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Review

Revisiting Two Decades of Research Focused on Targeting APE1 for Cancer Therapy: The Pros and Cons

by
Matilde Clarissa Malfatti
,
Alessia Bellina
,
Giulia Antoniali
and
Gianluca Tell
*
Laboratory of Molecular Biology and DNA Repair, Department of Medicine, University of Udine, 33100 Udine, Italy
*
Author to whom correspondence should be addressed.
Cells 2023, 12(14), 1895; https://doi.org/10.3390/cells12141895
Submission received: 30 May 2023 / Revised: 6 July 2023 / Accepted: 14 July 2023 / Published: 20 July 2023
(This article belongs to the Special Issue DNA Damage and DNA Repair: What’s New in Biology and Cancer Therapeutics?)
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Abstract

:
APE1 is an essential endodeoxyribonuclease of the base excision repair pathway that maintains genome stability. It was identified as a pivotal factor favoring tumor progression and chemoresistance through the control of gene expression by a redox-based mechanism. APE1 is overexpressed and serum-secreted in different cancers, representing a prognostic and predictive factor and a promising non-invasive biomarker. Strategies directly targeting APE1 functions led to the identification of inhibitors showing potential therapeutic value, some of which are currently in clinical trials. Interestingly, evidence indicates novel roles of APE1 in RNA metabolism that are still not fully understood, including its activity in processing damaged RNA in chemoresistant phenotypes, regulating onco-miRNA maturation, and oxidized RNA decay. Recent data point out a control role for APE1 in the expression and sorting of onco-miRNAs within secreted extracellular vesicles. This review is focused on giving a portrait of the pros and cons of the last two decades of research aiming at the identification of inhibitors of the redox or DNA-repair functions of APE1 for the definition of novel targeted therapies for cancer. We will discuss the new perspectives in cancer therapy emerging from the unexpected finding of the APE1 role in miRNA processing for personalized therapy.
Keywords:
APE1; inhibitors; cancer

1. A Brief Introduction to APE1 Biology and Different Functions

The acronym APE1/Ref1 (or more simply APE1) stands for apurinic/apyrimidinic endodeoxyribonuclease-reduction/oxidation factor 1, which is a well-known protein with multifunctional roles ranging from the endodeoxyribonuclease activity on DNA and RNA to the hub role in several reduction/oxidation (redox) signaling pathways [1,2,3].
Historically, APE1 has been largely known for its function during the base excision repair (BER) pathway [4], in which non-bulky DNA lesions are repaired. In the BER, APE1 functions as the main specific endodeoxyribonuclease able to cleave abasic sites (AP), which are generated spontaneously or by the action of specific glycosylases. The single strand break (SSB) generated by APE1 cleavage is then brought to complete repair by other downstream BER enzymes (i.e., Polβ, XRCC1, FEN1, and Ligase III). Recent data have demonstrated that SSBs are also sensed by APE1 to initiate 3′-5′ SSB end resection and to promote ATR/Chk1-mediated DNA damage response (DDR) activation [5]. Indeed, through its exonuclease activity, APE1 generates a short ssDNA gap that, via PCNA and APE2, becomes a longer stretch of ssDNA coated by RPA that leads to the assembly of the ATR/Chk1 DDR complex [5,6]. Another main cellular role of APE1 is to function as a redox hub for several transcription factors (TFs). Indeed, the reduction of some TFs (i.e., NF-κB, p53, Hif-1α, AP-1, Pax-5/8, etc.) by APE1 allows their activation and, consequently, the initiation of the transcription of specific genes (i.e., IL-8, SIRT-1, VEGF, etc.). An additional role of APE1 in transcriptional regulation is due to its capacity to stabilize G-quadruplex (G4), which are stable conformational structures in the G-rich DNA portion of certain human promoters [7,8,9]. Although, following oxidative stress, the newly formed 8-oxoguanine (8-oxoG) can stall transcription due to its destabilizing effect, there is evidence that its presence in some promoters may induce the formation of BER-stabilized G4 that enhances gene expression [10,11]. In this context, the binding of APE1 to G4 sequences promotes G4 folding. Moreover, the acetylation of APE1 (acAPE1) enhances its residence time on DNA and stabilizes G4 structures in cells [12]. In this way, APE1 facilitates transcription factor loading at the promoter, thus modulating gene expression [13].
Finally, some recently characterized APE1 functions, especially those involved in RNA metabolism [14,15,16,17,18], have drawn particular attention. Specifically, APE1 has been demonstrated to be able to cleave abasic RNA [15] and damaged ribonucleotides embedded in DNA [17,18], revealing it as an efficient endoribonuclease. Furthermore, only in the last few years, in concomitance with its novel and unsuspected involvement in the RNA metabolism, it has been described that APE1 can be present in subcellular condensates formed through liquid-liquid phase separation mechanisms (LLPS) [19,20,21] and can be secreted by tumoral cells through extracellular vesicles (EVs) [22].
These intriguing APE1 roles have been discovered in three decades of constant interest in this protein, delineating them in physiological and pathological contexts and making APE1 an attractive therapeutic target for several pathologies, including cancer [23]. However, after more than 20 years of attempts, targeting APE1 still represents an important challenge in cancer therapy. In this review, we will focus on the dysregulation of APE1 in cancer, and then we will describe well-known inhibitors of the main functions of APE1, paving the way for novel functions involved in chemoresistance and potentially used as new therapeutic targets.

2. APE1 and Cancer: A Focus on Polymorphisms and Tissue Expression

As previously discussed, being involved in such focal cellular processes, the dysregulation of APE1 has a great impact on pathologies like cancer, making it an attractive therapeutical target [2,24]. APE1 dysregulation is involved in tumor development at three different levels, as it may concern alterations to its genetic sequence, expression, or localization [2]. It must be clearly stated, however, that, up to now, there is not clear evidence for a driver or passenger function of either of the above-mentioned alterations in the tumorigenic processes.
Several studies pointed out the importance of single nucleotide polymorphisms (SNPs) on the APE1 gene in cancer pathology [25] (Figure 1). The most common and studied APE1 variant is Asp148Glu (D148E), which is present in about 48% of the population [26]. X-ray crystallography experiments showed that this variant lacks significant structural changes and is considered benign [27]. As a matter of fact, the protein bearing this SNP holds normal AP endonuclease and DNA binding properties, but its 3′-RNA phosphatase and endoribonuclease activities are affected [16,28]. The role of this polymorphism in cancer is controversial due to several conflicting studies in the literature [26]. This common variant has been widely studied in more than one hundred publications. Indeed, numerous studies and meta-analyses observed an association between the D148E variant and an increased risk of different cancers, while others reported the opposite pattern even in the same tumor type [2,26,29].
Another biochemically studied APE1 polymorphic variant associated with cancer development is Arg237Cys (R237C) [30,31]. This substitution, which is prevalently observed in endometrial cancer [30,31], affects the functional activity of the whole protein [27]. X-ray crystal protein structure analysis revealed that this aminoacidic variation caused significant shifts in adjacent DNA binding residues, leading to a great decrease (~3-fold) of APE1 DNA binding ability [27]. Remarkably, this polymorphic variant showed a reduced ability to interact with its BER partners, such as Pol β and XRCC1 [25]. For example, X-ray data highlighted that the close lysine 244 (K244), which is implicated in the APE1-Pol β interaction [32], was shifted in the 3D structure, affecting the protein-protein interaction [27]. Moreover, the R237C variant showed reduced AP-endonuclease [25], 3′->5′ exonuclease, and 3′-damage excision [31] activities other than a reduced incision capacity close to nucleosomes [33].
One additional endometrial tumor-associated variant is Pro112Leu (P112L) [30], which exhibits comparable AP-endonuclease activity to the wild-type form [31].
In this review, we performed an analysis on cBioPortal to find SNPs or insertion/deletions (IN/DELs) in the APEX1 gene that are in association with different cancer types, considering a curated selection of non-redundant studies (213 studies selected, 69,223 samples, and 65,853 patients) (https://bit.ly/3M9Oya7 (accessed on 22 March 2023)) [34,35]. The somatic mutation frequency of APEX1 was 0.2%, with 108 unique variants. None of the variants detected represented a driver mutation for cancer, and most of them were sporadic. The most frequent variants were R193C/H, D148E, and H289Y/Q. Interestingly, even though R193C and R193H variants were detected to a comparable extent to D148E in the selected cohort of studies, there are no published works that focus on this mutation and its functional impact. According to the Mutation Assessor tool [36,37], R193H had a low impact on the protein’s functional activity, while R193C might have a worse one. There were no functional studies, even regarding H289Y/Q variants, which were predicted to have a neutral impact on protein activity. In Table 1, we report each variant found by using the cBioPortal tool, divided by tumor type.
APE1 overexpression, as well as its altered localization, are prominent features of several different tumors, often with poor prognosis and malignant phenotypes. We hereafter provide a description of how APE1 is altered in cancer and how it impacts tumorigenesis (Table 2).
In bladder cancer (BCa), several studies detected high expression levels of the APE1 protein in tumor tissues, compared to normal adjacent tissues, that were associated with poor outcomes [39,41,44]. APE1 overexpression was also linked to lymphovascular invasion features, as high VEGFA levels and an infiltration of CD163+ tumor-associated macrophages (TAMs) [42]. Moreover, the cellular distribution of APE1 was variable between high- and low-grade tumors. Whereas low-grade cancers displayed increased APE1 levels only in the nucleus, high-grade invasive tumors showed increased positive staining even in the cytoplasm [39]. APE1 is also a promising diagnostic biomarker in BCa, as its levels were increased in serum and urine when compared to normal healthy controls and were associated with tumor grade and stage, recurrence, and invasion [38,40,43]. Interestingly, a study observed an increased secretion of APE1 in bladder tumors displaying the D148E variant compared to the ones expressing the wild-type form, which contributed to increased serum levels of the protein in patients [129].
Concerning hepatocellular carcinoma (HCC), APE1 was upregulated at both transcriptional and translational levels compared to normal liver tissues [81,82,83]. Moreover, the mRNA content increased with tumor progression and was higher in less differentiated and more aggressive tumors [81]. Patients with higher APE1 protein levels exhibited unfavorable prognoses and a lower OS [82,83]. Interestingly, both APE1 truncated forms, missing the first 33 residues (N∆33–35 kDa), and APE1 full length (37 kDa), were detected in HCC tissue samples and HCC cell lines [84]. Moreover, the cellular distribution of APE1 was altered, with nuclear staining only in normal liver tissues while presenting a significant fraction of cytoplasmic positivity in tumor tissues [85]. Cytoplasmic APE1 was about three times higher in poorly differentiated tumors and was associated with a reduced OS [85]. Noteworthy, the cytoplasmic staining was prevalently associated with APE1 mitochondrial accumulation in grade 1 and grade 2 HCC tumors, but not in grade 3 tumors [86]. Even in HCC, APE1 serum levels can be exploited as a novel diagnostic biomarker, correlating with its overexpression in HCC tissues [84].
The APE1 protein was also overexpressed in pancreatic adenocarcinoma (PDAC) tissues and cell lines and associated with tumor aggressiveness and poor survival [122,123,124]. The proteolytic form of APE1 N∆33 has been detected even in PDAC tissues, with different abundances versus adjacent non-tumor tissue [55]. Interestingly, acAPE1 was overexpressed in PDAC tumors, while being almost undetectable in healthy pancreatic tissues [55,87]. acAPE1 has increased AP-endonuclease activity, which has been proposed as a cancer mechanism to overcome chemotherapy genotoxic stress and uphold proliferation [87]. APE1 localization in PDAC was mainly nuclear and similar between primary tumors and metastases [123]. An increased cytosolic localization was observed only in advanced tumor stages and was always concurrent with nuclear localization, while the complete absence of the cytoplasmic fraction was associated with invasion and poor differentiation [101,123].
Concerning prostate cancer (PCa), APE1 protein levels were upregulated compared to normal or benign hypertrophy (BPH) tissue [125,126]. Moreover, higher APE1 levels were observed in tumors bearing the TMPRSS2:ERG fusion [126]. APE1 localization was only nuclear in normal prostate tissue and non-cancerous prostate cell lines, while there was an increased expression in the cytoplasm compartment in tumor tissues and tumoral cell lines [125].
APE1 overexpression occurs also in oesophageal carcinomas, like oesophageal adenocarcinoma (EAC) [102,103,104] and oesophageal squamous cell carcinoma (ESCC) [105,106], probably as a mechanism adopted by cancer cells to survive the genotoxic effects of bile reflux [105,106]. APE1 localization was mainly nuclear and also associated with a worse OS in patients receiving platinum chemotherapy [101].
An in silico analysis identified APE1 as a central hub gene for gastric cancer, as its overexpression had a great prognostic value in two analyzed datasets (GSE1611533 and GSE54129) [64]. Indeed, APE1 is overexpressed at both transcriptional and translational levels in gastric cancer [65,66]. APE1 staining was weak in normal, non-cancerous gastric tissues, while it was high in tumor tissues. APE1 localization was detected both in the nuclear and cytoplasmic compartments of tumor tissues [66]. High levels of APE1 were also correlated with invasion and poor prognosis [66], as its serum levels are a valuable diagnostic biomarker for lymph node metastasis prediction [67].
APE1 was also upregulated in salivary gland carcinomas, and its levels increased depending on the malignant transformation process of the tumor [127]. APE1 overexpression was higher in smaller tumors displaying lymph node metastasis and invasive growth [127,128]. APE1 localization was mainly nuclear in every salivary gland tumor subtype analysed, except for adenoid cystic carcinomas, in which it was highlighted to present both nuclear and cytoplasmic localization [127,128].
Furthermore, the overexpression of APE1 protein and mRNA levels was also reported in non-small-cell lung cancers (NSCLCs) [88,89,90,91]. High APE1 expression was associated with poor prognosis, invasion, and chemoresistance as its levels increased upon treatment with platinum compounds [90]. Moreover, high APE1 serum levels, post-treatment, were correlated with a poorer OS [92]. Nuclear APE1 staining was associated with favourable patient outcomes [93], while a higher cytoplasmic localization was correlated with both poor survival and a shorter RFS [94,95,96]. Although both full-length and truncated forms were found in lung cancer, APE1 was prevalently truncated at the N-terminus in adjacent non-tumor tissues in NSCLC [55]. Moreover, acAPE1 was overexpressed in NSCLC tumors, with a strictly nuclear localization [55,87].
Several studies identified the overexpression of the APE1 protein in ovarian cancers, which has been associated with advanced tumor stages and decreased OS [101,114,115]. Moreover, patients with high levels of APE1 showed more frequent resistance to platinum therapy [101,114,116]. The interaction between APE1 and nucleophosmin 1 (NPM1) has been extensively examined in ovarian cancer, as the levels of the two proteins were positively associated with tumor aggressiveness, malignant phenotype, lymph node metastasis, and poor chemosensitivity [114,117]. It has been shown that compounds that impair this interaction can exert a synergistic effect on traditional chemotherapeutic molecules [118]. APE1 localization seemed to be heterogeneous in ovarian cancers, depending on the stage and histological subtype [24]. Some studies showed prominent cytoplasmic staining, which increased from well- to poorly-differentiated cancers and was higher in advanced-stage tumors [116,117,119,120]. In non-responding cisplatin patients, the observed APE1 overexpression was mainly at the cytoplasmic level, a feature that was also observed in cisplatin-resistant cell lines [116]. Interestingly, almost 90% of patients with abnormal levels of cytosolic APE1 displayed an abnormal distribution of NPM1 too [117]. Additionally, cytosolic APE1 can be considered an independent predictive factor for poor PFS and OS in ovarian cancer [119]. Other works showed prominent nuclear APE1 staining, which increased during tumorigenesis and was associated with survival time [115,121]. Additional studies showed an increase in APE1 in both compartments, but higher nuclear staining was associated with cancer aggressiveness, lower debulking after surgery, platinum resistance, and lower OS [101,116].
Concerning breast cancer, different studies reported conflicting results about APE1 protein expression levels. Some works described APE1 overexpression as mostly nuclear and associated with malignant phenotypes and an unfavourable prognosis [45,46,47]. Contrary to the pattern of increased acetylation observed in other cancer types [55,87], APE1 acetylation was lower in breast cancer compared to healthy tissues [48]. Even in this case, the functional interaction between APE1 and NPM1 in promoting platinum resistance has been described [49]. In contrast to these findings, another study showed that lower levels of APE1 were associated with tumor aggressiveness and a triple-negative phenotype [50]. Interestingly, in the Ki-67 low-level expression group, lower levels of APE1 were associated with poor OS [46].
APE1 protein levels were upregulated even in cervical tumors and were associated with Epithelial-to-Mesenchymal transition (EMT), lymph node metastasis, and poor radio-sensitivity [51,52,53,54]. APE1 localization was widely heterogeneous among cervical tumors, although with a main nuclear stain [52]. Remarkably, there was a significant difference in the subcellular localization of APE1 between radiotherapy non-responding and responding tumor cell lines. Indeed, radio-resistant cervical tumor cell lines showed higher levels of the cytoplasmic fraction and lower levels in the nucleus, suggesting a role for cytosolic APE1 in radio-resistance promotion [53].
Several studies described an overexpression of APE1 in colorectal cancers (CRC), observing a gradual increase in its expression during tumor progression [56,57,58,59] and in liver metastasis [60]. APE1 localization was heterogeneous between CRC cells, as the protein was found concurrently both in the nucleolus and cytoplasmic compartment, or, otherwise, it displayed an exclusive cytoplasmic localization [56]. Even in CRC tumor samples and cell lines, nuclear acAPE1 was overexpressed [55,61] and positively correlated with resistance to 5-Fluorouracil (5-FU) [61]. Moreover, both full-length and truncated forms were detected in colon cancer [55]. Interestingly, the levels of serum APE1 autoantibodies are valuable as diagnostic biomarkers for CRC [62].
Regarding gliomas, conflicting data are available. Some studies described an overexpression of APE1 in tumoral tissues compared to healthy ones [68,69], with a 13-fold increase in AP-endonuclease activity in 93% of tumors [68]. Glioma radioresistant cell lines displayed higher levels of APE1 compared to responding cell lines [70]. Indeed, an increase in APE1 expression was observed in patients after treatment and recurrence [71]. On the other hand, different studies have evidenced low mRNA and protein expression in adult high-grade gliomas, which was associated with poor OS [72,73]. Moreover, APE1 localization was predominantly nuclear [72].
Concerning melanoma, several studies identified APE1 overexpression at both transcriptional and translational levels [97,98,99]. Indeed, APE1 was overexpressed in melanoma cancer cell lines and in clinical samples, showing a prominent nuclear localization in both cases [98,99]. High mRNA levels were associated with vascular invasion, high proliferation rates, poor RFS, and OS [97,100]. Patients with higher levels of APE1 also showed a lower response to therapy [100]. APE1 was also overexpressed in another skin tumor, namely cutaneous squamous cell carcinoma (cSCC) [63], which was associated with increased proliferation and migration by EMT [63].
APE1 was dysregulated in several head and neck squamous cell carcinomas (HNSCC). In oral SCC (oSCC), APE1 was overexpressed at the protein level, and its high expression was significantly correlated with nodal status, shorter OS, and DFS [74,75]. APE1 localization was mainly nuclear, but translocation to the cytoplasm was observed after cisplatin treatment [74,76]. Moreover, APE1 serum levels represent a promising diagnostic biomarker [77]. Indeed, high levels of serum APE1 (sAPE1) were associated with late TNM stages, lymph node metastasis, and worse pathological differentiation [77]. Patients with lower levels of sAPE1 went through longer DFS after post-surgery cisplatin therapy and longer OS [77]. APE1 overexpression was also observed in laryngeal SCC (LSCC) [78], in sino-nasal SCC (sSCC), and in SCC with inverted papilloma (SCCwIP), with a vivid nuclear localization associated with metastatization [79]. Moreover, sSCC tumors showed higher cytoplasmatic staining compared to SCCwIP [79], which was associated with a higher T-stage and histological grade [79]. Lastly, APE1 overexpression, also characterized by lip SCC (lSCC), showed strong nuclear localization [80].
Furthermore, APE1 levels were upregulated in osteosarcoma and associated with poor prognosis and cisplatin resistance [107,108,109,110,111,112,113]. APE1 localization was both nuclear and cytoplasmic [107,112]. Patients with higher levels of the protein in the cytoplasmic content were less responsive to cisplatin treatment and experienced recurrence and metastasis [107].
Therefore, in general, APE1 is significantly overexpressed in different kinds of cancers, and subcellular distribution may significantly change depending on the specific tissue and tumoral stage, but in which way the overexpression and localization of APE1 in tumors are causally responsible for cancer onset and development, aggressiveness, and invasion is still debated. Currently, knowledge about the role played by APE1 polymorphic variants in cancer onset and progression is still unknown, as are the possible driver or passenger functions of APE1 mutations in cancer tumorigenesis. As mentioned above, the most accepted hypothesis regards the increased expression of APE1 in tumoral cells as they acquire a proliferative and chemoresistant phenotype. Several studies have proposed that the upregulation of APE1, as well as that of other BER enzymes, may underlie pro-survival mechanisms adopted by tumors to efficiently repair DNA damage, thus contributing to the onset of resistance mechanisms. Although the main function of APE1 is attributable to its endoribonuclease activity, it is believed that APE1 overexpression may also contribute to tumorigenesis through increased activity as a redox activator of several TFs, such as NF-κB, thus leading to an increase in tumor proliferation and survival and affecting the tumor microenvironment. We do believe that additional dysregulated functions of APE1, including dysregulation of RNA and miRNA metabolism and regulation of G4-structures containing promoter genes, could play an essential role in cancer development, although more detailed investigations are needed along these lines.
In conclusion, further analysis on how and why altered APE1 expression is differentially associated with cancer development and metastasis should be a central aim of further study in the future.

