains imino proton signals in regions characteristic of both rG4 (as in h_mutG3) and Watson-Crick GC base pairs (as in mutG3).

CD spectra of mutG3 and h_mutG3 corroborated the structural assignments derived from the ¹H NMR experiments. The CD spectrum of mutG3 had a positive peak at 260 nm, without minimum at 240 nm, which corresponds to a hairpin structure [42,56] (Figure S3). The presence of a positive peak at 263 nm and a negative peak at 240 nm indicated that h_mutG3 was folded into the rG4 structure. According to CD melting experiments, h_mutG3 was stabilized in the presence of 1 eq. PDS by 12 °C, while moderate (+7 °C) and little (+3 °C) changes in T_m for G3 and mutG3, respectively, were revealed (Figure 4E). The observed increase in G3 T_m does not contradict the absence of an increase in the CD maximum (Figure 3D), as has already been demonstrated for G4 ligands, including PDS [57,58]. In addition, UV melting proven to be ineffective for studying small RNAs that fold into alternative metastable structures [59]. These results confirmed that G3 could fold, at least partially, into rG4 in vitro.

To summarize this part, while the G3 sequence may adopt hairpin-like and rG4 conformations at equilibrium in vitro, as confirmed by spectroscopic methods, cell-based assays showed no response to the treatment with the G4 stabilizer PDS. Thus, none of the selected sequences forms a stable rG4 structure that may be regulatory. In contrast, a hairpin can be formed within the G3 sequence or the other part of the 5’ UTR. Such hairpin(s) could be involved in regulation of DDX23 mRNA translation.

2.2. Analysis of Regulatory Stem-Loop Elements

We identified the most probable hairpin within the 44-64 nt region by RNA fold [30,31]. Two oligoribonucleotides were synthesized to evaluate the influence of sequence context: hair_short (minimal hairpin-forming sequence) and hair_long (minimal hairpin-forming sequence with 6-nt flanks) (Table S1, Figure 1B). CD spectra showed maxima at 265 nm and minima at 233 nm (hair_short) and 236 nm (hair_long), consistent with A-form RNA helix formation (Figure 5A). CD melting analysis revealed T_m of 56 °C for hair_long and 66 °C for hair_short, indicating physiological stability despite the negative impact of additional 6-nt flanks on T_m (Figure 5B,C). Conditions with slow annealing produced alternative structures with uniform melting temperatures of 44 °C for both constructs (Figure 5B,C).

¹H NMR spectra of both sequences contained three distinct signals that were attributed to guanine imino protons from Watson-Crick GC pairs (Figure 5D). Thus, CD and ¹H NMR spectroscopies confirmed the hairpin structure predicted by RNA fold [30,31], which should be thermodynamically stable under cellular conditions.

The identified structured elements within 44-64 nt (hair_short) and 73-99 nt (G3) regions of DDX23 mRNA 5’ UTR may act as a translation-inhibiting element. While the thermal stability of hair_short appears insufficient for substantial translation inhibition (T_m around 60 °C, less than 13 kcal/mol based on ViennaRNAfold computational analysis [30,31]), its position downstream of the uORF start codon might facilitate synergistic inhibition of CDS translation, consistent with previous observations in other systems and partially explaining efficient uORF translation indicated by ribosome profiling data (Figure 1C) [60,61,62]. In turn, G3 also has T_m close to 60 °C and may promote the recognition of the uORF start codon and inhibit the CDS translation.

2.3 Evaluation of LNA-based ASOs Activity in DDX23 5’ UTR Translation Control

Since downregulation of DDX23 expression has shown therapeutic potential in cancer treatment, and current approaches are limited to non-selective helicase inhibitors and siRNAs with transient silencing effect [8,11], we designed a set of fully LNA-modified ASOs targeting start codons of uORF and CDS and/or the structured regions hair_short and G3 within DDX23 mRNA 5’ UTR and assessed their effects on the translation efficacy (Figure 6A, Table 1). LNA modifications were used to enhance nuclease resistance and hybridization properties, the latter being particularly important for unfolding of stem-loop structures. Previous study demonstrated that fully LNA-modified ASOs targeting 5’ UTR can equally or, in some cases, more effectively suppress mRNA translation compared to LNA-DNA chimeras with predicted ability to recruit RNase H [63]. Furthermore, fully modified blocker ASO targeting 5’ UTR can enhance the efficacy of RNase H1-activating ASOs that target mRNA coding regions [64].

