Background
Heart failure (HF) is a foremost side-effect of oncological therapies, most prominently those comprising anthracyclines, which are administered to an estimated 50% of cancer patients. Certain reductions in heart failure rates have been achieved by capping the maximal doses of anthracyclines and by changing their administration schedules. Nevertheless, heart failure continues to affect up to 20% of anthracycline-treated patients [
1]. The retrospectively identified individual risk factors such as young or old age, female sex, cardiovascular co-morbidities, certain co-therapies, and gene variants are currently of limited help. This is due to the lack of prospective clinical validation and to the scarcity of equipotent anthracycline-free treatment alternatives. Particularly problematic is the high HF risk in anthracycline-treated children and in the elderly attributed, respectively, to the long life expectancy and cardiac co-morbidities.
The bisdioxopiperazine dexrazoxane (DRZ, ICRF-187) reduces the incidence of anthracycline-induced heart failure by 80% and is the only drug approved for its prevention [
2]. Despite its impressive clinical effect, DRZ is indicated only in patients with metastatic (in the EU also with advanced) breast cancer who have already received 300 mg/m
2 doxorubicin (in the EU also epirubicin, 540 mg/m
2). Anecdotal evidence indicates a limited off-label use of DRZ in cancer patients with cardiac co-morbidities. DRZ is currently not approved for use in children and adolescents. Besides complex patent ownership and marketing history, the limited indication and use of DRZ reflect the persisting concerns of interference with antitumor efficacy of anthracyclines [
3], of induction of secondary malignancies, and of myelodysplastic syndrome [
4], although recent meta-analyses [
5] do not support these concerns. One study even reported prolonged, almost doubled, survival of doxorubicin (DOX) responders co-treated with DRZ [
6].
The clinical acceptance of DRZ has also suffered from the incomplete understanding of its pharmacology. The cardioprotective effect of DRZ is usually attributed to iron chelating by ADR-925, an EDTA-like product of the enzymatic DRZ hydrolysis. This is consistent with the hypothesis of heart failure arising from iron-dependent oxidative stress triggered by “redox cycling” of anthracyclines. However, ADR-925 applied directly does not protect cardiomyocytes against anthracyclines [
7]. Conversely, the inhibition of the enzymatic DRZ conversion to ADR-925 does not abolish the cardioprotective effect [
8]. Furthermore, cardioprotective activities of DRZ analogues are unrelated to the rates of formation of their iron-chelating (i.e. ADR-925-like) metabolites [
9]. Finally, the oxidative stress theory of anthracycline cardiotoxicity has been questioned, since oxidative stress is detectable in the heart following supra-clinical, but not clinically-relevant anthracycline doses [
10]. Accordingly, neither antioxidants [
11] nor iron chelators other than DRZ [
12,
13] prevent anthracycline-induced HF in cancer patients.
On the other hand, several investigators have observed depletion of the anthracycline target topoisomerase IIβ (TOP2B) in cells treated with DRZ or its analogues [
14‐
16]. Lyu et al. [
15] reported that DRZ-induced Top2b depletion prevented anthracycline-induced DNA damage in cardiomyocyte-derived H9C2 cells. Based on these observations, Lyu et al. proposed that DRZ prevents anthracycline-induced cardiomyocyte damage via TOP2B depletion. Importantly, this model also implicates that the anthracycline-induced cardiotoxicity is primarily driven by TOP2B-mediated DNA damage. In support of these findings, a recent study in cardiomyocyte-specific knockouts suggested the involvement of Top2b in DOX-induced cardiotoxicity [
17]. Importantly, Top2b deletion prevented DOX-driven mitochondrial damage, implicating this enzyme as a common denominator of the mitochondrial and DNA damage-based models of anthracycline cardiotoxicity.
The TOP2B-centered model of anthracycline-induced heart failure and its prevention by DRZ clearly needs further verification when weighed against the body of literature supporting the original oxidative stress hypothesis. Furthermore, this model is incompatible with some other findings. Thus, it is inexplicable why DRZ fully abolished DOX-induced DNA double strand breaks (DSB) from cultured cardiomyocytes, as DRZ left unchanged the expression level of the sister isoform Topoisomerase IIα (TOP2A) [
15], an established DOX target. The TOP2A expression itself raises concerns regarding the validity of the cells used as a cardiomyocyte model, as it is usually expressed in proliferating and not post-mitotic cells [
18]. On the other hand, DRZ has been recently reported to deplete TOP2A from tumor cells [
14]. This depletion was proteasome-independent but it was associated with a strong reduction of TOP2A mRNA, whereas TOP2B mRNA remained unchanged. These results suggested that DRZ may deplete both TOP2B and TOP2A via different, transcriptional and proteolytic mechanisms, respectively. The verification of this possibility is important not only in organ protection but also for tumor treatments. Indeed, tumor TOP2A expression is a strong predictor of the therapeutic response to anthracyclines [
19] and its reduction by DRZ could be deleterious. Therefore, we set out to characterize the response of TOP2 isozymes to DRZ in cardiac and tumor cells.