3. APE1 as a Still Promising Therapeutic Target after 20 Years of Research

In the last decades, APE1 has emerged as a promising therapeutic target in cancer, either for its role in DNA repair or in redox regulation of TF activities. In the next paragraphs, we will dive deeper into these functions of APE1, highlighting the study progression around the discovery of specific inhibitors, principally employed in chemotherapy (Table 3). Finally, we will discuss the new roles of APE1 in RNA metabolism and in cell signaling through its secretion, hypothesizing these novel functions as promising new targets in cancer therapy.

3.1. Targeting the APE1 Endonuclease Activity

The endonuclease function of APE1, which is essential in the BER pathway, depends on residues sited on the C-terminal region of APE1. The most important amino acids involved in this activity are E96, which is implied in the coordination of divalent metals, and D210 and H309, both required for the hydrolytic reaction [130] (Figure 1). Other important residues that mediate different cleavage functions can be found in the C-terminal region too, including: D70, involved in the 3′-phosphodiesterase activity [131], K98, required in the Nucleotide Incision Repair (NIR) [132], and F266, implicated in the 3′-5′ exonuclease activity [133].
Previous studies identified different compounds that inhibit the endonuclease APE1 activity in vitro and in human cells, as summarized in different reviews [134,135,136,137]. Over the years, various groups have extensively worked towards the identification of specific small-molecule inhibitors able to target the DNA repair function of APE1 in combination studies, with the rationale that the blockade of APE1 endonuclease activity might have various therapeutic applications, particularly in cancer treatment, by sensitizing cancer cells to DNA-damaging agents and leading to tumor cell death. Although many studies support the inhibition of APE1 as a means of complementing current chemotherapeutic regimens and, accordingly, various chemical inhibitors have been developed, a clinical candidate has yet to be realized. Indeed, despite their high activity in vitro, the toxicity and selectivity in cells of the majority of the reported endonuclease inhibitors remain to be established. In this section, we attempt to present the major APE1 inhibitors identified thus far and discuss their activity. It is not within our scope to revisit all the inhibitors in depth; a comprehensive list of APE1 endonuclease inhibitors is reviewed in [130,137,138]. The published approaches utilized for the development of APE1 endonuclease inhibitors can be mainly categorized into: (i) screening of commercially available compounds that were synthesized for targeting other molecules; (ii) computational screening, and (iii) pharmacophore modeling.
One of the first studied molecules impairing APE1 repair activity was Methoxyamine (MX), an alkoxyamine derivative that reacts to form an imine with the aldehyde group in the ring-open form of the abasic lesion, thereby indirectly blocking APE1 endonuclease activity [139,140]. Since MX was demonstrated to enhance the cytotoxicity effect of alkylating agents such as temozolomide (TMZ) in a wide variety of cancer cell lines both in vitro and in xenograft models [141,142], it advanced to clinical trials; however, to date, clinical studies have not shown any clear success.
A second compound that was first identified as a radio-sensitizer of HeLa cells [143] and subsequently reported to be an inhibitor of APE1 by Luo and Kelly in 2004 [144] is Lucanthone, or Miracil D. Lucanthone was shown to enhance the cell-killing effect of TMZ and an alkylating agent such as methyl methanesulfonate (MMS) in culture and was further characterized by Naidu et al. to bind to the hydrophobic pocket site of APE1 [145]. No other studies were successively reported, but its specificity is still debated since a part of its inhibitory effect is mediated by its ability to intercalate within DNA and through the inhibition of topoisomerase II and possibly other cellular proteins [23].
Afterward, numerous laboratories relied on high-throughput screens (HTS), mainly based on fluorescence assays, to identify inhibitors of APE1 endonuclease activity. In general, the identification of the potential hits was followed by different assays aiming to prove specificity and selectivity for APE1 inhibition, including the AP site incision assay, the ability of the compound to bind DNA per se, and the ability to enhance the cytotoxicity of alkylating agents (i.e., TMZ, MMS). It is worth mentioning that the inhibitors reported so far showed affinities in the µM range that are not compatible with a suitable pharmaceutical agent, and more importantly, none of them has been demonstrated to have utility in pre-clinical animal cancer models. CRT0044876 (7-nitroindole- 2-carboxylic acid) is the first biochemically and biologically reported APE1 inhibitor identified through a fluorescein/dabcyl-based AP site incision assay [146]. Madhusudan et al. identified the compound CRT0044876 from a screening of a collection of structurally diverse small molecules. Despite the initial promising results obtained in the potentiation of the cell-killing effects of MMS and TMZ, the reproducibility of this compound has been brought into question [23,147], and because of its poor solubility and permeability, this compound has been further neglected until now, since its usage has been proposed conjugated with platinum [148]. Considering the weak results obtained with CRT0044876, other screenings were performed. Using a similar HTS approach, Seiple et al. screened the 2000-compound NCI Diversity Set of small molecules and identified aromatic nitroso, carboxylate, sulfonamide, and arylstibonic acid compounds with µM affinities for the APE1 protein [149]. Again, for these compounds, the relatively high inhibitory potency observed in vitro did not match a significant parallel effect in cells. Successively, various one-off studies did not progress to lead optimization. For example, in 2009, prompted by the evidence that APE1 represents an attractive therapeutic target in anticancer drug development, Zawahir et al. utilized a pharmacophore-based approach that was used to carry out a virtual screen of a 365,000 small molecule library [150]. The known interactions of APE1 with AP site-containing DNA, including components of hydrophobicity, H-bond acceptor, and negatively ionizable features, were utilized to design a virtual screen. In the same year, Simeonov et al. employing a quantitative HTS, screened the commercially available Library of Pharmacologically Active Compounds (LOPAC), identifying 6-hydroxy-DL-DOPA, Reactive blue 2, and myricetin as possible APE1 inhibitors [147]. Although these approaches predicted several potentially positive hits, they were not all tested in cell-based assays and thus have not been evaluated for cell permeability.
Successively, Kelley’s group has also used a fluorescence-based high-throughput assay to screen a library of 60,000 small-molecule compounds for their ability to inhibit the AP endonuclease activity of APE1 [151]. The most promising compounds were designated as APE1 Repair Inhibitor AR01, 02, 03, and 06. AR03 is chemically distinct from the previously reported small-molecule inhibitors of APE1. This compound was demonstrated to inhibit the cleavage of AP sites in vitro using whole cell extracts and to potentiate the cytotoxicity of TMZ and MMS in glioblastoma SF767 cells. Furthermore, very recently, AR03 was demonstrated to inhibit the exonuclease activity of APE1 in the SSB-induced ATR-Chk1 DDR pathway in human bone osteosarcoma U2OS cells, MDA-MB-231, and PANC1 [5,20]. While it is cell-permeable, its planar fused-ring structure may suggest its DNA intercalating ability, thus potentially being non-specific.
In 2011, Mohammed et al. focused on developing APE1 inhibitors for melanoma and glioma treatments using a structure-based drug design approach [98]. The crystal structure of APE1 was utilized to create four pharmacophore models, including the interactions of the previously identified inhibitor CRT0044876 with active site residues and molecular scaffolds designed to fit the ligand binding site. From the screening of 1679 hits, the authors identified compound 4 (N-(4-fluorophenyl)-2-(4-phenylsulfonyl-2- (p-tolyl)oxazol-5-yl) sulfanyl-acetamide) as the one with the highest AP endonuclease inhibitory activity and the potential to sensitize the activity of MMS and TMZ in both glioma and melanoma cell lines but not in HUVEC cells, suggesting specificity for malignant tissue.
In 2012, a new class of inhibitors of the catalytic endonuclease function was identified by Aiello et al. [152]. Compounds 32–35, which have a 3-benzylcarbamoyl-2-methoxybenzoic acid structure, showed the most active and selective inhibition activity of APE1. These compounds have the potential to be used in combination therapy with 5-fluorodeoxyuridine for colon cancer treatment. In the same year, using docking-based virtual screening, 15 potential compounds were identified as inhibitors of APE1 from a library of over 4 million molecules [153]. Two of these compounds, 36 and 37, were found to be potent inhibitors of the protein and could increase the toxicity of MMS. Through molecular dynamics simulations, it was discovered that these compounds may interact with the protein through important binding modes such as hydrogen bonds with specific residues and hydrophobic interactions by virtue of their quinoxaline core. In 2012, Simeonov’s group performed a fully automated HTS using a kinetic fluorescence assay on the NIH Molecular Libraries Small Molecule Repository and other collections, examining each agent at different concentrations [154]. They identified active APE1 inhibitors able to potentiate the genotoxic effect of MMS, leading to an increase in AP sites. The chemical structures of the most effective inhibitors, namely MLS001196838, MLS000587064, MLS000737267, MLS000090966, and MLS000863573, would have served as starting points for medicinal chemists to further optimize them.
Another fluorescence-based quantitative HTS of 352,489 small molecules from the NIH Molecular Libraries Small Molecule Repository was performed by Rai et al. [155]. APE Inhibitor III (N-(3-(1,3-Benzo[d]thiazol-2-yl)-6-isopropyl-4,5,6,7-tetrahydrothieno[2,3-c]pyridin-2-yl)acetamide) has been demonstrated to potentiate MMS and TMZ activity in HeLa cells. This compound was further used and distributed by the sellers as one of the most promising APE1 inhibitors for both its endonuclease and exonuclease activities; however, this compound has not significantly advanced beyond in vitro studies. Using the crystal structure of APE1, Srinivasan et al. computationally constructed molecules that would sterically block its endonuclease site and identified molecules that all contain the 2-methyl-4-amino-6,7-dioxoloquinoline structure [156]. The mechanism of action of the compounds was probed by fluorescence and competition studies in T98G glioma cell lines, which indicated for compounds 1 and 4 a direct interaction between the inhibitor and the active site of the APE1 protein.
In 2015, a pharmacophore model for APE1 small-molecule inhibitors was used to identify new compounds by means of in silico screening of 10,159 compounds [157]. The virtual docking assay identified four compounds with a 2-methyl-4-amino-6,7-dioxoloquinoline core (AJAY 1–4); AJAY 4 showed the best results in the inhibition of cell growth; however, none of the compounds have advanced in clinical studies.
Another novel in silico approach was pursued by Trilles et al., who, guided by X-ray crystal structures of APE1 and computational docking of solvents, identified binding hotspots for small organic molecules [158]. Accordingly, they screened a library of macrocycles for inhibition of APE1 endonuclease activity and identified four novel macrocycles that they used as a starting point for designing APE1 ligands. From the initial screening of 66 compounds, only four exhibited concentration-dependent inhibition of APE1 endonuclease activity (MC043, MC047, MC042, and MC019). Building on these hits, additional macrocycles were synthesized, and macrocyclic lactams 13, 21, and 24 have been demonstrated to be more effective in inhibiting APE1 endonuclease function in combination with MMS.
Unfortunately, none of the compounds developed so far have advanced to significant in vivo studies or clinical trials. Very recently, two works argued about the specificity of some of the most prominent compounds that are usually sold by suppliers as APE1 inhibitors. In the work of Pidugu et al., it has been demonstrated through structural, biophysical, and biochemical approaches that several reported small molecules are weak APE1 inhibitors [159]. In particular, through an NMR chemical shift perturbation assay, they showed that CRT0044876 and three similar indole-2-carboxylic acid compounds (5-fluoroindole-2-carboxylic acid [98], 5-nitroindole-2-carboxylic acid, and 6-bromoindole-2-carboxylic acid) bind at a pocket of APE1 that is distal from its active site. Furthermore, using Dynamic light scattering (DLS), they also demonstrated that CRT0044876 [146], myricetin [147], and APE Inhibitor III [155] form colloidal aggregates that could sequester APE1, causing non-specific inhibition. For this latter compound, Xue and Demple recently questioned about the specificity of this molecule [138]. Since APE1 knock-out lines (CH12F3 [160]) showed equal sensitivity to direct killing by APE Inhibitor III, being even more sensitive to APE Inhibitor III than its wildtype counterpart, the authors claimed possible off-target effects that must be taken into account when using these inhibitors at high dosages.