Since the efficiency of ASO translation inhibition depends on the stability of ASO-RNA duplex, T_m was calculated using T_m predictor (Table 1) [65]. The predictor data show that all LNAs form duplexes with high stability under physiological conditions, exceeding the stability of the endogenous structures that have been detected in the 5’ UTR (with T_m < 70 °C). Therefore, LNAs are predicted to be highly effective in binding to mRNA and inhibiting translation. To evaluate LNA-modified ASO efficacy, we performed a dual luciferase assay. Fluc mRNA was synthesized using the wild-type DDX23 luciferase reporter construct and the construct with the inactivated uORF start codon (Figure 6B). For the control, we synthesized Rluc mRNA (Figure 6B) (see Materials and methods). HEK293T cells were co-transfected with Fluc reporter and Rluc control mRNAs as well as with ASOs LNA1-6 or the scramble LNA (SCR). The ASOs were used at 2, 10 and 100 nM concentrations, with SCR demonstrating no significant effects on the Fluc/Rluc ratio at any concentration compared to no ASO control (Figure 6C,D).

We observed translational repression with all ASOs targeting the DDX23 reporter mRNA of wild type, particularly at 100 nM concentration (Figure 6C). This result may be explained by the general inhibition of the translational machinery’s activity on the reporter mRNA. Nevertheless, the effects were not uniform across ASOs type and concentration. ASOs LNA1 and LNA2 target regions around the uORF start codon and should therefore mask it and repress uORF translation while enhancing CDS translation. However, they were the most effective inhibitors among ASOs under study at 10 and 100 nM concentrations (Figure 6C). This may be explained by their cap proximity, which hinders PIC loading. Interestingly, LNA ASOs exhibited a concentration dependency except for LNA3, which was less effective inhibitor. This difference was especially noticeable at 100 nM concentration (Figure 6C). Such effect may be explained by targeting of uORF or hair_short. To resolve this issue, we performed the same experiment with the DDX23 reporter mRNA lacking the uORF start codon. All LNAs showed inhibitory effects at 10 and 100 nM concentrations, which were concentration-dependent for all LNA ASOs (Figure 6D).

All LNA-modified ASOs except LNA2 and LNA3 demonstrated marginally diminished inhibitory effects for the no uORF reporter in comparison to the wild-type mRNA reporter (Figure 6E). Weaker effects observed for LNA2 in the mutated construct may be attributed to a nucleotide mismatch at its 3’ end because of the point substitution in the uORF start codon. Such mismatch should result in a reduction of the thermodynamic stability of the RNA–LNA duplex and also make it a more favorable substrate for RNA-helicases.

Interestingly, in the case of mutation in the uORF start codon, LNA3 exhibits approximately the same inhibitory properties as the other ASOs (Figure 6D). Thus, the low efficiency of translation inhibition by LNA3 in the WT reporter is likely attributable to uORF translation. Hair_short might be suggested to enhance uORF translation, so LNA3, by unwinding it, would be expected to reduce uORF translation and correspondingly increase translation of the CDS, thereby yielding the observed low apparent efficacy of LNA3 due to mixed positive and negative effects. However, this explanation is unlikely. First, by unwinding the endogenous hairpin (T_m close to 60 °C), LNA3 forms an even more stable mRNA–LNA3 duplex (predicted T_m 82 °C, Table 1) closer to the uORF start codon, which could even enhance uORF translation and, relative to other ASOs, more effectively inhibit translation of the CDS. Second, although LNA4, like LNA5 and LNA6, masks the CDS start codon, its effects on translation should be different due to its partial overlap with hair_short. Because none of these outcomes is observed, we suppose that both the endogenous hairpin and the mRNA–LNA3 duplex are insufficiently stable to increase uORF translation efficiency at that distance (>15 nt) from the uORF start codon. Moreover, enhancement of translation by a downstream hairpin has been reported primarily for start codons in a weak context [61,62,66], whereas in DDX23 the context is strong: A at –3 and G at +4 positions (Figure 1) considering the optimal Kozak context [67].