Methods
Drugs and antibodies
DRZ was purchased from Chiron (Amsterdam, The Netherlands), DOX was from Pfizer (Karlsruhe, Germany). ICRF-161 and ICRF-193 were kindly provided by Dr. Annemette V. Thougaard (TopoTarget A/S, Copenhagen, Denmark). The following antibodies were used in Western blot: TOP2A/B (1: 200) and TOP2A (1:2,000) from StressGen, TOP2B (1:2,000) from BD Pharmingen, γ-H2AX (1:500) from Abcam, GFP (1:5,000) from Clontech, GAPDH (1:10,000) from Santa Cruz Biotechnology, α-tubulin (1:5,000) from Dianova (Germany) and β-tubulin (1:100,000) from Sigma.
Cell culture
HTETOP cells express TOP2A exclusively from a transgene under the control of a tetracycline-repressive promoter, have been previously established [
20]. HTETOP and the parental HT1080 cells were provided by Dr. Andrew C.G. Porter (Centre for Haematology, Faculty of Medicine, Imperial College London, England) and cultured as previously described [
14]. To obtain differentiation, H9C2 cells (provided by Dr. Tomas Simunek, Department of Biochemical Sciences, Charles University in Prague, Czech Republic) were continuously cultured for 14 days: 3 days in 10% FCS medium and the following 11 days in 1% FCS medium. HEK293 cells were obtained from Dr. Christian Mielke (Institute of Clinical Chemistry and Laboratory Diagnostics, Heinrich-Heine-University, Düsseldorf, Germany) and NYH cells were from Dr. Annemette V. Thougaard (TopoTarget A/S, Copenhagen, Denmark).
Mice and treatment
Wild type C57BL/6 J (B6) mice were purchased from Jackson Lab (Bar Harbor, ME) and they were 8–12 weeks old at the onset of experiment. Mice were injected i.p. with 100 μl of saline (control group, n =3) or 200 mg/kg DRZ in the same volume of saline (DRZ group, n =9). Animals were sacrificed by cervical dislocation 6, 24 or 48 h after DRZ injection and the whole hearts were isolated and snap-frozen in liquid nitrogen. In parallel experiments, mice were injected with 200 mg/kg DRZ alone (n =3), 20 mg/kg DOX (n =3) alone or in combination (n =3, DRZ was injected 30 min before DOX). Heart tissues were removed 24 h later for Western blot analysis. The mouse experiments described in this paper have been permitted by the Animal Care Committee of Rhineland-Palatinate (Koblenz, Germany) with the permit No. AZ 23 177-07/G 12-1-043.
Western blot
Heart tissues from control or drug-treated mice were homogenized thoroughly in RIPA buffer containing proteinase inhibitors [
14]. The lysate was subsequently incubated for 2 h at 4°C with agitation. Cultured cells were harvested and lysed in RIPA buffer followed by 30 min incubation on ice. Twenty to 50 μg protein samples were separated by SDS-PAGE as described previously [
14]. Densitometric analysis of protein bands was performed using the NIH Image J software.
RNA interfering and transient transfection
siRNA oligos were used to knock down human TOP2B with the target region GCTTAACAATCAAGCCCGT [
21]. siRNA oligos against the GFP sequence GGCTACGTCCAGGAGCGCACC were used as non-silencing control. To specifically knock down the endogenous TOP2B without affecting the transfected TOP2B-YFP, three siRNA oligos targeting the 3-UTR of human TOP2B mRNA were applied, since the TOP2B-YFP expression vector encompasses only the open reading frame of TOP2B without 3-UTR. The target sequences for 3-UTR region were as follows: siRNA1: GAAATGTCACGTACTGTCTGA; siRNA2: ACTGTCTGATTGGCTTGTAGA; siRNA3: GCTTGTAGAATTGTTATAGAC. For H9C2 cells, the target sequence of siRNA to knock down rat Top2b was: GAACAAAGCTGGTGTATCA. siRNA oligos were transfected at the final concentration of 50 nM using the jetPRIME
TM transfection reagent (Polyplus Transfection SA, Illkirch, France) according to the specifications of the manufacturer.