3.2. Targeting the APE1 Redox Activity

Unlike the BER function, which is highly conserved from prokaryotes (E. coli exonuclease III) to humans, the redox function is probably unique to mammalians [161]. Whereas the C-terminal of APE1 is mainly involved in the regulation of endodeoxyribonuclease activity, the N-terminal, principally consisting of an unstructured region, is strongly implicated in protein-protein interactions and in the activation of several TFs via a redox mechanism. Specifically, the redox function of APE1 is exploited by cysteine residues sited at positions 65, 93, and 99 of the N-terminal region (Figure 1). These residues are involved in the redox cycle responsible for controlling the reduced state of several TFs [161]. By reducing the TFs, APE1 makes them able to bind DNA. APE1 then returns to its basal state through another reduction that occurs via a thiol/sulfide exchange with thioredoxin. Among the several TFs regulated by APE1, we include the principals such as NF-κB [162], AP-1 [162], HIF1α [163], STAT3 [164,165], p53 [166], NRF2 [167], Pax-5 and -8 [168], and others [169]. Given the roles of all these TFs in cellular biological processes, the effects of APE1 as a redox signaling factor regard principally the promotion of growth, migration, DDR signaling, and survival in tumor cells, as well as inflammation and angiogenesis in the tumor microenvironment. Thus, inhibition of APE1 redox activity can be a target for slowing growth and progression during tumoral processes. Indeed, the pharmacological inhibition of APE1 redox activity causes a decrease in the ability of the TFs to bind to DNA [169,170,171] and thereby increases the cancer cells’ response to chemotherapeutic agents [172,173].
Differently from the AP-endonuclease inhibitors, testing redox inhibitors resulted in more complications during these years, due in part to the arduous modalities of detection of the redox activity of APE1. In this paragraph, we propose a roundup of the literature on a few redox inhibitors that have emerged on the scientific scene.
Dietary agents and several compounds from natural sources, such as soy isoflavones, resveratrol, and curcumin, as well as the vitamins ascorbate and α-tocopherol [174], were initially tested. Curcumin is a polyphenol with the potential for treatment or prevention of particular human diseases such as oxidative and inflammatory conditions, metabolic syndrome, arthritis, anxiety, hyperlipidemia, and cancer [175]. In 2017, it was demonstrated that curcumin affected the APE1 redox function, inhibiting the transcriptional activity of APE1 on AP-1 and NF-κB genes in vitro [176]. For its multiple anti-inflammatory, antioxidant, and anti-neoplastic properties, curcumin has been enrolled in more than 300 clinical trials. Resveratrol is a naturally occurring polyphenolic compound present in red wine and grapes. It has been demonstrated that it exhibits a neuroprotective role in models of central nervous system diseases, including cerebral ischemia/reperfusion injury [177]. By inhibiting APE1 redox function, resveratrol caused a significantly diminished activity of AP-1 and NF-κB proteins in different human cancer models, enhancing the cytotoxicity of chemotherapy [99]. Similarly, utilizing soy isoflavones to block redox signaling through APE1 and NF-κB dramatically increased prostate cancer cells’ sensitivity to radiation [178].
About ten years ago, the Kelley’ group synthesized a molecule that turned out to be highly promising in the inhibition of APE1 redox activity in several cancer models [24,179]. This molecule [(2E)-2-[(4,5-dimethoxy-2-methyl-3,6-dioxo-1,4-cyclohexadien-1-yl)methylene]-undecanoic acid, commonly denoted as APX3330 (or E3330), is a quinone derivative. Several studies were then performed using different pathological models both in vitro and in vivo, in which it was demonstrated that APX3330 selectively inhibited NF-κB-mediated gene expression through APE1 binding [180]. In 2009, Zou et al. demonstrated that APX3330 blocked the in vitro growth of pancreatic cancer-associated endothelial cells and the differentiation of bone marrow-derived mesenchymal stem cells into CD31(+) endothelial progeny. Specifically, the effect was attributable to a reduction of H-Ras expression and intracellular nitric oxide (NO) levels, as well as decreased DNA-binding activity of HIF-1α. Inhibition of the APE1 redox function by APX3330 might be a potent therapeutic strategy in solid tumors [181]. Indeed, APX3330 showed anticancer properties in pancreatic cancer, including inhibition of cancer cell growth and migration in several cancer cell lines and xenograft models in mice [182]. APX3330 inhibited the proliferation, migration, and tube formation of retinal vascular endothelial cells in vitro and reduced retinal angiomatous proliferation and neovascularization in vivo [183]. As anticipated in the previous paragraphs, elevated expression levels of APE1 have been correlated with more aggressive phenotypes and a poor prognosis for NSCLC. Recently, Manguinhas et al. demonstrated that APX3330, in combination with cisplatin, reduced H1975 cell viability, migration, and invasion, highlighting its use as a boost for cisplatin in NSCLC cells [184]. Moreover, the inhibition of APE1 redox function through APX3330 combined with docetaxel treatment decreased the proliferative rate, migration, and invasion of MDA-MB-231 breast cancer cells [185]. The APX3330 inhibitory activity was also assessed in pathological angiogenesis, such as retinal neovascularization [186]. Li et al. demonstrated that APX3330 treatment suppressed experimental choroidal neovascularization in vitro and in vivo, demonstrating that APE1 regulates multiple TFs and inflammatory molecules and is essential for CEC angiogenesis. That could represent a novel candidate for therapeutically targeting neovascular eye diseases and alleviating the burden associated with anti-VEGF intravitreal injections [187]. Recently, it has also been demonstrated that APX3330 has the potential to be used for the treatment of γ-herpesvirus infection and associated diseases [188].
Given its promising and potential anti-angiogenic and antineoplastic activities obtained in vitro, APX3330 was enrolled in the APX_CLN_0011 Phase 1 clinical trial in 2017. This trial (ClinicalTrials.gov (accessed on 4 April 2023) Identifier: NCT03375086) was a multi-center, open-label, dose-escalation oncology study of APX3330 in patients with advanced solid tumors. The study was completed in 2020, showing the assessment of APX3330’s safety, anti-tumor activity, pharmacokinetic and pharmacodynamic profile [189], and the recommendations for the Phase 2 study dose. Oral APX3330 demonstrated a favorable safety and tolerability profile and was suitable for Phase 2. In 2020, APX3330 was enrolled in the ZETA-1 Phase 2 clinical trial to evaluate its safety and efficacy to treat diabetic retinopathy and diabetic macular edema. The trial was completed this year (2023) (ClinicalTrials.gov (accessed on 4 April 2023) Identifier: NCT03375086). Oral administration of APX3330 and placebo has demonstrated a favorable ophthalmic and systemic safety and tolerability profile. Additional safety data from the ongoing ZETA-1 trial will be evaluated to further characterize the efficacy and safety of APX3330 for the oral treatment of diabetic eye diseases.
On the basis of the results obtained with APX3330, new analogues of this inhibitor were synthesized, including RN8–51, 10–52, and 7–60 [190]. Data have demonstrated that especially the analogue RN8–51 decreased cancer cell growth with little apoptosis, demonstrating itself as particularly promising for further anticancer therapeutic development. Kelley et al. synthesized novel, second-generation APE1 redox-targeted molecules such as APX2007, APX2009, APX2014, and APX2032 and determined whether they would be protective against neurotoxicity induced by cisplatin or oxaliplatin while not diminishing the platins’ antitumor effect. Specifically, they used an ex vivo model of sensory neurons in culture, through which they demonstrated that especially APX2009 [(2E)-2-[(3-methoxy-1,4-dioxo-1,4-dihydronaphthalen-2-yl)methylidene]-N,N-diethylpentanamide] was an effective small-molecule neuroprotective against cisplatin and oxaliplatin-induced toxicity. APX2009 also demonstrated a strong tumor cell killing effect in monodimensional cultured tumor cells, which was further substantiated in a more robust three-dimensional pancreatic tumor model [179]. Together, these data suggested that the second-generation compound APX2009 was effective in preventing or reversing platinum-induced CIPN while not affecting the anticancer activity of platins [179]. Moreover, all three compounds (APX2007, APX2009, and APX2032) demonstrated similar inhibition of NF-κB binding [179].
Finally, in 2010, Nyland et al. described a series of quinones, including benzoquinone and naphthoquinone, analogues of APX3330, with the ability to reduce tumor growth [191].

3.3. Targeting Both the APE1 Endonuclease and Redox Activities

Very few molecules have been demonstrated to inhibit both APE1 endonuclease and redox function. Among them, one was Gossypol [192]. Gossypol is a natural polyphenolic aldehyde that exhibits various effects, including antioxidant, anticancer, antiviral, antiparasitic, and antimicrobial activities. It can directly interact with APE1 and enhance the cell-killing effects of MMS and cisplatin. A recent clinical trial (ClinicalTrials.gov (accessed on 4 April 2023) Identifier: NCT00540722) aimed to investigate the potential clinical benefit of combining Gossypol with docetaxel and cisplatin in patients with NSCLC who have high expression of APE1 [193]. The trial, designed as a prospective and randomized study, did not show a significant difference between the Gossypol and placebo groups, although the Gossypol-treated patients had better outcomes in terms of increased PFS and OS.
One additional inhibitor was AT-101, a derivative of Gossypol and an oral inhibitor of the anti-apoptotic Bcl-2 and Bcl-xL proteins. AT-101 has been shown to exhibit potent anticancer activity, although its chemosensitizing effects are not fully understood. Indeed, AT-101 enhanced the sensitivity of A549 cells to cisplatin in vitro and in vivo by inhibiting APE1-mediated IL-6/STAT3 signaling activation, suggesting its potential use in NSCLC chemotherapy [194]. Moreover, it was also found to suppress gastric cancer cell migration and renewal and promote chemotherapeutic sensitivity in a gastric cancer model in vivo [195]. The molecular mechanism of its anticancer activity via inhibition of the endoribonuclease or redox activities of APE1 remains unclear.

4. Future Perspectives from Targeting the Non-Canonical Roles of APE1 in miRNA Processing

We recently proved that APE1 contributes to the expression of chemoresistance genes via functions in RNA metabolism involving miRNAs. We found that APE1: (i) binds to structured RNAs, including pri-miRNAs [14,196]; (ii) is involved in the processing of miRNAs implicated in cancer development (e.g., miR-221/222, miR-1246, miR-130b, miR-146a) [197]; and (iii) is a central hub connecting different subnetworks of cancer-associated proteins involved in RNA metabolism and miRNA sorting (e.g., NPM1, hnRNPA2/B1, AUF1, FUS, and SFPQ) [196,198,199]. We demonstrated that, during genotoxic stress, nuclear APE1 favors the processing and stability of miRNA precursors through its association with the DROSHA microprocessor complex, impacting, for example, the miR-221/222 axis and, in turn, modulating the expression of the tumor suppressor PTEN [14]. Using NSCLC cancer cell lines, we recently defined a signature of 13 miRNAs (miR-1246, miR-4488, miR-24, miR-183, miR-660, miR-130b, miR-543, miR-200c, miR-376c, miR-218, miR-146a, miR-92b, and miR-33a) that strongly correlate with APE1 expression in human lung cancer and play a central role in cancer cell proliferation and survival [197]. Whether these APE1-regulated miRNAs are responsible for cancer cell response to genotoxic treatment and explain the role of APE1 in chemoresistance through post-transcriptional mechanisms is still unknown and should be addressed to understand the central role of APE1 in cancer progression and to define new antitumor strategies. It should be defined whether APE1 recognizes specific oncogenic miRNAs alone or in combination with specific proteins through the detection of regulatory motifs present in the miRNA structure.

5. Secreted APE1 as a Novel Prognostic Non-Invasive Biomarker of Cancer Development

We recently showed that enzymatically active APE1 can be secreted (sAPE1) by cancer cells through EVs, including exosomes, during genotoxic stress conditions [8]. However, APE1’s presence in the extracellular milieu is still poorly characterized [186,187,188]. sAPE1 expression is actually considered a novel biomarker for the prognosis of NSCLC, as proved in a previous study performed on NSCLC patients, in which their levels of sAPE1 were significantly higher compared to healthy controls and were associated with a worse PFS [198]. Recently, data obtained by our research group confirmed these observations in a cohort of HCC patients [190], in which we found that sAPE1 levels correlated with poor prognosis and were able to discriminate between cancer patients and cirrhotic or healthy donors. The presence of this protein in the sera of patients is not solely restricted to cancer diseases but also in inflammatory models, such as coronary artery disease and endotoxemia [191,192]. The biological function of sAPE1 is still completely unknown. An intriguing hypothesis sees its action as a paracrine molecule triggering cell-to-cell communication, which is important for the local tissue microenvironment’s inflammatory response.
Evidence on the mechanisms responsible for APE1 secretion is lacking, even though the importance of the acetylation, occurring on specific lysine residues sited in the first 33 N-terminal portions of the protein (K27, K31, K32, and K35), has been highlighted in cells treated with the histone deacetylase inhibitor trichostatin A [14]. It seems reasonable that APE1 secretion might derive from EV formation via the endosomal sorting complex (ESCRT), due to the protein lacking a classic secretory signal peptide [193]. This pathway is responsible for the biogenesis and maturation of multivesicular bodies (MVBs), composed of many intraluminal vesicles (ILVs), that are released in the extracellular milieu as exosomes. ILV formation can occur through several mechanisms, and information about the regulation of these processes and the possible differences between the promoted cargo selections is still missing [194].
It is conceivable that these vesicles might be highly shuttled between cells within the tumor mass and deliver their content to target cells. This process may fulfill the cancer cells’ requirement for a high amount of APE1 to counteract the DNA damage inferred by drugs in a paracrine manner, suggesting that APE1-secretion could represent a novel damage-associated molecular pattern (DAMP) mechanism that deserves further in-depth study to develop inhibitors that could specifically target alterations of APE1 secretion in different cancers.

6. Conclusive Remarks and Future Perspectives

Despite the high potency of many of the compounds aforementioned, additional work is necessary to deliver more specific inhibitors of APE1-altered functions in tumors, which could be useful for clinical trials. While progress has certainly been made in identifying potent APE1 inhibitors, further efforts are needed to specifically achieve selectivity and efficacy. This will require consideration of both the abasic site binding pocket and more distal features of the enzyme that might be important for DNA binding. X-ray crystallography and in vivo experiments would be crucial to expedite rational inhibitor design, validate APE1 as a target, and explore possible side effects. Moreover, knowing the multiple APE1 cellular functions and their detailed molecular mechanisms could allow us to better target APE1 dysregulation in pathologies (Figure 2).
The discovery of novel functions for APE1 is constantly evolving. As mentioned in the introduction, the ability of APE1 to recognize and process SSBs through its 3′-5′ exonuclease activity [5,6] could represent an interesting target for developing new inhibitors specifically directed against this APE1 function and able to inhibit in ultimum the promotion of the ATR/Chk1-mediated DDR activation.
Moreover, targeting a protein-nucleic acid interaction is challenging, and this has contributed to the limited success in developing APE1 inhibitors. New approaches are needed for the discovery of novel and selective APE1 inhibitors. In this context, Wilson DM III et al. proposed the application of fragment- and structure-based drug discovery (FBDD/SBDD) methods in the quest for new clinical agents [200]. They applied the ABSOneStepTM platform, identifying 25 high-quality crystal structures showing unique and diverse fragment hits bound at the endonuclease site as well as at a previously unidentified secondary site, overall suggesting multiple novel strategies for inhibiting APE1. Indeed, in addition to direct inhibitors of APE1 nuclease activities, inhibitors against other functions of APE1 may also be clinically valuable. Considering the complex role of APE1, exploring allosteric modes of inhibition, such as disrupting vital interactions between APE1 and other cellular protein partners, might be an alternative option [118,201]. For example, we demonstrated that the molecular association with NPM1 modulates the endonuclease activity of APE1 [118]. HTS for the disruption of this interaction led to the discovery of three compounds (fiduxosin, spiclomazine, and SB 206553); of these, fiduxosin and spiclomazine displayed anti-proliferative activity and sensitized cells to bleomycin. A synergistic effect with platinum drugs was also observed by using these inhibitors in a triple-negative breast cancer cell model, demonstrating how APE1 could also represent a useful therapeutic biomarker in this type of tumor [49,202]. Similarly, the disruption of other APE1 protein interactions or functions can be taken into consideration.
Table
Table 3. List of the principal APE1 inhibitors. The principal APE1 inhibitors are grouped by the APE1 function inhibited, including the endonuclease activity, the redox activity, and the protein-protein interaction. For each inhibitor, the IUPAC name, the PubChem CID, the molecular formula and weight (MW), and the structure (obtained with PubChem Sketcher V2.4) are reported. At the end, the main references for each inhibitor are indicated. For more detailed information, refer to the text.
Table 3. List of the principal APE1 inhibitors. The principal APE1 inhibitors are grouped by the APE1 function inhibited, including the endonuclease activity, the redox activity, and the protein-protein interaction. For each inhibitor, the IUPAC name, the PubChem CID, the molecular formula and weight (MW), and the structure (obtained with PubChem Sketcher V2.4) are reported. At the end, the main references for each inhibitor are indicated. For more detailed information, refer to the text.
APE1
Function-
Inhibited		NameIUPAC
Name		PubChem CIDMolecular FormulaMW (g/mol)StructureRefs
EndonucleaseMethoxyamineO-methylhydroxylamine4113CH5NO47.057Cells 12 01895 i001[139,140,141]
Lucanthone1-[2-(diethylamino)ethylamino]-4-methylthioxanthen-9-one10180C20H24N2OS340.5Cells 12 01895 i002[143,144,145]
CRT00448677-Nitroindole-2-carboxylic acid81409C9H6N2O4206.15Cells 12 01895 i003[23,146,147,148]
Myricetin3,5,7-trihydroxy-2-(3,4,5-trihydroxyphenyl)chromen-4-one5281672C15H10O8318.23Cells 12 01895 i004[147]
AR032,4,9-Trimethylbenzo[b][1,8]naphthyridin-5-amine698490C15H15N3237.30Cells 12 01895 i005[151]
APE Inhibitor IIIN-[3-(1,3-benzothiazol-2-yl)-6-isopropyl-4,5,6,7-tetrahydrothieno[2,3-c]pyridin-2-yl]acetamide3581333C19H21N3OS2371.5Cells 12 01895 i006[155,156]
RedoxCurcumin(1E,6E)-1,7-bis(4-hydroxy-3-methoxyphenyl)hepta-1,6-diene-3,5-dione969516C21H20O6368.4Cells 12 01895 i007[175,176]
Resveratrol5-[(E)-2-(4-hydroxyphenyl)ethenyl]benzene-1,3-diol445154C14H12O3228.24Cells 12 01895 i008[99,177]
APX3330(2E)-2-[(4,5-dimethoxy-2-methyl-3,6-dioxocyclohexa-1,4-dien-1-yl)methylidene]undecanoic acid6439397C21H30O6378.5Cells 12 01895 i009[24,179,180,181,182,183,184,185,186,187,188,189]
APX2009(2E)-N,N-diethyl-2-[(3-methoxy-1,4-dioxonaphthalen-2-yl)methylidene]pentanamide71618575C21H25NO4355.4Cells 12 01895 i010[179]
Endonuclease RedoxGossypol7-(8-formyl-1,6,7-trihydroxy-3-methyl-5-propan-2-ylnaphthalen-2-yl)-2,3,8-trihydroxy-6-methyl-4-propan-2-ylnaphthalene-1-carbaldehyde3503C30H30O8518.6Cells 12 01895 i011[192,193]
Protein-protein interactionFiduxosin5-[4-[(3aR,9bR)-9-methoxy-3,3a,4,9b-tetrahydro-1H-chromeno[3,4-c]pyrrol-2-yl]butyl]-12-phenyl-8-thia-3,5,10,13-tetrazatricyclo[7.4.0.02,7]trideca-1(13),2(7),9,11-tetraene-4,6-dione172307C30H29N5O4S555.6Cells 12 01895 i012[49,118,202]
Spiclomazine8-[3-(2-chlorophenothiazin-10-yl)propyl]-1-thia-4,8-diazaspiro[4.5]decan-3-one65714C22H24ClN3OS2446.0Cells 12 01895 i013[49,118,202]
SB 2065531-methyl-N-pyridin-3-yl-6,7-dihydropyrrolo[2,3-f]indole-5-carboxamide5163C17H16N4O292.33Cells 12 01895 i014[49,118,202]
A new hot topic concerns RNA G-quadruplexes (RG4s), which are disease-associated non-canonical structures composed of stacks of guanine tetrads (called G-quartets) kept together by Hoogsteen hydrogen bonds. RG4s are increasingly recognized as fundamental post-transcriptional regulators of gene expression [203]. Interestingly, these elements are widespread in the transcriptome and are particularly enriched in miRNAs [204]. The folding of these structures can be controlled by their RBP interactors (i.e., hnRNPA2B1, FUS, etc.), cations (i.e., K+), and small molecule ligands [205], making RG4s highly dynamic. Very recent data underline a regulatory function played by RG4 in miRNA maturation through DROSHA- and Dicer-inhibition [206] and a potential role in physiological and pathological LLPS [207,208]. The presence of the RG4 structure in pre-miRNA exists in equilibrium with the canonical stem-loop structures, and this equilibrium regulates the maturation of some miRNAs, such as miR-92b [209]. However, mechanistic information on RG4 function in miRNA sorting is missing, as is information on the functional role of oxidized guanine (8-oxo) or abasic (AP) sites in the RG4-forming structures in the stability and biological properties of the miRNAs in which these structures are present. Understanding whether APE1 function in miRNA processing and degradation could be driven by RG4-mediated folding will open mechanistic views as well as translational applications in cancer biology. We are working along these lines.
Finally, this fascinating field of research relies on the findings that APE1 can be secreted in the extracellular milieu through EVs. Understanding the intracellular routes responsible for this secretion in cancer cells and the role of sAPE1 as a potential paracrine molecule will open new perspectives on precision medicine.

Author Contributions

Conceptualization, M.C.M. and G.T.; software, M.C.M. and A.B.; data curation, M.C.M., A.B., G.A. and G.T.; writing—original draft preparation, M.C.M., A.B., G.A. and G.T.; writing—review and editing, M.C.M., A.B., G.A. and G.T.; supervision, G.T.; funding acquisition, G.T. All authors have read and agreed to the published version of the manuscript.

Funding

This research was funded by AIRC under IG 2017, grant number ID. 19862 (Gianluca Tell).

Institutional Review Board Statement

Not applicable.

Informed Consent Statement

Not applicable.

Data Availability Statement

No new data were created with this paper.

Acknowledgments

The authors thank all the members of the G.T. lab for their fruitful feedback.