A more plausible explanation is that the ribosome translating the uORF impedes LNA3 binding to the 5’ UTR and/or promotes the dissociation of already bound LNA3, which accounts for its low efficacy as a translation inhibitor. A similar effect is known for ASOs targeting CDS [64]; however, to our knowledge, it has not been described for uORFs. This model also explains the concentration-independent effects of LNA3 on translation of the wild-type construct (Figure 6C). Our explanation is indirectly supported by ribosome profiling data (Figure 1C) indicating high ribosome occupancy on the uORF of endogenous DDX23 mRNA, higher than on the CDS. This suggests that the LNA3 binding site is particularly well shielded by translating ribosomes.

Thus, our study of LNA-ASOs suggests a new hypothesis/design principle for ASOs inhibiting translation: an ASO should not target an efficiently translated uORF, because the high ribosome density in this region will preclude effective binding to the 5’ UTR. Furthermore, given that neither the unwinding of hair_short with LNA4 nor the formation of a more stable mRNA–LNA3 duplex closer to the uORF start codon has an effect on the efficiency of the CDS translation, we hypothesize that hair_short does not affect uORF translation efficiency, but rather may act as a weak inhibitor of the CDS translation by imposing steric hindrance to PIC scanning along the 5’ UTR or have a role unrelated to translation.

3. Materials and Methods

3.1 Oligonucleotide Synthesis and Sample Preparation

Unmodified RNAs were synthesized according to the optimized synthetic protocol on an automated ASM-800 DNA/RNA synthesizer (Biosset, Russia). For detritylation, capping and oxidation, 3% solution of dichloroacetic acid in CH₂Cl₂, propionic anhydride and N-methylimidazole, and iodine solution in tetrahydrofuran: water: pyridine mixture, respectively, were used. At the condensation stage, 0.1 M solutions of protected 2’-O-TBDMS-ribonucleotide 3’-phosphoramidites (ChemGen, USA) in absolute CH₃CN and 0.25 M solution of activator 42 (Sigma-Aldrich, USA) in absolute CH₃CN were used. Time of condensation was 7 min. The last 5’-O-dimetoxytrityl group was removed, and oligonucleotides were deprotected and cleaved from CPG support by the treatment with AMA (40% methylamine: 30% ammonium, 1:1) for 2 h at room temperature with subsequent treatment with NMP:TEA:TEA·3HF mixture for 1.5 h at 65 °C. After an addition of ethoxytrimethylsilane (Sigma-Aldrich, USA), precipitation with ethyl ether was carried out. All RNAs were isolated by preparative denaturating 15% PAGE. The RNA homogeneity was analyzed by analytical gel electrophoresis in denaturating 15% PAGE. Fully LNA-modified ASOs were purchased from Lumiprobe (Russia).

RNA solutions in 20 mM sodium phosphate buffer supplemented with 140 mM KCl (K⁺-buffer) or LiCl (Li⁺-buffer), pH 7.4, were annealed rapidly (heated to 90 °C and then snap-cooled on ice) to facilitate intramolecular folding. Thioflavin T (ThT) and pyridostatin (PDS) were obtained from Sigma-Aldrich (USA).

3.2 Thioflavin T (ThT) Light-Up Assays

Experiments were conducted using 384-well U-Bottom White Polystyrene microplates (CORNING, USA). Annealed RNA samples in K⁺-buffer and ThT were mixed to final concentrations of 2 µM and 1 µM, respectively, and incubated for 15 min. Measurements were performed at 25 °C. Fluorescence emission spectra were collected from 470 nm to 650 nm with excitation at 440 nm using a M200 PRO Tecan microplate reader (Tecan Group Ltd., Switzerland). Fluorescence intensities at 485 nm were used for data analysis.