Conflicts of Interest

The authors declare no conflict of interest.

References

  1. Antoniali, G.; Malfatti, M.C.; Tell, G. Unveiling the Non-Repair Face of the Base Excision Repair Pathway in RNA Processing: A Missing Link between DNA Repair and Gene Expression? DNA Repair 2017, 56, 65–74. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  2. Malfatti, M.C.; Antoniali, G.; Codrich, M.; Burra, S.; Mangiapane, G.; Dalla, E.; Tell, G. New Perspectives in Cancer Biology from a Study of Canonical and Non-Canonical Functions of Base Excision Repair Proteins with a Focus on Early Steps. Mutagenesis 2020, 35, 129–149. [Google Scholar] [CrossRef] [PubMed]
  3. Malfatti, M.C.; Antoniali, G.; Codrich, M.; Tell, G. Coping with RNA Damage with a Focus on APE1, a BER Enzyme at the Crossroad between DNA Damage Repair and RNA Processing/Decay. DNA Repair 2021, 104, 103133. [Google Scholar] [CrossRef] [PubMed]
  4. Allinson, S.L.; Sleeth, K.M.; Matthewman, G.E.; Dianov, G.L. Orchestration of Base Excision Repair by Controlling the Rates of Enzymatic Activities. DNA Repair 2004, 3, 23–31. [Google Scholar] [CrossRef] [PubMed]
  5. Lin, Y.; Raj, J.; Li, J.; Ha, A.; Hossain, M.A.; Richardson, C.; Mukherjee, P.; Yan, S. APE1 Senses DNA Single-Strand Breaks for Repair and Signaling. Nucleic Acids Res. 2020, 48, 1925–1940. [Google Scholar] [CrossRef] [Green Version]
  6. Lin, Y.; Li, J.; Zhao, H.; McMahon, A.; McGhee, K.; Yan, S. APE1 Recruits ATRIP to SsDNA in an RPA-Dependent and -Independent Manner to Promote the ATR DNA Damage Response. eLife 2023, 12, e82324. [Google Scholar] [CrossRef]
  7. Hurley, L.H.; Wheelhouse, R.T.; Sun, D.; Kerwin, S.M.; Salazar, M.; Fedoroff, O.Y.; Han, F.X.; Han, H.; Izbicka, E.; Von Hoff, D.D. G-Quadruplexes as Targets for Drug Design. Pharmacol. Ther. 2000, 85, 141–158. [Google Scholar] [CrossRef]
  8. Fleming, A.M.; Burrows, C.J. G-Quadruplex Folds of the Human Telomere Sequence Alter the Site Reactivity and Reaction Pathway of Guanine Oxidation Compared to Duplex DNA. Chem. Res. Toxicol. 2013, 26, 593–607. [Google Scholar] [CrossRef] [Green Version]
  9. Fleming, A.M.; Zhu, J.; Ding, Y.; Visser, J.A.; Zhu, J.; Burrows, C.J. Human DNA Repair Genes Possess Potential G-Quadruplex Sequences in Their Promoters and 5′-Untranslated Regions. Biochemistry 2018, 57, 991–1002. [Google Scholar] [CrossRef]
  10. Fleming, A.M.; Burrows, C.J. 8-Oxo-7,8-Dihydroguanine, Friend and Foe: Epigenetic-like Regulator versus Initiator of Mutagenesis. DNA Repair 2017, 56, 75–83. [Google Scholar] [CrossRef]
  11. Fleming, A.M.; Zhu, J.; Ding, Y.; Burrows, C.J. 8-Oxo-7,8-dihydroguanine in the Context of a Gene Promoter G-Quadruplex Is an On–Off Switch for Transcription. ACS Chem. Biol. 2017, 12, 2417–2426. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  12. Burra, S.; Marasco, D.; Malfatti, M.C.; Antoniali, G.; Virgilio, A.; Esposito, V.; Demple, B.; Galeone, A.; Tell, G. Human AP-Endonuclease (Ape1) Activity on Telomeric G4 Structures Is Modulated by Acetylatable Lysine Residues in the N-Terminal Sequence. DNA Repair 2019, 73, 129–143. [Google Scholar] [CrossRef]
  13. Roychoudhury, S.; Pramanik, S.; Harris, H.L.; Tarpley, M.; Sarkar, A.; Spagnol, G.; Sorgen, P.L.; Chowdhury, D.; Band, V.; Klinkebiel, D.; et al. Endogenous Oxidized DNA Bases and APE1 Regulate the Formation of G-Quadruplex Structures in the Genome. Proc. Natl. Acad. Sci. USA 2020, 117, 11409–11420. [Google Scholar] [CrossRef] [PubMed]
  14. Antoniali, G.; Serra, F.; Lirussi, L.; Tanaka, M.; D’Ambrosio, C.; Zhang, S.; Radovic, S.; Dalla, E.; Ciani, Y.; Scaloni, A.; et al. Mammalian APE1 Controls MiRNA Processing and Its Interactome Is Linked to Cancer RNA Metabolism. Nat. Commun. 2017, 8, 797. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  15. Barnes, T.; Kim, W.-C.; Mantha, A.K.; Kim, S.-E.; Izumi, T.; Mitra, S.; Lee, C.H. Identification of Apurinic/Apyrimidinic Endonuclease 1 (APE1) as the Endoribonuclease That Cleaves c-Myc MRNA. Nucleic Acids Res. 2009, 37, 3946–3958. [Google Scholar] [CrossRef] [Green Version]
  16. Chohan, M.; Mackedenski, S.; Li, W.-M.; Lee, C.H. Human Apurinic/Apyrimidinic Endonuclease 1 (APE1) Has 3′ RNA Phosphatase and 3′ Exoribonuclease Activities. J. Mol. Biol. 2015, 427, 298–311. [Google Scholar] [CrossRef]
  17. Malfatti, M.C.; Balachander, S.; Antoniali, G.; Koh, K.D.; Saint-Pierre, C.; Gasparutto, D.; Chon, H.; Crouch, R.J.; Storici, F.; Tell, G. Abasic and Oxidized Ribonucleotides Embedded in DNA Are Processed by Human APE1 and Not by RNase H2. Nucleic Acids Res. 2017, 45, 11193–11212. [Google Scholar] [CrossRef] [Green Version]
  18. Malfatti, M.C.; Codrich, M.; Dalla, E.; D’Ambrosio, C.; Storici, F.; Scaloni, A.; Tell, G. AUF1 Recognizes 8-Oxo-Guanosine Embedded in DNA and Stimulates APE1 Endoribonuclease Activity. Antioxid. Redox Signal. 2023; ahead of print. [Google Scholar] [CrossRef]
  19. Tosolini, D.; Antoniali, G.; Dalla, E.; Tell, G. Role of Phase Partitioning in Coordinating DNA Damage Response: Focus on the Apurinic Apyrimidinic Endonuclease 1 Interactome. Biomol. Concepts 2020, 11, 209–220. [Google Scholar] [CrossRef]
  20. Li, J.; Zhao, H.; McMahon, A.; Yan, S. APE1 Assembles Biomolecular Condensates to Promote the ATR–Chk1 DNA Damage Response in Nucleolus. Nucleic Acids Res. 2022, 50, 10503–10525. [Google Scholar] [CrossRef]
  21. Dall’Agnese, G.; Dall’Agnese, A.; Banani, S.F.; Codrich, M.; Malfatti, M.C.; Antoniali, G.; Tell, G. Role of Condensates in Modulating DNA Repair Pathways and Its Implication for Chemoresistance. J. Biol. Chem. 2023, 299, 104800. [Google Scholar] [CrossRef] [PubMed]
  22. Mangiapane, G.; Parolini, I.; Conte, K.; Malfatti, M.C.; Corsi, J.; Sanchez, M.; Pietrantoni, A.; D’Agostino, V.G.; Tell, G. Enzymatically Active Apurinic/Apyrimidinic Endodeoxyribonuclease 1 Is Released by Mammalian Cells through Exosomes. J. Biol. Chem. 2021, 296, 100569. [Google Scholar] [CrossRef]
  23. Fishel, M.L.; Kelley, M.R. The DNA Base Excision Repair Protein Ape1/Ref-1 as a Therapeutic and Chemopreventive Target. Mol. Asp. Med. 2007, 28, 375–395. [Google Scholar] [CrossRef]
  24. Shah, F.; Logsdon, D.; Messmann, R.A.; Fehrenbacher, J.C.; Fishel, M.L.; Kelley, M.R. Exploiting the Ref-1-APE1 Node in Cancer Signaling and Other Diseases: From Bench to Clinic. NPJ Precis. Oncol. 2017, 1, 19. [Google Scholar] [CrossRef] [Green Version]
  25. Lirussi, L.; Antoniali, G.; D’Ambrosio, C.; Scaloni, A.; Nilsen, H.; Tell, G. APE1 Polymorphic Variants Cause Persistent Genomic Stress and Affect Cancer Cell Proliferation. Oncotarget 2016, 7, 26293–26306. [Google Scholar] [CrossRef] [PubMed]
  26. Wallace, S.S.; Murphy, D.L.; Sweasy, J.B. Base Excision Repair and Cancer. Cancer Lett. 2012, 327, 73–89. [Google Scholar] [CrossRef] [Green Version]
  27. Whitaker, A.M.; Stark, W.J.; Flynn, T.S.; Freudenthal, B.D. Molecular and Structural Characterization of Disease-Associated APE1 Polymorphisms. DNA Repair 2020, 91–92, 102867. [Google Scholar] [CrossRef]
  28. Kim, W.C.; Ma, C.; Li, W.-M.; Chohan, M.; Wilson, D.M., III; Lee, C.H. Altered Endoribonuclease Activity of Apurinic/Apyrimidinic Endonuclease 1 Variants Identified in the Human Population. PLoS ONE 2014, 9, e90837. [Google Scholar] [CrossRef] [PubMed]
  29. Wilson, D.M.; Kim, D.; Berquist, B.R.; Sigurdson, A.J. Variation in Base Excision Repair Capacity. Mutat. Res. 2011, 711, 100–112. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  30. Pieretti, M.; Khattar, N.H.; Smith, S.A. Common Polymorphisms and Somatic Mutations in Human Base Excision Repair Genes in Ovarian and Endometrial Cancers. Mutat. Res. 2001, 432, 53–59. [Google Scholar] [CrossRef]
  31. Illuzzi, J.L.; Harris, N.A.; Manvilla, B.A.; Kim, D.; Li, M.; Drohat, A.C.; Iii, D.M.W. Functional Assessment of Population and Tumor-Associated APE1 Protein Variants. PLoS ONE 2013, 8, e65922. [Google Scholar] [CrossRef] [PubMed]
  32. Abyzov, A.; Uzun, A.; Strauss, P.R.; Ilyin, V.A. An AP Endonuclease 1-DNA Polymerase Beta Complex: Theoretical Prediction of Interacting Surfaces. PLoS Comput. Biol. 2008, 4, e1000066. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  33. Hinz, J.M.; Mao, P.; McNeill, D.R.; Wilson, D.M. Reduced Nuclease Activity of Apurinic/Apyrimidinic Endonuclease (APE1) Variants on Nucleosomes: Identification of Access Residues. J. Biol. Chem. 2015, 290, 21067–21075. [Google Scholar] [CrossRef] [Green Version]
  34. Gao, J.; Aksoy, B.A.; Dogrusoz, U.; Dresdner, G.; Gross, B.; Sumer, S.O.; Sun, Y.; Jacobsen, A.; Sinha, R.; Larsson, E.; et al. Integrative Analysis of Complex Cancer Genomics and Clinical Profiles Using the CBioPortal. Sci. Signal. 2013, 6, pl1. [Google Scholar] [CrossRef] [Green Version]
  35. Cerami, E.; Gao, J.; Dogrusoz, U.; Gross, B.E.; Sumer, S.O.; Aksoy, B.A.; Jacobsen, A.; Byrne, C.J.; Heuer, M.L.; Larsson, E.; et al. The CBio Cancer Genomics Portal: An Open Platform for Exploring Multidimensional Cancer Genomics Data. Cancer Discov. 2012, 2, 401–404. [Google Scholar] [CrossRef] [Green Version]
  36. Reva, B.; Antipin, Y.; Sander, C. Predicting the Functional Impact of Protein Mutations: Application to Cancer Genomics. Nucleic Acids Res. 2011, 39, e118. [Google Scholar] [CrossRef] [Green Version]
  37. Reva, B.; Antipin, Y.; Sander, C. Determinants of Protein Function Revealed by Combinatorial Entropy Optimization. Genome Biol. 2007, 8, R232. [Google Scholar] [CrossRef] [Green Version]
  38. Choi, S.; Shin, J.H.; Lee, Y.R.; Joo, H.K.; Song, K.H.; Na, Y.G.; Chang, S.J.; Lim, J.S.; Jeon, B.H. Urinary APE1/Ref-1: A Potential Bladder Cancer Biomarker. Dis. Markers 2016, 2016, 7276502. [Google Scholar] [CrossRef] [Green Version]
  39. Fishel, M.L.; Xia, H.; McGeown, J.; McIlwain, D.W.; Elbanna, M.; Craft, A.A.; Kaimakliotis, H.Z.; Sandusky, G.E.; Zhang, C.; Pili, R.; et al. Antitumor Activity and Mechanistic Characterization of APE1/Ref-1 Inhibitors in Bladder Cancer. Mol. Cancer Ther. 2019, 18, 1947–1960. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  40. Shin, J.H.; Choi, S.; Lee, Y.R.; Park, M.S.; Na, Y.G.; Irani, K.; Lee, S.D.; Park, J.B.; Kim, J.M.; Lim, J.S.; et al. APE1/Ref-1 as a Serological Biomarker for the Detection of Bladder Cancer. Cancer Res. Treat. 2015, 47, 823–833. [Google Scholar] [CrossRef] [Green Version]
  41. Song, H.; Zeng, J.; Lele, S.; LaGrange, C.A.; Bhakat, K.K. APE1 and SSRP1 Is Overexpressed in Muscle Invasive Bladder Cancer and Associated with Poor Survival. Heliyon 2021, 7, e06756. [Google Scholar] [CrossRef] [PubMed]
  42. Wang, L.-A.; Yang, B.; Tang, T.; Yang, Y.; Zhang, D.; Xiao, H.; Xu, J.; Wang, L.; Lin, L.; Jiang, J. Correlation of APE1 with VEGFA and CD163+ Macrophage Infiltration in Bladder Cancer and Their Prognostic Significance. Oncol. Lett. 2020, 20, 2881–2887. [Google Scholar] [CrossRef]
  43. Güllü Amuran, G.; Tinay, I.; Filinte, D.; Ilgin, C.; Peker Eyüboğlu, I.; Akkiprik, M. Urinary micro-RNA Expressions and Protein Concentrations May Differentiate Bladder Cancer Patients from Healthy Controls. Int. Urol. Nephrol. 2020, 52, 461–468. [Google Scholar] [CrossRef] [PubMed]
  44. Kumar, M.; Shukla, V.K.; Misra, P.K.; Raman, M.J. Dysregulated Expression and Subcellular Localization of Base Excision Repair (BER) Pathway Enzymes in Gallbladder Cancer. Int. J. Mol. Cell. Med. 2018, 7, 119–132. [Google Scholar] [CrossRef] [PubMed]
  45. Chen, T.; Liu, C.; Lu, H.; Yin, M.; Shao, C.; Hu, X.; Wu, J.; Wang, Y. The Expression of APE1 in Triple-Negative Breast Cancer and Its Effect on Drug Sensitivity of Olaparib. Tumour Biol. 2017, 39, 1010428317713390. [Google Scholar] [CrossRef] [Green Version]
  46. Woo, J.; Park, H.; Sung, S.H.; Moon, B.-I.; Suh, H.; Lim, W. Prognostic Value of Human Apurinic/Apyrimidinic Endonuclease 1 (APE1) Expression in Breast Cancer. PLoS ONE 2014, 9, e99528. [Google Scholar] [CrossRef]
  47. Jian, D.; Li, X.-M.; Dai, N.; Liang, D.-D.; Zhang, G.; Mao, C.-Y.; Wang, D.; Song, G.-B.; Li, M.-X.; Luo, H. Inhibition of APE1 Expression Enhances the Antitumor Activity of Olaparib in Triple-Negative Breast Cancer. Evid.-Based Complement. Altern. Med. 2022, 2022, 6048017. [Google Scholar] [CrossRef]
  48. Poletto, M.; Di Loreto, C.; Marasco, D.; Poletto, E.; Puglisi, F.; Damante, G.; Tell, G. Acetylation on Critical Lysine Residues of Apurinic/Apyrimidinic Endonuclease 1 (APE1) in Triple Negative Breast Cancers. Biochem. Biophys. Res. Commun. 2012, 424, 34–39. [Google Scholar] [CrossRef]
  49. Malfatti, M.C.; Gerratana, L.; Dalla, E.; Isola, M.; Damante, G.; Di Loreto, C.; Puglisi, F.; Tell, G. APE1 and NPM1 Protect Cancer Cells from Platinum Compounds Cytotoxicity and Their Expression Pattern Has a Prognostic Value in TNBC. J. Exp. Clin. Cancer Res. 2019, 38, 309. [Google Scholar] [CrossRef] [Green Version]
  50. Abdel-Fatah, T.M.A.; Perry, C.; Moseley, P.; Johnson, K.; Arora, A.; Chan, S.; Ellis, I.O.; Madhusudan, S. Clinicopathological Significance of Human Apurinic/Apyrimidinic Endonuclease 1 (APE1) Expression in Oestrogen-Receptor-Positive Breast Cancer. Breast Cancer Res. Treat. 2014, 143, 411–421. [Google Scholar] [CrossRef]
  51. Herring, C.J.; West, C.M.L.; Wilks, D.P.; Davidson, S.E.; Hunter, R.D.; Berry, P.; Forster, G.; MacKinnon, J.; Rafferty, J.A.; Elder, R.H.; et al. Levels of the DNA Repair Enzyme Human Apurinic/Apyrimidinic Endonuclease (APE1, APEX, Ref-1) Are Associated with the Intrinsic Radiosensitivity of Cervical Cancers. Br. J. Cancer 1998, 78, 1128–1133. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  52. Schindl, M.; Oberhuber, G.; Pichlbauer, E.G.; Obermair, A.; Birner, P.; Kelley, M.R. DNA Repair-Redox Enzyme Apurinic Endonuclease in Cervical Cancer: Evaluation of Redox Control of HIF-1alpha and Prognostic Significance. Int. J. Oncol. 2001, 19, 799–802. [Google Scholar] [CrossRef] [PubMed]
  53. Li, Q.; Wei, X.; Zhou, Z.-W.; Wang, S.-N.; Jin, H.; Chen, K.-J.; Luo, J.; Westover, K.D.; Wang, J.-M.; Wang, D.; et al. GADD45α Sensitizes Cervical Cancer Cells to Radiotherapy via Increasing Cytoplasmic APE1 Level. Cell Death Dis. 2018, 9, 524. [Google Scholar] [CrossRef] [PubMed]
  54. Li, Q.; Zhou, Z.-W.; Duan, W.; Qian, C.-Y.; Wang, S.-N.; Deng, M.-S.; Zi, D.; Wang, J.-M.; Mao, C.-Y.; Song, G.; et al. Inhibiting the Redox Function of APE1 Suppresses Cervical Cancer Metastasis via Disengagement of ZEB1 from E-Cadherin in EMT. J. Exp. Clin. Cancer Res. 2021, 40, 220. [Google Scholar] [CrossRef] [PubMed]
  55. Bhakat, K.K.; Sengupta, S.; Adeniyi, V.F.; Roychoudhury, S.; Nath, S.; Bellot, L.J.; Feng, D.; Mantha, A.K.; Sinha, M.; Qiu, S.; et al. Regulation of Limited N-Terminal Proteolysis of APE1 in Tumor via Acetylation and Its Role in Cell Proliferation. Oncotarget 2016, 7, 22590–22604. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  56. Kakolyris, S.; Kaklamanis, L.; Engels, K.; Turley, H.; Hickson, I.D.; Gatter, K.C.; Harris, A.L. Human Apurinic Endonuclease 1 Expression in a Colorectal Adenoma-Carcinoma Sequence. Cancer Res. 1997, 57, 1794–1797. [Google Scholar]
  57. Lou, D.; Zhu, L.; Ding, H.; Dai, H.-Y.; Zou, G.-M. Aberrant Expression of Redox Protein Ape1 in Colon Cancer Stem Cells. Oncol. Lett. 2014, 7, 1078–1082. [Google Scholar] [CrossRef] [Green Version]
  58. Codrich, M.; Comelli, M.; Malfatti, M.C.; Mio, C.; Ayyildiz, D.; Zhang, C.; Kelley, M.R.; Terrosu, G.; Pucillo, C.E.M.; Tell, G. Inhibition of APE1-Endonuclease Activity Affects Cell Metabolism in Colon Cancer Cells via a P53-Dependent Pathway. DNA Repair 2019, 82, 102675. [Google Scholar] [CrossRef]
  59. Kühl Svoboda Baldin, R.; Austrália Paredes Marcondes Ribas, C.; de Noronha, L.; Veloso da Silva-Camargo, C.C.; Santos Sotomaior, V.; Martins Sebastião, A.P.; Vasconcelos de Castilho, A.P.; Rodrigues Montemor Netto, M. Expression of Parkin, APC, APE1, and Bcl-XL in Colorectal Polyps. J. Histochem. Cytochem. 2021, 69, 437–449. [Google Scholar] [CrossRef]
  60. Noike, T.; Miwa, S.; Soeda, J.; Kobayashi, A.; Miyagawa, S. Increased Expression of Thioredoxin-1, Vascular Endothelial Growth Factor, and Redox Factor-1 Is Associated with Poor Prognosis in Patients with Liver Metastasis from Colorectal Cancer. Hum. Pathol. 2008, 39, 201–208. [Google Scholar] [CrossRef]
  61. Song, H.; Zeng, J.; Roychoudhury, S.; Biswas, P.; Mohapatra, B.; Ray, S.; Dowlatshahi, K.; Wang, J.; Band, V.; Talmon, G.; et al. Targeting Histone Chaperone FACT Complex Overcomes 5-Fluorouracil Resistance in Colon Cancer. Mol. Cancer Ther. 2020, 19, 258–269. [Google Scholar] [CrossRef] [Green Version]
  62. Huajun, W.; Ying, F.; Hongxing, Z.; Weifeng, S.; Pingyang, S.; Mingde, H.; Guoguang, L. Clinical Value of Combined Detection of Serum APE1-Aabs and CEACAM-1 in the Diagnosis of Colorectal Cancer. Eur. Rev. Med. Pharmacol. Sci. 2018, 22, 1286–1289. [Google Scholar] [CrossRef] [PubMed]
  63. Deng, X.; Zhen, P.; Niu, X.; Dai, Y.; Wang, Y.; Zhou, M. APE1 Promotes Proliferation and Migration of Cutaneous Squamous Cell Carcinoma. J. Dermatol. Sci. 2020, 100, 67–74. [Google Scholar] [CrossRef]
  64. Ajucarmelprecilla, A.; Pandi, J.; Dhandapani, R.; Ramanathan, S.; Chinnappan, J.; Paramasivam, R.; Thangavelu, S.; Mohammed Ghilan, A.-K.; Aljohani, S.A.S.; Oyouni, A.A.A.; et al. In Silico Identification of Hub Genes as Observing Biomarkers for Gastric Cancer Metastasis. Evid.-Based Complement. Altern. Med. 2022, 2022, 6316158. [Google Scholar] [CrossRef] [PubMed]
  65. Manoel-Caetano, F.S.; Rossi, A.F.T.; Calvet de Morais, G.; Severino, F.E.; Silva, A.E. Upregulation of the APE1 and H2AX Genes and miRNAs Involved in DNA Damage Response and Repair in Gastric Cancer. Genes Dis. 2019, 6, 176–184. [Google Scholar] [CrossRef] [PubMed]
  66. Qing, Y.; Li, Q.; Ren, T.; Xia, W.; Peng, Y.; Liu, G.-L.; Luo, H.; Yang, Y.-X.; Dai, X.-Y.; Zhou, S.-F.; et al. Upregulation of PD-L1 and APE1 Is Associated with Tumorigenesis and Poor Prognosis of Gastric Cancer. Drug Des. Dev. Ther. 2015, 9, 901–909. [Google Scholar] [CrossRef] [Green Version]
  67. Wei, X.; Li, Y.-B.; Li, Y.; Lin, B.-C.; Shen, X.-M.; Cui, R.-L.; Gu, Y.-J.; Gao, M.; Li, Y.-G.; Zhang, S. Prediction of Lymph Node Metastases in Gastric Cancer by Serum APE1 Expression. J. Cancer 2017, 8, 1492–1497. [Google Scholar] [CrossRef]
  68. Bobola, M.S.; Blank, A.; Berger, M.S.; Stevens, B.A.; Silber, J.R. Apurinic/Apyrimidinic Endonuclease Activity Is Elevated in Human Adult Gliomas. Clin. Cancer Res. 2001, 7, 3510–3518. [Google Scholar]
  69. Scott, T.L.; Wicker, C.A.; Suganya, R.; Dhar, B.; Pittman, T.; Horbinski, C.; Izumi, T. Polyubiquitination of Apurinic/Apyrimidinic Endonuclease 1 by Parkin. Mol. Carcinog. 2017, 56, 325–336. [Google Scholar] [CrossRef] [Green Version]
  70. Naidu, M.D.; Mason, J.M.; Pica, R.V.; Fung, H.; Peña, L.A. Radiation Resistance in Glioma Cells Determined by DNA Damage Repair Activity of Ape1/Ref-1. J. Radiat. Res. 2010, 51, 393–404. [Google Scholar] [CrossRef] [Green Version]
  71. Hudson, A.L.; Parker, N.R.; Khong, P.; Parkinson, J.F.; Dwight, T.; Ikin, R.J.; Zhu, Y.; Chen, J.; Wheeler, H.R.; Howell, V.M. Glioblastoma Recurrence Correlates With Increased APE1 and Polarization Toward an Immuno-Suppressive Microenvironment. Front. Oncol. 2018, 8, 314. [Google Scholar] [CrossRef] [PubMed]
  72. Wang, Q.; Xiao, H.; Luo, Q.; Li, M.; Wei, S.; Zhu, X.; Xiao, H.; Chen, L. Low APE1/Ref-1 Expression Significantly Correlates with MGMT Promoter Methylation in Patients with High-Grade Gliomas. Int. J. Clin. Exp. Pathol. 2016, 9, 9562–9568. [Google Scholar]
  73. Perry, C.; Agarwal, D.; Abdel-Fatah, T.M.A.; Lourdusamy, A.; Grundy, R.; Auer, D.T.; Walker, D.; Lakhani, R.; Scott, I.S.; Chan, S.; et al. Dissecting DNA Repair in Adult High Grade Gliomas for Patient Stratification in the Post-Genomic Era. Oncotarget 2014, 5, 5764–5781. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  74. Hsia, K.-T.; Liu, C.-J.; Mar, K.; Lin, L.-H.; Lin, C.-S.; Cheng, M.-F.; Lee, H.-S.; Chiu, S.-Y. Impact of Apurinic/Apyrimidinic Endonuclease 1/Redox Factor-1 on Treatment Response and Survival in Oral Squamous Cell Carcinoma. Head Neck 2016, 38, 550–559. [Google Scholar] [CrossRef]
  75. Wicker, C.A.; Takiar, V.; Suganya, R.; Arnold, S.M.; Brill, Y.M.; Chen, L.; Horbinski, C.M.; Napier, D.; Valentino, J.; Kudrimoti, M.R.; et al. Evaluation of Antioxidant Network Proteins as Novel Prognostic Biomarkers for Head and Neck Cancer Patients. Oral. Oncol. 2020, 111, 104949. [Google Scholar] [CrossRef]
  76. Santana, T.; Sá, M.C.; de Moura Santos, E.; Galvão, H.C.; Coletta, R.D.; Freitas, R. de A. DNA Base Excision Repair Proteins APE-1 and XRCC-1 Are Overexpressed in Oral Tongue Squamous Cell Carcinoma. J. Oral. Pathol. Med. 2017, 46, 496–503. [Google Scholar] [CrossRef]
  77. Xie, J.; Li, Y.; Kong, J.; Li, C. Apurinic/Apyrimidinic Endonuclease 1/Redox Factor-1 Could Serve as a Potential Serological Biomarker for the Diagnosis and Prognosis of Oral Squamous Cell Carcinoma. J. Oral Maxillofac. Surg. 2019, 77, 859–866. [Google Scholar] [CrossRef]
  78. Wang, J.; Lun, L.; Jiang, X.; Wang, Y.; Li, X.; Du, G.; Wang, J. APE1 Facilitates PD-L1-Mediated Progression of Laryngeal and Hypopharyngeal Squamous Cell Carcinoma. Int. Immunopharmacol. 2021, 97, 107675. [Google Scholar] [CrossRef]
  79. Lee, J.W.; Jin, J.; Rha, K.-S.; Kim, Y.M. Expression Pattern of Apurinic/Apyrimidinic Endonuclease in Sinonasal Squamous Cell Carcinoma. Otolaryngol. Head Neck Surg. 2012, 147, 788–795. [Google Scholar] [CrossRef]
  80. Souza, L.R.; Fonseca-Silva, T.; Pereira, C.S.; Santos, E.P.; Lima, L.C.; Carvalho, H.A.; Gomez, R.S.; Guimarães, A.L.S.; De Paula, A.M.B. Immunohistochemical Analysis of P53, APE1, HMSH2 and ERCC1 Proteins in Actinic Cheilitis and Lip Squamous Cell Carcinoma. Histopathology 2011, 58, 352–360. [Google Scholar] [CrossRef]
  81. Di Maso, V.; Mediavilla, M.G.; Vascotto, C.; Lupo, F.; Baccarani, U.; Avellini, C.; Tell, G.; Tiribelli, C.; Crocè, L.S. Transcriptional Up-Regulation of APE1/Ref-1 in Hepatic Tumor: Role in Hepatocytes Resistance to Oxidative Stress and Apoptosis. PLoS ONE 2015, 10, e0143289. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  82. Sun, Z.; Zhu, Y.; Aminbuhe; Fan, Q.; Peng, J.; Zhang, N. Differential Expression of APE1 in Hepatocellular Carcinoma and the Effects on Proliferation and Apoptosis of Cancer Cells. BST 2018, 12, 456–462. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  83. Lu, X.; Zhao, H.; Yuan, H.; Chu, Y.; Zhu, X. High Nuclear Expression of APE1 Correlates with Unfavorable Prognosis and Promotes Tumor Growth in Hepatocellular Carcinoma. J. Mol. Histol. 2021, 52, 219–231. [Google Scholar] [CrossRef] [PubMed]
  84. Pascut, D.; Sukowati, C.H.C.; Antoniali, G.; Mangiapane, G.; Burra, S.; Mascaretti, L.G.; Buonocore, M.R.; Crocè, L.S.; Tiribelli, C.; Tell, G. Serum AP-Endonuclease 1 (SAPE1) as Novel Biomarker for Hepatocellular Carcinoma. Oncotarget 2019, 10, 383–394. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  85. Di Maso, V.; Avellini, C.; Crocè, L.S.; Rosso, N.; Quadrifoglio, F.; Cesaratto, L.; Codarin, E.; Bedogni, G.; Beltrami, C.A.; Tell, G.; et al. Subcellular Localization of APE1/Ref-1 in Human Hepatocellular Carcinoma: Possible Prognostic Significance. Mol. Med. 2007, 13, 89–96. [Google Scholar] [CrossRef]
  86. Bazzani, V.; Barchiesi, A.; Radecka, D.; Pravisani, R.; Guadagno, A.; Di Loreto, C.; Baccarani, U.; Vascotto, C. Mitochondrial Apurinic/Apyrimidinic Endonuclease 1 Enhances MtDNA Repair Contributing to Cell Proliferation and Mitochondrial Integrity in Early Stages of Hepatocellular Carcinoma. BMC Cancer 2020, 20, 969. [Google Scholar] [CrossRef]
  87. Sengupta, S.; Mantha, A.K.; Song, H.; Roychoudhury, S.; Nath, S.; Ray, S.; Bhakat, K.K. Elevated Level of Acetylation of APE1 in Tumor Cells Modulates DNA Damage Repair. Oncotarget 2016, 7, 75197–75209. [Google Scholar] [CrossRef] [Green Version]
  88. Long, K.; Gu, L.; Li, L.; Zhang, Z.; Li, E.; Zhang, Y.; He, L.; Pan, F.; Guo, Z.; Hu, Z. Small-Molecule Inhibition of APE1 Induces Apoptosis, Pyroptosis, and Necroptosis in Non-Small Cell Lung Cancer. Cell Death Dis. 2021, 12, 503. [Google Scholar] [CrossRef]
  89. Yoo, D.G.; Song, Y.J.; Cho, E.J.; Lee, S.K.; Park, J.B.; Yu, J.H.; Lim, S.P.; Kim, J.M.; Jeon, B.H. Alteration of APE1/Ref-1 Expression in Non-Small Cell Lung Cancer: The Implications of Impaired Extracellular Superoxide Dismutase and Catalase Antioxidant Systems. Lung Cancer 2008, 60, 277–284. [Google Scholar] [CrossRef]
  90. Wei, X.; Li, Q.; Li, Y.; Duan, W.; Huang, C.; Zheng, X.; Sun, L.; Luo, J.; Wang, D.; Zhang, S.; et al. Prediction of Survival Prognosis of Non-Small Cell Lung Cancer by APE1 through Regulation of Epithelial-Mesenchymal Transition. Oncotarget 2016, 7, 28523–28539. [Google Scholar] [CrossRef]
  91. Gu, X.; Cun, Y.; Li, M.; Qing, Y.; Jin, F.; Zhong, Z.; Dai, N.; Qian, C.; Sui, J.; Wang, D. Human Apurinic/Apyrimidinic Endonuclease SiRNA Inhibits the Angiogenesis Induced by X-Ray Irradiation in Lung Cancer Cells. Int. J. Med. Sci. 2013, 10, 870–882. [Google Scholar] [CrossRef] [Green Version]
  92. Zhang, S.; He, L.; Dai, N.; Guan, W.; Shan, J.; Yang, X.; Zhong, Z.; Qing, Y.; Jin, F.; Chen, C.; et al. Serum APE1 as a Predictive Marker for Platinum-Based Chemotherapy of Non-Small Cell Lung Cancer Patients. Oncotarget 2016, 7, 77482–77494. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  93. Kakolyris, S.; Giatromanolaki, A.; Koukourakis, M.; Kaklamanis, L.; Kanavaros, P.; Hickson, I.D.; Barzilay, G.; Georgoulias, V.; Gatter, K.C.; Harris, A.L. Nuclear Localization of Human AP Endonuclease 1 (HAP1/Ref-1) Associates with Prognosis in Early Operable Non-Small Cell Lung Cancer (NSCLC). J. Pathol. 1999, 189, 351–357. [Google Scholar] [CrossRef]
  94. Puglisi, F.; Aprile, G.; Minisini, A.M.; Barbone, F.; Cataldi, P.; Tell, G.; Kelley, M.R.; Damante, G.; Beltrami, C.A.; Di Loreto, C. Prognostic Significance of Ape1/Ref-1 Subcellular Localization in Non-Small Cell Lung Carcinomas. Anticancer Res. 2001, 21, 4041–4049. [Google Scholar] [PubMed]
  95. Wu, H.-H.; Chu, Y.-C.; Wang, L.; Tsai, L.-H.; Lee, M.-C.; Chen, C.-Y.; Shieh, S.-H.; Cheng, Y.-W.; Lee, H. Cytoplasmic Ape1 Expression Elevated by P53 Aberration May Predict Survival and Relapse in Resected Non-Small Cell Lung Cancer. Ann. Surg. Oncol. 2013, 20 (Suppl. 3), S336–S347. [Google Scholar] [CrossRef]
  96. Wu, H.-H.; Cheng, Y.-W.; Chang, J.T.; Wu, T.-C.; Liu, W.-S.; Chen, C.-Y.; Lee, H. Subcellular Localization of Apurinic Endonuclease 1 Promotes Lung Tumor Aggressiveness via NF-κB Activation. Oncogene 2010, 29, 4330–4340. [Google Scholar] [CrossRef] [Green Version]
  97. Abbotts, R.; Jewell, R.; Nsengimana, J.; Maloney, D.J.; Simeonov, A.; Seedhouse, C.; Elliott, F.; Laye, J.; Walker, C.; Jadhav, A.; et al. Targeting Human Apurinic/Apyrimidinic Endonuclease 1 (APE1) in Phosphatase and Tensin Homolog (PTEN) Deficient Melanoma Cells for Personalized Therapy. Oncotarget 2014, 5, 3273–3286. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  98. Mohammed, M.Z.; Vyjayanti, V.N.; Laughton, C.A.; Dekker, L.V.; Fischer, P.M.; Wilson, D.M.; Abbotts, R.; Shah, S.; Patel, P.M.; Hickson, I.D.; et al. Development and Evaluation of Human AP Endonuclease Inhibitors in Melanoma and Glioma Cell Lines. Br. J. Cancer 2011, 104, 653–663. [Google Scholar] [CrossRef] [Green Version]
  99. Yang, S.; Irani, K.; Heffron, S.E.; Jurnak, F.; Meyskens, F.L. Alterations in the Expression of the Apurinic/Apyrimidinic Endonuclease-1/Redox Factor-1 (APE/Ref-1) in Human Melanoma and Identification of the Therapeutic Potential of Resveratrol as an APE/Ref-1 Inhibitor. Mol. Cancer Ther. 2005, 4, 1923–1935. [Google Scholar] [CrossRef] [Green Version]
  100. Guida, M.; Tommasi, S.; Strippoli, S.; Natalicchio, M.I.; De Summa, S.; Pinto, R.; Cramarossa, A.; Albano, A.; Pisconti, S.; Aieta, M.; et al. The Search for a Melanoma-Tailored Chemotherapy in the New Era of Personalized Therapy: A Phase II Study of Chemo-Modulating Temozolomide Followed by Fotemustine and a Cooperative Study of GOIM (Gruppo Oncologico Italia Meridionale). BMC Cancer 2018, 18, 552. [Google Scholar] [CrossRef] [Green Version]
  101. Al-Attar, A.; Gossage, L.; Fareed, K.R.; Shehata, M.; Mohammed, M.; Zaitoun, A.M.; Soomro, I.; Lobo, D.N.; Abbotts, R.; Chan, S.; et al. Human Apurinic/Apyrimidinic Endonuclease (APE1) Is a Prognostic Factor in Ovarian, Gastro-Oesophageal and Pancreatico-Biliary Cancers. Br. J. Cancer 2010, 102, 704–709. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  102. Hong, J.; Chen, Z.; Peng, D.; Zaika, A.; Revetta, F.; Washington, M.K.; Belkhiri, A.; El-Rifai, W. APE1-Mediated DNA Damage Repair Provides Survival Advantage for Esophageal Adenocarcinoma Cells in Response to Acidic Bile Salts. Oncotarget 2016, 7, 16688–16702. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  103. Bhat, A.A.; Lu, H.; Soutto, M.; Capobianco, A.; Rai, P.; Zaika, A.; El-Rifai, W. Exposure of Barrett’s and Esophageal Adenocarcinoma Cells to Bile Acids Activates EGFR-STAT3 Signaling Axis via Induction of APE1. Oncogene 2018, 37, 6011–6024. [Google Scholar] [CrossRef] [PubMed]