3.3 Circular Dichroism (CD) and UV Spectroscopy and Melting

CD and UV measurements were performed using a Chirascan spectropolarimeter (Applied Photophysics, UK) with a 10 mm optical path quartz cuvette. CD spectra of annealed 2 µM RNA samples in K⁺- or Li⁺-buffer were recorded at 10 °C from 230 nm to 300 nm. TDS spectra were obtained by subtracting the absorption spectra in the range 230 nm to 320 nm recorded at 90 °C from those recorded at 10 °C. For the experiments with PDS, annealed 2 µM RNA samples in K⁺-buffer were supplemented with PDS (2.5 mM stock solution in DMSO) to 2 µM final concentration or equivalent DMSO volume. Each reported spectrum represents an average of 2 scans. Melting/annealing experiments were conducted with a heating/cooling rate of 1 °C/min from 20 °C to 90 °C, monitoring changes at 265 nm (CD melting) or 295 nm (UV melting).

3.4 NMR Experiments

Samples was prepared in DEPC-treated water (100 μM RNA oligonucleotide, 25 mM PBS, 100 mM KCl, 90:10 H₂O/D₂O, pH 7.0) and annealed rapidly by heating at 90 °C for 5 min and then snap-cooling on ice for 10 min. NMR spectra were acquired at 25 °C on Bruker Avance III 600 MHz spectrometer (Bruker, Germany) equipped with a triple resonance cryogenic probe and Bruker Topspin 3.2 software. ¹H spectra were recorded using the standard zgesgp pulse sequence with water suppression at 4.7 ppm, 16 dummy scans and 1024 to 4096 scans. The pre-scan delay was set to 1 sec. FIDs were processed with an exponential window function and line broadening of 5.0 Hz.

3.5 Cell Culturing

The HEK293T cells (ATCC) were cultivated in DMEM/F12 medium (Servicebio), supplemented with L-alanyl-L-glutamine (Himedia, India), 10% fetal bovine serum (Himedia, India), 100 units/ml penicillin, and 100 μg/ml streptomycin (Himedia) at 37 °C in 5% CO₂ atmosphere. Cells were routinely tested for the absence of mycoplasma using the MycoReport kit (Evrogen, Russia).

3.6 Plasmid Constructs

The plasmid for the dual luciferase assay, containing firefly (Fluc) and Renilla (Rluc) under different promoters, was made from the pGL3-Rluc vector (a kind gift from Radik R. Shafikov, unpublished). The vector backbone was amplified using Q5 High-Fidelity DNA Polymerase (NEB, USA) with primers 5’-AGACGAGTTGGCACGTCTCAGGAGAAGACGCCAAAAACATAAAG-3’ and 5’-TAAGAGCTCGGTACCTATCGATAGAGAAATGTTCTGGCAC-3’, and the EF-1α core promoter was amplified from the lentiCas9-Blast plasmid (Addgene #52962) using primers 5’-AACATTTCTCTATCGATAGGTACCGAGCTCTTAGGGCAGAGCGCACATCG-3’ and 5’-TTCTCCTGAGACGTGCCAACTCGTCTCGACCTAACCGGTCCTGTGTTCTG-3’. The products were assembled into the reporter vector using NEBuilder HiFi DNA Assembly Master Mix (NEB, USA), introducing two BsmBI sites after the EF-1α core promoter and immediately before the Fluc ORF without AUG codon. The 5’ end of the DDX23 transcript, including 20 codons of CDS, was amplified from cDNA, obtained by the reverse transcriptase Magnus and oligo(dT)₁₅ primer (Evrogen, Russia), using primers 5’-GAACCTCGTCTCTAGGTTTCATCTCCGCGACCAG-3’ and 5’-TCAATGCGTCTCACTCCCCTTTCCTCCTTGGAAGGT-3’. The PCR-product was cloned into Esp3I sites of the reporter vector using Esp3I (Thermo Fisher, USA) and T4 ligase (Evrogen, Russia). The mutant with inactivated uORF start codon (no uORF) was obtained by overlap extension PCR of the wild-type sequence using primers 5’-GAAAGAAGGCGACGGCTCCGC-3’ and 5’-AGCCGTCGCCTTCTTTCC-3’.