  104. Sriramajayam, K.; Peng, D.; Lu, H.; Zhou, S.; Bhat, N.; McDonald, O.G.; Que, J.; Zaika, A.; El-Rifai, W. Activation of NRF2 by APE1/REF1 Is Redox-Dependent in Barrett’s Related Esophageal Adenocarcinoma Cells. Redox Biol. 2021, 43, 101970. [Google Scholar] [CrossRef]
  105. Han, G.; Tian, Y.; Duan, B.; Sheng, H.; Gao, H.; Huang, J. Association of Nuclear Annexin A1 with Prognosis of Patients with Esophageal Squamous Cell Carcinoma. Int. J. Clin. Exp. Pathol. 2014, 7, 751–759. [Google Scholar]
  106. Song, J.; Futagami, S.; Nagoya, H.; Kawagoe, T.; Yamawaki, H.; Kodaka, Y.; Tatsuguchi, A.; Gudis, K.; Wakabayashi, T.; Yonezawa, M.; et al. Apurinic/Apyrimidinic Endonuclease-1 (APE-1) Is Overexpressed via the Activation of NF-κB-P65 in MCP-1-Positive Esophageal Squamous Cell Carcinoma Tissue. J. Clin. Biochem. Nutr. 2013, 52, 112–119. [Google Scholar] [CrossRef] [Green Version]
  107. Liu, Y.; Zhang, Z.; Li, Q.; Zhang, L.; Cheng, Y.; Zhong, Z. Mitochondrial APE1 Promotes Cisplatin Resistance by Downregulating ROS in Osteosarcoma. Oncol. Rep. 2020, 44, 499–508. [Google Scholar] [CrossRef]
  108. Liu, Y.; Zhang, Z.; Zhang, L.; Zhong, Z. Cytoplasmic APE1 Promotes Resistance Response in Osteosarcoma Patients with Cisplatin Treatment. Cell Biochem. Funct. 2020, 38, 195–203. [Google Scholar] [CrossRef]
  109. Wang, D.; Luo, M.; Kelley, M.R. Human Apurinic Endonuclease 1 (APE1) Expression and Prognostic Significance in Osteosarcoma: Enhanced Sensitivity of Osteosarcoma to DNA Damaging Agents Using Silencing RNA APE1 Expression Inhibition. Mol. Cancer Ther. 2004, 3, 679–686. [Google Scholar] [CrossRef]
  110. Chen, Y.; Yang, Y.; Yuan, Z.; Wang, C.; Shi, Y. Predicting Chemosensitivity in Osteosarcoma Prior to Chemotherapy: An Investigational Study of Biomarkers with Immunohistochemistry. Oncol. Lett. 2012, 3, 1011–1016. [Google Scholar] [CrossRef] [Green Version]
  111. Ren, T.; Qing, Y.; Dai, N.; Li, M.; Qian, C.; Yang, Y.; Cheng, Y.; Li, Z.; Zhang, S.; Zhong, Z.; et al. Apurinic/Apyrimidinic Endonuclease 1 Induced Upregulation of Fibroblast Growth Factor 2 and Its Receptor 3 Induces Angiogenesis in Human Osteosarcoma Cells. Cancer Sci. 2014, 105, 186–194. [Google Scholar] [CrossRef] [PubMed]
  112. Jiang, X.; Shan, J.; Dai, N.; Zhong, Z.; Qing, Y.; Yang, Y.; Zhang, S.; Li, C.; Sui, J.; Ren, T.; et al. Apurinic/Apyrimidinic Endonuclease 1 Regulates Angiogenesis in a Transforming Growth Factor β-Dependent Manner in Human Osteosarcoma. Cancer Sci. 2015, 106, 1394–1401. [Google Scholar] [CrossRef] [Green Version]
  113. Dai, N.; Qing, Y.; Cun, Y.; Zhong, Z.; Li, C.; Zhang, S.; Shan, J.; Yang, X.; Dai, X.; Cheng, Y.; et al. MiR-513a-5p Regulates Radiosensitivity of Osteosarcoma by Targeting Human Apurinic/Apyrimidinic Endonuclease. Oncotarget 2016, 9, 25414–25426. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  114. Londero, A.P.; Orsaria, M.; Tell, G.; Marzinotto, S.; Capodicasa, V.; Poletto, M.; Vascotto, C.; Sacco, C.; Mariuzzi, L. Expression and Prognostic Significance of APE1/Ref-1 and NPM1 Proteins in High-Grade Ovarian Serous Cancer. Am. J. Clin. Pathol. 2014, 141, 404–414. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  115. Wen, X.; Lu, R.; Xie, S.; Zheng, H.; Wang, H.; Wang, Y.; Sun, J.; Gao, X.; Guo, L. APE1 Overexpression Promotes the Progression of Ovarian Cancer and Serves as a Potential Therapeutic Target. Cancer Biomark. 2016, 17, 313–322. [Google Scholar] [CrossRef] [PubMed]
  116. Zhang, Y.; Wang, J.; Xiang, D.; Wang, D.; Xin, X. Alterations in the Expression of the Apurinic/Apyrimidinic Endonuclease-1/Redox Factor-1 (APE1/Ref-1) in Human Ovarian Cancer and Indentification of the Therapeutic Potential of APE1/Ref-1 Inhibitor. Int. J. Oncol. 2009, 35, 1069–1079. [Google Scholar]
  117. Fan, X.; Wen, L.; Li, Y.; Lou, L.; Liu, W.; Zhang, J. The Expression Profile and Prognostic Value of APE/Ref-1 and NPM1 in High-Grade Serous Ovarian Adenocarcinoma. APMIS 2017, 125, 857–862. [Google Scholar] [CrossRef]
  118. Poletto, M.; Malfatti, M.C.; Dorjsuren, D.; Scognamiglio, P.L.; Marasco, D.; Vascotto, C.; Jadhav, A.; Maloney, D.J.; Wilson, D.M.; Simeonov, A.; et al. Inhibitors of the Apurinic/Apyrimidinic Endonuclease 1 (APE1)/Nucleophosmin (NPM1) Interaction That Display Anti-Tumor Properties. Mol. Carcinog. 2016, 55, 688–704. [Google Scholar] [CrossRef] [Green Version]
  119. Sheng, Q.; Zhang, Y.; Wang, R.; Zhang, J.; Chen, B.; Wang, J.; Zhang, W.; Xin, X. Prognostic Significance of APE1 Cytoplasmic Localization in Human Epithelial Ovarian Cancer. Med. Oncol. 2012, 29, 1265–1271. [Google Scholar] [CrossRef]
  120. Moore, D.H.; Michael, H.; Tritt, R.; Parsons, S.H.; Kelley, M.R. Alterations in the Expression of the DNA Repair/Redox Enzyme APE/Ref-1 in Epithelial Ovarian Cancers. Clin. Cancer Res. 2000, 6, 602–609. [Google Scholar]
  121. Tanner, B.; Grimme, S.; Schiffer, I.; Heimerdinger, C.; Schmidt, M.; Dutkowski, P.; Neubert, S.; Oesch, F.; Franzen, A.; Kölbl, H.; et al. Nuclear Expression of Apurinic/Apyrimidinic Endonuclease Increases with Progression of Ovarian Carcinomas. Gynecol. Oncol. 2004, 92, 568–577. [Google Scholar] [CrossRef]
  122. Pramanik, S.; Chen, Y.; Song, H.; Khutsishvili, I.; Marky, L.A.; Ray, S.; Natarajan, A.; Singh, P.K.; Bhakat, K.K. The Human AP-Endonuclease 1 (APE1) Is a DNA G-Quadruplex Structure Binding Protein and Regulates KRAS Expression in Pancreatic Ductal Adenocarcinoma Cells. Nucleic Acids Res. 2022, 50, 3394–3412. [Google Scholar] [CrossRef]
  123. Jiang, Y.; Zhou, S.; Sandusky, G.E.; Kelley, M.R.; Fishel, M.L. Reduced Expression of DNA Repair and Redox Signaling Protein APE1/Ref-1 Impairs Human Pancreatic Cancer Cell Survival, Proliferation, and Cell Cycle Progression. Cancer Investig. 2010, 28, 885–895. [Google Scholar] [CrossRef] [PubMed]
  124. Fishel, M.L.; Jiang, Y.; Rajeshkumar, N.V.; Scandura, G.; Sinn, A.L.; He, Y.; Shen, C.; Jones, D.R.; Pollok, K.E.; Ivan, M.; et al. Impact of APE1/Ref-1 Redox Inhibition on Pancreatic Tumor Growth. Mol. Cancer Ther. 2011, 10, 1698–1708. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  125. Kelley, M.R.; Cheng, L.; Foster, R.; Tritt, R.; Jiang, J.; Broshears, J.; Koch, M. Elevated and Altered Expression of the Multifunctional DNA Base Excision Repair and Redox Enzyme Ape1/Ref-1 in Prostate Cancer. Clin. Cancer Res. 2001, 7, 824–830. [Google Scholar] [PubMed]
  126. Juhnke, M.; Heumann, A.; Chirico, V.; Höflmayer, D.; Menz, A.; Hinsch, A.; Hube-Magg, C.; Kluth, M.; Lang, D.S.; Möller-Koop, C.; et al. Apurinic/Apyrimidinic Endonuclease 1 (APE1/Ref-1) Overexpression Is an Independent Prognostic Marker in Prostate Cancer without TMPRSS2:ERG Fusion. Mol. Carcinog. 2017, 56, 2135–2145. [Google Scholar] [CrossRef]
  127. Silva, L.P.; Santana, T.; Sedassari, B.T.; de Sousa, S.M.; Sobral, A.P.V.; Freitas, R.d.A.; Barboza, C.A.G.; de Souza, L.B. Apurinic/Apyrimidinic Endonuclease 1 (APE1) Is Overexpressed in Malignant Transformation of Salivary Gland Pleomorphic Adenoma. Eur. Arch. Otorhinolaryngol. 2017, 274, 3203–3209. [Google Scholar] [CrossRef] [PubMed]
  128. Felix, F.A.; da Silva, L.P.; Lopes, M.L.D.d.S.; Sobral, A.P.V.; Freitas, R.d.A.; de Souza, L.B.; Barboza, C.A.G. DNA Base Excision Repair and Nucleotide Excision Repair Proteins in Malignant Salivary Gland Tumors. Arch. Oral. Biol. 2021, 121, 104987. [Google Scholar] [CrossRef]
  129. Lee, Y.R.; Lim, J.S.; Shin, J.H.; Choi, S.; Joo, H.K.; Jeon, B.H. Altered Secretory Activity of APE1/Ref-1 D148E Variants Identified in Human Patients With Bladder Cancer. Int. Neurourol. J. 2016, 20, S30–S37. [Google Scholar] [CrossRef] [Green Version]
  130. Li, M.; Wilson, D.M. Human Apurinic/Apyrimidinic Endonuclease 1. Antioxid. Redox Signal. 2014, 20, 678–707. [Google Scholar] [CrossRef] [Green Version]
  131. Castillo-Acosta, V.M.; Ruiz-Perez, L.M.; Yang, W.; Gonzalez-Pacanowska, D.; Vidal, A.E. Identification of a Residue Critical for the Excision of 3′-Blocking Ends in Apurinic/Apyrimidinic Endonucleases of the Xth Family. Nucleic Acids Res. 2009, 37, 1829–1842. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  132. Timofeyeva, N.A.; Koval, V.V.; Ishchenko, A.A.; Saparbaev, M.K.; Fedorova, O.S. Lys98 Substitution in Human AP Endonuclease 1 Affects the Kinetic Mechanism of Enzyme Action in Base Excision and Nucleotide Incision Repair Pathways. PLoS ONE 2011, 6, e24063. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  133. Whitaker, A.M.; Flynn, T.S.; Freudenthal, B.D. Molecular Snapshots of APE1 Proofreading Mismatches and Removing DNA Damage. Nat. Commun. 2018, 9, 399. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  134. Wilson, D.M.; Simeonov, A. Small Molecule Inhibitors of DNA Repair Nuclease Activities of APE1. Cell. Mol. Life Sci. 2010, 67, 3621–3631. [Google Scholar] [CrossRef] [Green Version]
  135. Al-Safi, R.I.; Odde, S.; Shabaik, Y.; Neamati, N. Small-Molecule Inhibitors of APE1 DNA Repair Function: An Overview. Curr. Mol. Pharmacol. 2012, 5, 14–35. [Google Scholar] [CrossRef]
  136. Laev, S.S.; Salakhutdinov, N.F.; Lavrik, O.I. Inhibitors of Nuclease and Redox Activity of Apurinic/Apyrimidinic Endonuclease 1/Redox Effector Factor 1 (APE1/Ref-1). Bioorg. Med. Chem. 2017, 25, 2531–2544. [Google Scholar] [CrossRef]
  137. Caston, R.A.; Gampala, S.; Armstrong, L.; Messmann, R.A.; Fishel, M.L.; Kelley, M.R. The Multifunctional APE1 DNA Repair-Redox Signaling Protein as a Drug Target in Human Disease. Drug Discov. Today 2021, 26, 218–228. [Google Scholar] [CrossRef]
  138. Xue, Z.; Demple, B. Knockout and Inhibition of Ape1: Roles of Ape1 in Base Excision DNA Repair and Modulation of Gene Expression. Antioxidants 2022, 11, 1817. [Google Scholar] [CrossRef]
  139. Liuzzi, M.; Weinfeld, M.; Paterson, M.C. Selective Inhibition by Methoxyamine of the Apurinic/Apyrimidinic Endonuclease Activity Associated with Pyrimidine Dimer-DNA Glycosylases from Micrococcus Luteus and Bacteriophage T4. Biochemistry 1987, 26, 3315–3321. [Google Scholar] [CrossRef]
  140. Liu, L.; Gerson, S.L. Therapeutic Impact of Methoxyamine: Blocking Repair of Abasic Sites in the Base Excision Repair Pathway. Curr. Opin. Investig. Drugs 2004, 5, 623–627. [Google Scholar]
  141. Liu, L.; Nakatsuru, Y.; Gerson, S.L. Base Excision Repair as a Therapeutic Target in Colon Cancer. Clin. Cancer Res. 2002, 8, 2985–2991. [Google Scholar] [PubMed]
  142. Fishel, M.L.; He, Y.; Smith, M.L.; Kelley, M.R. Manipulation of Base Excision Repair to Sensitize Ovarian Cancer Cells to Alkylating Agent Temozolomide. Clin. Cancer Res. 2007, 13, 260–267. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  143. Bases, R. Enhancement of X-Ray Damage in HeLa Cells by Exposure to Lucanthone (Miracil D) Following Radiation. Cancer Res. 1970, 30, 2007–2011. [Google Scholar] [PubMed]
  144. Luo, M.; Kelley, M.R. Inhibition of the Human Apurinic/Apyrimidinic Endonuclease (Ape1) Repair Activity and Sensitization of Breast Cancer Cells to DNA Alkylating Agents with Lucanthone. Anticancer Res. 2004, 24, 2127–2134. [Google Scholar] [PubMed]
  145. Naidu, M.D.; Agarwal, R.; Pena, L.A.; Cunha, L.; Mezei, M.; Shen, M.; Wilson, D.M.; Liu, Y.; Sanchez, Z.; Chaudhary, P.; et al. Lucanthone and Its Derivative Hycanthone Inhibit Apurinic Endonuclease-1 (APE1) by Direct Protein Binding. PLoS ONE 2011, 6, e23679. [Google Scholar] [CrossRef] [Green Version]
  146. Madhusudan, S.; Smart, F.; Shrimpton, P.; Parsons, J.L.; Gardiner, L.; Houlbrook, S.; Talbot, D.C.; Hammonds, T.; Freemont, P.A.; Sternberg, M.J.E.; et al. Isolation of a Small Molecule Inhibitor of DNA Base Excision Repair. Nucleic Acids Res. 2005, 33, 4711–4724. [Google Scholar] [CrossRef] [Green Version]
  147. Simeonov, A.; Kulkarni, A.; Dorjsuren, D.; Jadhav, A.; Shen, M.; McNeill, D.R.; Austin, C.P.; Wilson, D.M. Identification and Characterization of Inhibitors of Human Apurinic/Apyrimidinic Endonuclease APE1. PLoS ONE 2009, 4, e5740. [Google Scholar] [CrossRef] [Green Version]
  148. Yuan, Y.; Fu, D.; Xu, Y.; Wang, X.; Deng, X.; Zhou, S.; Du, F.; Cui, X.; Deng, Y.; Tang, Z. Pt(IV) Prodrug as a Potential Antitumor Agent with APE1 Inhibitory Activity. J. Med. Chem. 2022, 65, 15344–15357. [Google Scholar] [CrossRef]
  149. Seiple, L.A.; Cardellina, J.H.; Akee, R.; Stivers, J.T. Potent Inhibition of Human Apurinic/Apyrimidinic Endonuclease 1 by Arylstibonic Acids. Mol. Pharmacol. 2008, 73, 669–677. [Google Scholar] [CrossRef] [Green Version]
  150. Zawahir, Z.; Dayam, R.; Deng, J.; Pereira, C.; Neamati, N. Pharmacophore Guided Discovery of Small-Molecule Human Apurinic/Apyrimidinic Endonuclease 1 Inhibitors. J. Med. Chem. 2009, 52, 20–32. [Google Scholar] [CrossRef]
  151. Bapat, A.; Glass, L.S.; Luo, M.; Fishel, M.L.; Long, E.C.; Georgiadis, M.M.; Kelley, M.R. Novel Small-Molecule Inhibitor of Apurinic/Apyrimidinic Endonuclease 1 Blocks Proliferation and Reduces Viability of Glioblastoma Cells. J. Pharmacol. Exp. Ther. 2010, 334, 988–998. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  152. Aiello, F.; Shabaik, Y.; Esqueda, A.; Sanchez, T.W.; Grande, F.; Garofalo, A.; Neamati, N. Design and Synthesis of 3-Carbamoylbenzoic Acid Derivatives as Inhibitors of Human Apurinic/Apyrimidinic Endonuclease 1 (APE1). ChemMedChem 2012, 7, 1825–1839. [Google Scholar] [CrossRef] [PubMed]
  153. Ruiz, F.M.; Francis, S.M.; Tintoré, M.; Ferreira, R.; Gil-Redondo, R.; Morreale, A.; Ortiz, Á.R.; Eritja, R.; Fàbrega, C. Receptor-Based Virtual Screening and Biological Characterization of Human Apurinic/Apyrimidinic Endonuclease (Ape1) Inhibitors. ChemMedChem 2012, 7, 2168–2178. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  154. Dorjsuren, D.; Kim, D.; Vyjayanti, V.N.; Maloney, D.J.; Jadhav, A.; Wilson, D.M.; Simeonov, A. Diverse Small Molecule Inhibitors of Human Apurinic/Apyrimidinic Endonuclease APE1 Identified from a Screen of a Large Public Collection. PLoS ONE 2012, 7, e47974. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  155. Rai, G.; Vyjayanti, V.N.; Dorjsuren, D.; Simeonov, A.; Jadhav, A.; Wilson, D.M.; Maloney, D.J. Synthesis, Biological Evaluation, and Structure–Activity Relationships of a Novel Class of Apurinic/Apyrimidinic Endonuclease 1 Inhibitors. J. Med. Chem. 2012, 55, 3101–3112. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  156. Srinivasan, A.; Wang, L.; Cline, C.J.; Xie, Z.; Sobol, R.W.; Xie, X.-Q.; Gold, B. Identification and Characterization of Human Apurinic/Apyrimidinic Endonuclease-1 Inhibitors; American Chemical Society: Washington, DC, USA, 2012; Volume 51, ISBN 00062960. [Google Scholar]
  157. Feng, Z.; Kochanek, S.; Close, D.; Wang, L.; Srinivasan, A.; Almehizia, A.A.; Iyer, P.; Xie, X.-Q.; Johnston, P.A.; Gold, B. Design and Activity of AP Endonuclease-1 Inhibitors. J. Chem. Biol. 2015, 8, 79–93. [Google Scholar] [CrossRef] [Green Version]
  158. Trilles, R.; Beglov, D.; Chen, Q.; He, H.; Wireman, R.; Reed, A.; Chennamadhavuni, S.; Panek, J.S.; Brown, L.E.; Vajda, S.; et al. Discovery of Macrocyclic Inhibitors of Apurinic/Apyrimidinic Endonuclease 1. J. Med. Chem. 2019, 62, 1971–1988. [Google Scholar] [CrossRef]
  159. Pidugu, L.S.; Servius, H.W.; Sevdalis, S.E.; Cook, M.E.; Varney, K.M.; Pozharski, E.; Drohat, A.C. Characterizing Inhibitors of Human AP Endonuclease 1. PLoS ONE 2023, 18, e0280526. [Google Scholar] [CrossRef]
  160. Masani, S.; Han, L.; Yu, K. Apurinic/Apyrimidinic Endonuclease 1 Is the Essential Nuclease during Immunoglobulin Class Switch Recombination. Mol. Cell. Biol. 2013, 33, 1468–1473. [Google Scholar] [CrossRef] [Green Version]
  161. Georgiadis, M.M.; Luo, M.; Gaur, R.K.; Delaplane, S.; Li, X.; Kelley, M.R. Evolution of the Redox Function in Mammalian Apurinic/Apyrimidinic Endonuclease. Mutat. Res./Fundam. Mol. Mech. Mutagen. 2008, 643, 54–63. [Google Scholar] [CrossRef] [Green Version]
  162. Ando, K.; Hirao, S.; Kabe, Y.; Ogura, Y.; Sato, I.; Yamaguchi, Y.; Wada, T.; Handa, H. A New APE1/Ref-1-Dependent Pathway Leading to Reduction of NF-κB and AP-1, and Activation of Their DNA-Binding Activity. Nucleic Acids Res. 2008, 36, 4327–4336. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  163. Logsdon, D.P.; Grimard, M.; Luo, M.; Shahda, S.; Jiang, Y.; Tong, Y.; Yu, Z.; Zyromski, N.; Schipani, E.; Carta, F.; et al. Regulation of HIF1α under Hypoxia by APE1/Ref-1 Impacts CA9 Expression: Dual Targeting in Patient-Derived 3D Pancreatic Cancer Models. Mol. Cancer Ther. 2016, 15, 2722–2732. [Google Scholar] [CrossRef] [Green Version]
  164. Ray, S.; Lee, C.; Hou, T.; Bhakat, K.K.; Brasier, A.R. Regulation of Signal Transducer and Activator of Transcription 3 Enhanceosome Formation by Apurinic/Apyrimidinic Endonuclease 1 in Hepatic Acute Phase Response. Mol. Endocrinol. 2010, 24, 391–401. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  165. Cardoso, A.A.; Jiang, Y.; Luo, M.; Reed, A.M.; Shahda, S.; He, Y.; Maitra, A.; Kelley, M.R.; Fishel, M.L. APE1/Ref-1 Regulates STAT3 Transcriptional Activity and APE1/Ref-1–STAT3 Dual-Targeting Effectively Inhibits Pancreatic Cancer Cell Survival. PLoS ONE 2012, 7, e47462. [Google Scholar] [CrossRef]
  166. Jayaraman, L.; Murthy, K.G.; Zhu, C.; Curran, T.; Xanthoudakis, S.; Prives, C. Identification of Redox/Repair Protein Ref-1 as a Potent Activator of P53. Genes Dev. 1997, 11, 558–570. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  167. Fishel, M.L.; Wu, X.; Devlin, C.M.; Logsdon, D.P.; Jiang, Y.; Luo, M.; He, Y.; Yu, Z.; Tong, Y.; Lipking, K.P.; et al. Apurinic/Apyrimidinic Endonuclease/Redox Factor-1 (APE1/Ref-1) Redox Function Negatively Regulates NRF2. J. Biol. Chem. 2015, 290, 3057–3068. [Google Scholar] [CrossRef] [PubMed]
  168. Tell, G.; Scaloni, A.; Pellizzari, L.; Formisano, S.; Pucillo, C.; Damante, G. Redox Potential Controls the Structure and DNA Binding Activity of the Paired Domain. J. Biol. Chem. 1998, 273, 25062–25072. [Google Scholar] [CrossRef] [Green Version]
  169. Evans, A.R.; Limp-Foster, M.; Kelley, M.R. Going APE over Ref-1. Mutat. Res. DNA Repair 2000, 461, 83–108. [Google Scholar] [CrossRef]
  170. Xanthoudakis, S.; Curran, T. Identification and Characterization of Ref-1, a Nuclear Protein That Facilitates AP-1 DNA-Binding Activity. EMBO J. 1992, 11, 653–665. [Google Scholar] [CrossRef]
  171. Xanthoudakis, S.; Miao, G.; Wang, F.; Pan, Y.C.; Curran, T. Redox Activation of Fos-Jun DNA Binding Activity Is Mediated by a DNA Repair Enzyme. EMBO J. 1992, 11, 3323–3335. [Google Scholar] [CrossRef]
  172. Arlt, A.; Vorndamm, J.; Breitenbroich, M.; Fölsch, U.R.; Kalthoff, H.; Schmidt, W.E.; Schäfer, H. Inhibition of NF-ΚB Sensitizes Human Pancreatic Carcinoma Cells to Apoptosis Induced by Etoposide (VP16) or Doxorubicin. Oncogene 2001, 20, 859–868. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  173. Arlt, A.; Gehrz, A.; Müerköster, S.; Vorndamm, J.; Kruse, M.-L.; Fölsch, U.R.; Schäfer, H. Role of NF-ΚB and Akt/PI3K in the Resistance of Pancreatic Carcinoma Cell Lines against Gemcitabine-Induced Cell Death. Oncogene 2003, 22, 3243–3251. [Google Scholar] [CrossRef] [Green Version]
  174. Raffoul, J.J.; Heydari, A.R.; Hillman, G.G. DNA Repair and Cancer Therapy: Targeting APE1/Ref-1 Using Dietary Agents. J. Oncol. 2012, 2012, 370481. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  175. Gupta, S.C.; Patchva, S.; Aggarwal, B.B. Therapeutic Roles of Curcumin: Lessons Learned from Clinical Trials. AAPS J. 2013, 15, 195–218. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  176. Li, H.; Zhong, C.; Wang, Q.; Chen, W.; Yuan, Y. Curcumin Is an APE1 Redox Inhibitor and Exhibits an Antiviral Activity against KSHV Replication and Pathogenesis. Antivir. Res. 2019, 167, 98–103. [Google Scholar] [CrossRef]
  177. Escobar, I.; Xu, J.; Jackson, C.W.; Stegelmann, S.D.; Fagerli, E.A.; Dave, K.R.; Perez-Pinzon, M.A. Resveratrol Preconditioning Protects Against Ischemia-Induced Synaptic Dysfunction and Cofilin Hyperactivation in the Mouse Hippocampal Slice. Neurotherapeutics 2023. [Google Scholar] [CrossRef]
  178. Raffoul, J.J.; Banerjee, S.; Singh-Gupta, V.; Knoll, Z.E.; Fite, A.; Zhang, H.; Abrams, J.; Sarkar, F.H.; Hillman, G.G. Down-Regulation of Apurinic/Apyrimidinic Endonuclease 1/Redox Factor-1 Expression by Soy Isoflavones Enhances Prostate Cancer Radiotherapy In Vitro and In Vivo. Cancer Res. 2007, 67, 2141–2149. [Google Scholar] [CrossRef] [Green Version]
  179. Kelley, M.R.; Wikel, J.H.; Guo, C.; Pollok, K.E.; Bailey, B.J.; Wireman, R.; Fishel, M.L.; Vasko, M.R. Identification and Characterization of New Chemical Entities Targeting Apurinic/Apyrimidinic Endonuclease 1 for the Prevention of Chemotherapy-Induced Peripheral Neuropathy. J. Pharmacol. Exp. Ther. 2016, 359, 300–309. [Google Scholar] [CrossRef] [Green Version]
  180. Shimizu, N.; Sugimoto, K.; Tang, J.; Nishi, T.; Sato, I.; Hiramoto, M.; Aizawa, S.; Hatakeyama, M.; Ohba, R.; Hatori, H.; et al. High-Performance Affinity Beads for Identifying Drug Receptors. Nat. Biotechnol. 2000, 18, 877–881. [Google Scholar] [CrossRef]
  181. Zou, G.-M.; Karikari, C.; Kabe, Y.; Handa, H.; Anders, R.A.; Maitra, A. The Ape-1/Ref-1 Redox Antagonist E3330 Inhibits the Growth of Tumor Endothelium and Endothelial Progenitor Cells: Therapeutic Implications in Tumor Angiogenesis. J. Cell. Physiol. 2009, 219, 209–218. [Google Scholar] [CrossRef]
  182. Zou, G.-M.; Maitra, A. Small-Molecule Inhibitor of the AP Endonuclease 1/REF-1 E3330 Inhibits Pancreatic Cancer Cell Growth and Migration. Mol. Cancer Ther. 2008, 7, 2012–2021. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  183. Jiang, A.; Gao, H.; Kelley, M.R.; Qiao, X. Inhibition of APE1/Ref-1 Redox Activity with APX3330 Blocks Retinal Angiogenesis in Vitro and in Vivo. Vis. Res. 2011, 51, 93–100. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  184. Manguinhas, R.; Fernandes, A.S.; Costa, J.G.; Saraiva, N.; Camões, S.P.; Gil, N.; Rosell, R.; Castro, M.; Miranda, J.P.; Oliveira, N.G. Impact of the APE1 Redox Function Inhibitor E3330 in Non-Small Cell Lung Cancer Cells Exposed to Cisplatin: Increased Cytotoxicity and Impairment of Cell Migration and Invasion. Antioxidants 2020, 9, 550. [Google Scholar] [CrossRef] [PubMed]
  185. Guerreiro, P.S.; Corvacho, E.; Costa, J.G.; Saraiva, N.; Fernandes, A.S.; Castro, M.; Miranda, J.P.; Oliveira, N.G. The APE1 Redox Inhibitor E3330 Reduces Collective Cell Migration of Human Breast Cancer Cells and Decreases Chemoinvasion and Colony Formation When Combined with Docetaxel. Chem. Biol. Drug Des. 2017, 90, 561–571. [Google Scholar] [CrossRef]
  186. Li, Y.; Liu, X.; Zhou, T.; Kelley, M.R.; Edwards, P.A.; Gao, H.; Qiao, X. Suppression of Choroidal Neovascularization Through Inhibition of APE1/Ref-1 Redox Activity. Investig. Ophthalmol. Vis. Sci. 2014, 55, 4461–4469. [Google Scholar] [CrossRef] [PubMed]
  187. Hartman, G.D.; Lambert-Cheatham, N.A.; Kelley, M.R.; Corson, T.W. Inhibition of APE1/Ref-1 for Neovascular Eye Diseases: From Biology to Therapy. Int. J. Mol. Sci. 2021, 22, 10279. [Google Scholar] [CrossRef]
  188. Hu, J.; Wang, Y.; Yuan, Y. Inhibitors of APE1 Redox Function Effectively Inhibit γ-Herpesvirus Replication in Vitro and in Vivo. Antivir. Res. 2021, 185, 104985. [Google Scholar] [CrossRef]
  189. Shahda, S.; Lakhani, N.J.; O’Neil, B.; Rasco, D.W.; Wan, J.; Mosley, A.L.; Liu, H.; Kelley, M.R.; Messmann, R.A. A Phase I Study of the APE1 Protein Inhibitor APX3330 in Patients with Advanced Solid Tumors. JCO 2019, 37 (Suppl. 15), 3097. [Google Scholar] [CrossRef]
  190. Kelley, M.R.; Luo, M.; Reed, A.; Su, D.; Delaplane, S.; Borch, R.F.; Nyland, R.L.; Gross, M.L.; Georgiadis, M.M. Functional Analysis of Novel Analogues of E3330 That Block the Redox Signaling Activity of the Multifunctional AP Endonuclease/Redox Signaling Enzyme APE1/Ref-1. Antioxid. Redox Signal. 2011, 14, 1387–1401. [Google Scholar] [CrossRef] [Green Version]
  191. Nyland, R.L.; Luo, M.; Kelley, M.R.; Borch, R.F. Design and Synthesis of Novel Quinone Inhibitors Targeted to the Redox Function of Apurinic/Apyrimidinic Endonuclease 1/Redox Enhancing Factor-1 (Ape1/Ref-1). J. Med. Chem. 2010, 53, 1200–1210. [Google Scholar] [CrossRef] [Green Version]
  192. Qian, C.; Li, M.; Sui, J.; Ren, T.; Li, Z.; Zhang, L.; Zhou, L.; Cheng, Y.; Wang, D. Identification of a Novel Potential Antitumor Activity of Gossypol as an APE1/Ref-1 Inhibitor. Drug Des. Dev. Ther. 2014, 8, 485–496. [Google Scholar] [CrossRef] [Green Version]
  193. Wang, Y.; Li, X.; Zhang, L.; Li, M.; Dai, N.; Luo, H.; Shan, J.; Yang, X.; Xu, M.; Feng, Y.; et al. A Randomized, Double-Blind, Placebo-Controlled Study of B-Cell Lymphoma 2 Homology 3 Mimetic Gossypol Combined with Docetaxel and Cisplatin for Advanced Non-Small Cell Lung Cancer with High Expression of Apurinic/Apyrimidinic Endonuclease 1. Investig. New Drugs 2020, 38, 1862–1871. [Google Scholar] [CrossRef] [PubMed]
  194. Ren, T.; Shan, J.; Qing, Y.; Qian, C.; Li, Q.; Lu, G.; Li, M.; Li, C.; Peng, Y.; Luo, H.; et al. Sequential Treatment with AT-101 Enhances Cisplatin Chemosensitivity in Human Non-Small Cell Lung Cancer Cells through Inhibition of Apurinic/Apyrimidinic Endonuclease 1-Activated IL-6/STAT3 Signaling Pathway. Drug Des. Dev. Ther. 2014, 8, 2517–2529. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  195. Wei, X.; Duan, W.; Li, Y.; Zhang, S.; Xin, X.; Sun, L.; Gao, M.; Li, Q.; Wang, D. AT101 Exerts a Synergetic Efficacy in Gastric Cancer Patients with 5-FU Based Treatment through Promoting Apoptosis and Autophagy. Oncotarget 2016, 7, 34430–34441. [Google Scholar] [CrossRef] [Green Version]
  196. Poletto, M.; Vascotto, C.; Scognamiglio, P.L.; Lirussi, L.; Marasco, D.; Tell, G. Role of the Unstructured N-Terminal Domain of the HAPE1 (Human Apurinic/Apyrimidinic Endonuclease 1) in the Modulation of Its Interaction with Nucleic Acids and NPM1 (Nucleophosmin). Biochem. J. 2013, 452, 545–557. [Google Scholar] [CrossRef] [Green Version]
  197. Antoniali, G.; Dalla, E.; Mangiapane, G.; Zhao, X.; Jing, X.; Cheng, Y.; De Sanctis, V.; Ayyildiz, D.; Piazza, S.; Li, M.; et al. APE1 Controls DICER1 Expression in NSCLC through MiR-33a and MiR-130b. Cell. Mol. Life Sci. 2022, 79, 446. [Google Scholar] [CrossRef]
  198. Vascotto, C.; Cesaratto, L.; Zeef, L.A.H.; Deganuto, M.; D’Ambrosio, C.; Scaloni, A.; Romanello, M.; Damante, G.; Taglialatela, G.; Delneri, D.; et al. Genome-Wide Analysis and Proteomic Studies Reveal APE1/Ref-1 Multifunctional Role in Mammalian Cells. Proteomics 2009, 9, 1058–1074. [Google Scholar] [CrossRef] [Green Version]
  199. Ayyildiz, D.; Antoniali, G.; D’Ambrosio, C.; Mangiapane, G.; Dalla, E.; Scaloni, A.; Tell, G.; Piazza, S. Architecture of The Human Ape1 Interactome Defines Novel Cancers Signatures. Sci. Rep. 2020, 10, 28. [Google Scholar] [CrossRef] [Green Version]
  200. Wilson, D.M.; Deacon, A.M.; Duncton, M.A.J.; Pellicena, P.; Georgiadis, M.M.; Yeh, A.P.; Arvai, A.S.; Moiani, D.; Tainer, J.A.; Das, D. Fragment- and Structure-Based Drug Discovery for Developing Therapeutic Agents Targeting the DNA Damage Response. Prog. Biophys. Mol. Biol. 2021, 163, 130–142. [Google Scholar] [CrossRef]
  201. Codrich, M.; Degrassi, M.; Malfatti, M.C.; Antoniali, G.; Gorassini, A.; Ayyildiz, D.; De Marco, R.; Verardo, G.; Tell, G. APE1 Interacts with the Nuclear Exosome Complex Protein MTR4 and Is Involved in Cisplatin- and 5-Fluorouracil-Induced RNA Damage Response. FEBS J. 2022, 290, 1740–1764. [Google Scholar] [CrossRef]
  202. Garutti, M.; Pelizzari, G.; Bartoletti, M.; Malfatti, M.C.; Gerratana, L.; Tell, G.; Puglisi, F. Platinum Salts in Patients with Breast Cancer: A Focus on Predictive Factors. Int. J. Mol. Sci. 2019, 20, 3390. [Google Scholar] [CrossRef] [Green Version]
  203. Dumas, L.; Herviou, P.; Dassi, E.; Cammas, A.; Millevoi, S. G-Quadruplexes in RNA Biology: Recent Advances and Future Directions. Trends Biochem. Sci. 2021, 46, 270–283. [Google Scholar] [CrossRef]
  204. Kwok, C.K.; Sahakyan, A.B.; Balasubramanian, S. Structural Analysis Using SHALiPE to Reveal RNA G-Quadruplex Formation in Human Precursor MicroRNA. Angew. Chem. Int. Ed. 2016, 55, 8958–8961. [Google Scholar] [CrossRef]
  205. Figueiredo, J.; Santos, T.; Miranda, A.; Alexandre, D.; Teixeira, B.; Simões, P.; Lopes-Nunes, J.; Cruz, C. Ligands as Stabilizers of G-Quadruplexes in Non-Coding RNAs. Molecules 2021, 26, 6164. [Google Scholar] [CrossRef] [PubMed]
  206. Koralewska, N.; Szczepanska, A.; Ciechanowska, K.; Wojnicka, M.; Pokornowska, M.; Milewski, M.C.; Gudanis, D.; Baranowski, D.; Nithin, C.; Bujnicki, J.M.; et al. RNA and DNA G-Quadruplexes Bind to Human Dicer and Inhibit Its Activity. Cell. Mol. Life Sci. 2021, 78, 3709–3724. [Google Scholar] [CrossRef]
  207. Asamitsu, S.; Shioda, N. Potential Roles of G-Quadruplex Structures in RNA Granules for Physiological and Pathological Phase Separation. J. Biochem. 2021, 169, 527–533. [Google Scholar] [CrossRef]
  208. Zhang, Y.; Yang, M.; Duncan, S.; Yang, X.; Abdelhamid, M.A.S.; Huang, L.; Zhang, H.; Benfey, P.N.; Waller, Z.A.E.; Ding, Y. G-Quadruplex Structures Trigger RNA Phase Separation. Nucleic Acids Res. 2019, 47, 11746–11754. [Google Scholar] [CrossRef] [PubMed]