3.7 Transfection

HEK293T cells were transfected with plasmids using the Lipofectamine 3000 Transfection Reagent Kit (Invitrogen, USA) in 96-well format according to the manufacturer’s protocol. In brief, 24,000 cells per well were seeded overnight in 200 µl of the medium for plasmid transfection, or 100 µl of the medium for mRNA transfection. 50 ng of plasmid DNA or a mixture containing 49 ng of Fluc reporter mRNA, 1 ng of Rluc control mRNA, and 10 pmol of LNA ASO, as well as 0.2 µl of Lipofectamine 3000 Transfection Reagent per well were used. If a treatment was required, the medium was replaced with a substance-supplemented medium prior to adding the transfection mixtures. The cells were harvested 4 hours after mRNA transfection and 24 hours after plasmid transfection for luciferase assays.

3.8 In vitro Transcription

Fluc reporter constructs were amplified (Q5 High-Fidelity DNA Polymerase, NEB) from plasmid reporters using primers 5’-GAGTACTTAATACGACTCACTATAGATCTCCGCGACCAGGAAACG-3’ and 5’-TTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTCCGCCCCGACTCTAGAATTACACGG-3’, and the Rluc control was amplified from pGL4.70[hRluc] (Promega) using primers 5’-GAGTACTTAATACGACTCACTATAGTGGTTCTTTCCGCCTCAGGCCACCATGGCTTCCAAG-3’ and 5’-TTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTTCTCTAGAATTACTGCTCGTTCTTCAGCACG-3’ to add the T7 promoter and a poly(A) tail consisting of 50 adenosine bases. Capped mRNA was synthesized from these PCR products and was treated with TURBO DNase using the mMESSAGE mMACHINE T7 Transcription Kit (Invitrogen). The mRNA was subsequently purified with the CleanRNA Standard kit (Evrogen, Russia), and its integrity was assessed by denaturing urea polyacrylamide gel electrophoresis. RNA concentrations were measured using the Qubit RNA HS Assay Kit (Invitrogen).

3.9 Luciferase Assay

Luciferase activities were measured using the TransDetect Double-Luciferase Reporter Assay Kit (TransGen Biotech, China) according to manufacturer protocol in a 96-well format using Victor X5 plate reader (Perkin Elmer, USA).

3.10 Visualization of Ribosome Profiling

Aggregate ribosome profiling data were accessed using the RiboCrypt browser for ENST00000308025 in RFP modality for all merged Homo sapiens datasets (accessed on 22 September 2025). The link is available below.

https://ribocrypt.org/?dff=all_merged-Homo_sapiens&gene=DDX23-ENSG00000174243&tx=ENST00000308025&library=RFP&frames_type=columns&kmer=1&log_scale=FALSE&log_scale_protein=FALSE&extendLeaders=0&extendTrailers=0&viewMode=FALSE&other_tx=FALSE&add_uorfs=FALSE&add_translon=FALSE&genomic_region=&zoom_range=0:101&customSequence=&phyloP=FALSE&summary_track=FALSE&summary_track_type=lines&collapsed_introns_width=30&collapsed_introns=FALSE&go=TRUE#browser

3.11 Statistical Analysis

The samples were analyzed using the Shapiro-Wilk test, indicating normal distribution at p > 0.05. Statistical analysis was performed using GraphPad Prism 10.3.1 software (GraphPad Software).

4. Conclusions

Using fluorescence, CD, UV and ¹H NMR spectroscopies, two structured elements were identified within DDX23 5’ UTR mRNA coding for the full-length protein and then, together with the sequences covering start codons, were targeted with LNA-modified ASOs. The study yields several significant outcomes. First, it suggests a new principle for designing translation-inhibiting ASOs: avoid targeting efficiently translated uORFs, as their high ribosome density blocks ASO binding. Second, there are several elements in DDX23 mRNA 5’ UTR relevant to its translation. The first is uORF, which represses the CDS translation, and the other are two structured elements within 44-64 nt and 76-96 nt. The hairpin hair_short within 44-64 nt likely inhibits translation of DDX23 mRNA blocking PIC scanning, without interference with uORF translation, 76-96 nt element may have a similar influence. ASO targeting 5’ proximal region of mRNA are effective translation inhibitors due to impaired PIC loading. To carefully modulate uORF translation, the thermal stability of ASO-RNA duplex formed should be carefully tuned to avoid creating a roadblock for translation machinery, more powerful than endogenous structures. These findings provide valuable insights for developing more effective ASOs targeting the main DDX23 transcript, and mRNA in general, and regulating its translation for potential anticancer applications.