  209. Mirihana Arachchilage, G.; Dassanayake, A.C.; Basu, S. A Potassium Ion-Dependent RNA Structural Switch Regulates Human Pre-MiRNA 92b Maturation. Chem. Biol. 2015, 22, 262–272. [Google Scholar] [CrossRef] [PubMed] [Green Version]
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Figure 1. Human APE1 structure and its key residues. A schematic representation of the primary sequence of APE1, in which the most important aminoacids are highlighted. In the first 33 residues required for protein-protein interaction, residues K6 and K7 (green, ο) are involved in the shuttling between the nucleus and the cytoplasm. Residues K27, K31, K32, and K35 are essential for proteosomal cleavage. All the above mentioned lysine residues can also be acetylated. The redox regulatory region is included between aminoacids 35 and 125, in which the main residues involved are C65, C93, and C99 (red). The endonuclease domain spans between 65 and 318 (residues indicated in blue, •). Specifically, E96 is involved in divalent metal coordination, while D210 and H309 have functions in the hydrolytic reaction. Other important residues in the endonuclease domain are D70, which is implicated in the 3′-phosphodiesterase activity; K98, important for the nucleotide incision repair (NIR); and F266, which is involved in the 3′-5′ exonuclease activity. Lastly, P112L, D148E, R193C/H, R237C, and H298Y/Q (yellow, ο) are some of the polymorphisms of APE1 that will be discussed in this review. Below, the tridimensional structure of APE1 is reported (PDB ID: 7SVB). Created with BioRender.com (accessed on 31 May 2023).
Figure 1. Human APE1 structure and its key residues. A schematic representation of the primary sequence of APE1, in which the most important aminoacids are highlighted. In the first 33 residues required for protein-protein interaction, residues K6 and K7 (green, ο) are involved in the shuttling between the nucleus and the cytoplasm. Residues K27, K31, K32, and K35 are essential for proteosomal cleavage. All the above mentioned lysine residues can also be acetylated. The redox regulatory region is included between aminoacids 35 and 125, in which the main residues involved are C65, C93, and C99 (red). The endonuclease domain spans between 65 and 318 (residues indicated in blue, •). Specifically, E96 is involved in divalent metal coordination, while D210 and H309 have functions in the hydrolytic reaction. Other important residues in the endonuclease domain are D70, which is implicated in the 3′-phosphodiesterase activity; K98, important for the nucleotide incision repair (NIR); and F266, which is involved in the 3′-5′ exonuclease activity. Lastly, P112L, D148E, R193C/H, R237C, and H298Y/Q (yellow, ο) are some of the polymorphisms of APE1 that will be discussed in this review. Below, the tridimensional structure of APE1 is reported (PDB ID: 7SVB). Created with BioRender.com (accessed on 31 May 2023).
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Cells 12 01895 g002 550
Figure 2. Illustration of the main functions of APE1 and its relative inhibitors. The DNA repair mediated by the endonuclease activity of APE1 is inhibited by Methoxyamine, APE Inhibitor III, and Gossypol (blue blunt arrows). The gene expression promoted by the redox activity of APE1 on TFs is inhibited by Gossypol, curcumin, resveratrol, and APX3330 (green blunt arrows). Especially through its N-terminal region, APE1 is involved in several PPIs, including Nucleophosmin 1 (NPM1). This interaction is inhibited by fiduxosin, SB 206553, and spiclomazine (fuchsia blunt arrows). Recent findings have shown that APE1 is secreted by EVs in the microambient and is involved in RNA metabolism, including the regulation of miRNA processing. If these novel features of APE1 can be inhibited, it is still unknown (brown blunt arrows) and an interesting starting point for future explorations. For each inhibitor, pillows are drawn when the inhibitor has been enrolled in one or more clinical trials. Created with BioRender.com (accessed on 31 May 2023).
Figure 2. Illustration of the main functions of APE1 and its relative inhibitors. The DNA repair mediated by the endonuclease activity of APE1 is inhibited by Methoxyamine, APE Inhibitor III, and Gossypol (blue blunt arrows). The gene expression promoted by the redox activity of APE1 on TFs is inhibited by Gossypol, curcumin, resveratrol, and APX3330 (green blunt arrows). Especially through its N-terminal region, APE1 is involved in several PPIs, including Nucleophosmin 1 (NPM1). This interaction is inhibited by fiduxosin, SB 206553, and spiclomazine (fuchsia blunt arrows). Recent findings have shown that APE1 is secreted by EVs in the microambient and is involved in RNA metabolism, including the regulation of miRNA processing. If these novel features of APE1 can be inhibited, it is still unknown (brown blunt arrows) and an interesting starting point for future explorations. For each inhibitor, pillows are drawn when the inhibitor has been enrolled in one or more clinical trials. Created with BioRender.com (accessed on 31 May 2023).
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Table
Table 1. APE1 polymorphisms detected in different cancer types by using the cBioPortal tool. * stands for type of mutation. Further information is available at https://bit.ly/3M9Oya7 (accessed on 22 March 2023).
Table 1. APE1 polymorphisms detected in different cancer types by using the cBioPortal tool. * stands for type of mutation. Further information is available at https://bit.ly/3M9Oya7 (accessed on 22 March 2023).
CancerPolymorphisms
Adrenocortical carcinomaD283H; X20_splice
Ampullary cancerM271T
Bladder cancerD15H; S146L; Q109E; E217 *
Bone cancerV131M
Breast cancerL244Tfs * 8; Q51 *; H289Y; G5A;
K7Rfs * 75; R185W; A60G
Cervical cancerR281C; K7R
Colorectal cancerA273T; R193C; R221H; G130D; R247Q; A230D; M271I; R221H; R181 *; E242D; R274 *; P293S; P49Qfs * 33; L220I; T233M; N226Efs * 26; V131M; L291Vfs * 6; R221C; K63E; D210N; R281H; X82_splice; E101D; K77N; P331H; G306S; G132D
Endometrial cancerR193H; S164L; R221H; A170V; P223L; V84I; V278D; R281H; K228T
Gastric cancerR281C; P122A; K27N
GliomaH289Q; Q245R; G80E; D142N
Head and Neck cancerP48H
Leukemia and LymphomaR181Q; L17P; K7R; R187H
Liver cancerG5E; W280S; L220P; W280R; D50Rfs * 28; G8R; H289Y, N226Efs * 26; Y264_G279del
Lung cancerG41C; V206Cfs * 11; V142Sfs * 8; E16Q; P331T; E149Q; X147_splice; R177*; D90H; Q51 *; X237_splice; R193C; R28S; M271del; V206Cfs * 11; S115F; G8R; I146V; D148E
MelanomaG241W; E16K; G127V; R136S; P122T; D148E; A263V; K7Rfs * 75; L108F; V69L
Oesophageal cancerE46D; D251N; M270Nfs * 14; F165V; N102I; L291Vfs * 6; K3R; G145D
Ovarian cancerQ95 *, V168I; R193H; L291Vfs * 6
Pancreatic cancerR193C; M271del
Prostate cancerP139Q; A30T; R187H
Renal cancerE149 *
SarcomaR187L; K35Rfs * 11; K35Q
Skin cancerP89S
Table
Table 2. Overview of the dysregulation of APE1 observed in different tumors. For each cancer type, the APE1 expression, diagnostic value, and localization are described and complemented by relevant references. n.d.: not defined; OS: overall survival; DFS: disease-free survival; PFS: progression-free survival; RFS: relapse-free survival; acAPE1: acetylated APE1.
Table 2. Overview of the dysregulation of APE1 observed in different tumors. For each cancer type, the APE1 expression, diagnostic value, and localization are described and complemented by relevant references. n.d.: not defined; OS: overall survival; DFS: disease-free survival; PFS: progression-free survival; RFS: relapse-free survival; acAPE1: acetylated APE1.
CancerExpressionDiagnostic ValueLocalizationRefs
Bladder
cancer (Bca)		Protein overexpression, associated with poor survival and invasion.Serum and urine levels as a diagnostic biomarker.
  • In non-invasive, low-grade tumors, localization is mainly in the nucleus.
  • In invasive, high-grade tumors, both nuclear and cytoplasmic localization.
[38,39,40,41,42,43,44]
Breast
cancer
  • Conflicting data on protein expression: in some cases, overexpression is associated with a malignant phenotype and an unfavorable prognosis; in other cases, low APE1 is associated with an aggressive triple-negative phenotype;
  • Deregulation of acAPE1.
n.d.Nuclear localization. [45,46,47,48,49,50]
Cervical
cancer		High protein expression is associated with lymph node metastasis, EMT, and decreasing radiosensitivity.n.d.
  • Moderate and heterogeneous nuclear staining;
  • Radioresistant cervical cancer cell lines show higher levels of cytoplasmic APE1 and lower levels of nuclear proteins.
[51,52,53,54]
Colorectal cancer (CRC)
  • Protein overexpression in cancer tissues is increasing from benign to malignant forms;
  • Overexpression of acAPE1 in tumor tissues is positively correlated with 5-FU resistance;
  • Presence of both the full-length and the N∆33 proteins;
Serum APE1-autoantibody levels as a diagnostic biomarker.
  • Nuclear and cytoplasmic localization;
  • The acetylated form accumulates in the nucleus.
[55,56,57,58,59,60,61,62]
Cutaneous Squamous Cell
carcinoma (cSCC)		Protein overexpression in tumor tissues, which promotes cell proliferation and migration by EMT.n.d.n.d.[63]
Gastric
carcinoma		mRNA and protein upregulation are correlated with lymph node metastasis, depth of invasion, and poor prognosis.Serum levels as a diagnostic biomarker for metastasis prediction.Nuclear and cytoplasmic localization.[64,65,66,67]
Glioma
  • Conflicting data are available in some cases, APE1 overexpression is shown, whereas in other cases, low mRNA and protein expression is associated with poor OS;
  • APE1 expression increases following treatment and recurrence.
n.d.Nuclear localization. [68,69,70,71,72,73]
Head and Neck Squamous Cell carcinoma (HNSCC)
  • In oral SCC (oSCC), protein overexpression, correlated with nodal status and lymph node invasion, shorter OS and DFS;
  • In laryngeal SCC (LSCC): protein overexpression in cancer tissues;
  • In sino-nasal SCC (sSCC) and SCC with inverted papilloma (SCCwIP): protein overexpression in cancer tissues;
  • In lip SCC (lSCC), protein overexpression in cancer tissues.
In oSCC: serum levels are used as a diagnostic biomarker, with high levels correlated with late TNM stages, lymph node metastasis, and worse pathologic differentiation.
  • oSCC: mainly nuclear localization with a weak cytoplasmic expression;
  • In sSCC and SCCwIP: vivid nuclear localization, associated with metastasis; higher cytoplasmic staining in sSCC, associated with T-stage and histological grade;
  • In lSCC: nuclear localization.
[74,75,76,77,78,79,80]
Liver
cancer
  • mRNA and protein overexpression, correlated with poor survival and cancer aggressiveness;
  • Presence of both the full-length and the N∆33 proteins.
Serum levels as a diagnostic biomarker.
  • Strong nuclear and cytoplasmic positivity, with higher cytosol expression in poorly differentiated tumors;
  • In lower-grade tumors, cytoplasmic positivity is associated with mitochondrial accumulation.
[81,82,83,84,85,86]
Lung
cancer
  • mRNA and protein overexpression in NSCLC (non-small-cell lung cancer), are associated with linfonodal metastasis and EMT promotion;
  • Increase in APE1 expression after cisplatin treatment;
  • High levels of acAPE1;
  • Presence of both the full length and N∆33 proteins.
High post-treatment serum levels are associated with lower OS.
  • Nuclear and cytoplasmic staining: higher cytoplasmic localization correlates with poor prognosis;
  • acAPE1 is strictly nuclear.
[55,87,88,89,90,91,92,93,94,95,96]
MelanomamRNA and protein overexpression are associated with vascular invasion, a high mitotic rate, lower response to therapy, and a poor prognosis.n.d.Nuclear localization. [97,98,99,100]
Oesophageal carcinoma (EAC)Protein overexpression in tumor tissues is associated with worse OS.n.d.Mainly nuclear localization.[101,102,103,104,105,106]
Osteosarcoma
  • Protein overexpression in cancer samples is associated with poor prognosis and cisplatin resistance.
n.d.
  • Mostly nuclear localization and variable cytoplasmic staining;
  • High cytoplasmic localization correlates with poor response to cisplatin therapy.
[107,108,109,110,111,112,113]
Ovarian
cancer		Protein overexpression in tumor tissues is associated with advanced stages, platinum resistance, poor chemosensitivity, decreased OS, and lymph node metastasis.n.d.
  • Strong nuclear and cytoplasmic localization, heterogeneous between different histological subtypes;
  • Cytoplasmic localization increases from well-to-poorly differentiated tumors, and it is higher in advanced stages;
  • Cytoplasmic localization is associated with lower PFS time and decreased OS.
[101,114,115,116,117,118,119,120,121]
Pancreatic adenocarcinoma (PDAC)
  • Protein overexpression in tumor tissues is associated with poor prognosis and tumor aggressiveness;
  • Elevated levels of acAPE1;
  • Presence of both the full-length and the N∆33 proteins.
n.d.Strong nuclear staining in tumor tissues, with cytosol staining only in advanced stages.[55,87,101,122,123,124]
Prostate
carcinoma (PCa)		Protein overexpression in cancer samples.n.d.Nuclear and cytoplasmic localization.[125,126]
Salivary gland carcinoma
  • Protein overexpression in tumor tissues increases dependence on malignant transformation and is correlated with lymph node metastasis and invasive growth;
  • Higher protein levels in smaller tumors.
n.d.Mainly nuclear staining, with nuclear and cytosolic staining in some malignant forms.[127,128]
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Malfatti, M.C.; Bellina, A.; Antoniali, G.; Tell, G. Revisiting Two Decades of Research Focused on Targeting APE1 for Cancer Therapy: The Pros and Cons. Cells 2023, 12, 1895. https://doi.org/10.3390/cells12141895

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Malfatti MC, Bellina A, Antoniali G, Tell G. Revisiting Two Decades of Research Focused on Targeting APE1 for Cancer Therapy: The Pros and Cons. Cells. 2023; 12(14):1895. https://doi.org/10.3390/cells12141895

Chicago/Turabian Style

Malfatti, Matilde Clarissa, Alessia Bellina, Giulia Antoniali, and Gianluca Tell. 2023. "Revisiting Two Decades of Research Focused on Targeting APE1 for Cancer Therapy: The Pros and Cons" Cells 12, no. 14: 1895. https://doi.org/10.3390/cells12141895

APA Style

Malfatti, M. C., Bellina, A., Antoniali, G., & Tell, G. (2023). Revisiting Two Decades of Research Focused on Targeting APE1 for Cancer Therapy: The Pros and Cons. Cells, 12(14), 1895. https://doi.org/10.3390/cells12141895

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