Site-directed mutagenesis
The bicistronic vector expressing human TOP2B fused with enhanced yellow fluorescent protein (YFP) at the C-terminal has been described previously [
22]. Single amino acid substitution was introduced into this vector with the site-directed mutagenesis Kit (QuikChange, Stratagene). Primers for individual TOP2B mutants are shown in Table
1. The mutated sites are highlighted by italic bold letters. PCR conditions for mutagenesis were according to the manufacturer’s instructions. The introduction of the desired and the absence of off-target mutations was verified by sequencing.
Table 1
Primers for site-directed mutagenesis of human TOP2B
T65I | forward | cattcttcttcgtcctgatatatatattgggtcagtggagc |
| reverse | gctccactgacccaatatatatatcaggacgaagaagaatg |
Y66F | forward | tcttcgtcctgatacatttattgggtcagtggagc |
| reverse | gctccactgacccaataaatgtatcaggacgaaga |
R178Q | forward | gatgagaaaaaagttacaggtggtcaaaatggttatggtgcaaaactttgta |
| reverse | tacaaagttttgcaccataaccattttgaccacctgtaacttttttctcatc |
Y181S | forward | aaagttacaggtggtcgtaatggttctggtgcaaaactttg |
| reverse | caaagttttgcaccagaaccattacgaccacctgtaacttt |
L185F | forward | ggtcgtaatggttatggtgcaaaattttgtaatattttcagtacaaagt |
| reverse | actttgtactgaaaatattacaaaattttgcaccataaccattacgacc |
RNA-Seq data analysis
The raw RNA-Seq data obtained from diverse human or mouse organs were downloaded in Fastq format from Gene Expression Omnibus (GEO) in NCBI (accession number GSE30352) [
23]. Original reads were mapped against human (version GRCh37/hg19) or mouse (version NCBI37/mm9) genome with TopHat using gene annotation file as the reference for alignment [
24]. The genomic sequence data and gene annotation files were downloaded from UCSC (
http://genome.ucsc.edu/). Mapped reads were assembled with the program Cufflinks [
24] and the expression levels of individual transcripts were calculated as Fragment Per Kilobase of exon per Million fragments mapped (FPKM).
Statistical analysis
All experiments were repeated at least three times. Data were expressed as mean ± SE and analyzed with the two-tailed Student’s t-test or one-way ANOVA. P <0.05 was considered statistically significant.
Discussion
Our study contributes to the mechanistic understanding of the prevention of anthracycline-induced heart failure by DRZ. Simultaneously, it suggests mechanistic explanation for the inconsistent and sometimes contradictory reports of DRZ impact on anthracycline anticancer therapies. In the light of our data, these effects may be mediated by DRZ-triggered depletion of TOP2B.
The long-held view that cardioprotection involves iron-chelation by the EDTA-like product of the enzymatic DRZ hydrolysis ADR-925 has been recently questioned. Indeed, ADR-925 does not protect cardiomyocytes against anthracyclines [
7], while prevention of its generation from DRZ does not abolish the cardioprotective effect [
8]. These observations implicate DRZ itself as the cardioprotective compound. As several previous studies demonstrated TOP2B depletion by DRZ and its analogues [
14‐
16], we first verified these observations and investigated the underlying mechanism in more detail. We found DRZ capable of TOP2B depletion in all cell lines tested, including differentiated cardiomyocytes. In agreement with cell line data, we detected transient depletion of Top2b by DRZ in the mouse heart tissue, which constitutes a first report of this phenomenon
in vivo.
We provide several lines of complementary evidence for DRZ-mediated TOP2B depletion being protective against anthracycline-induced DNA damage. The reduction of DOX-induced DNA damage by DRZ was associated with TOP2B depletion and it was similar to that observed upon TOP2B removal by siRNA. That this reduction was indeed mediated by the TOP2B removal was evidenced first of all by the differential effect of DRZ analogues. Thus, the reduction of DOX-induced DNA damage was conferred by TOP2B-binding and -depleting (DRZ, ICRF-193), but not by the non-binding and non-depleting bisdioxopiperazine ICRF-161. In contrast to DRZ, ICRF-161 is not protective against DOX-induced heart damage [
25]. Taken together with our experiments, a bisdioxopiperazine’s cardioprotective effect seems therefore to be determined by its capability to deplete TOP2B rather than to chelate iron. Indirectly, these results support the emerging evidence that anthracycline-induced cardiotoxicity is driven by TOP2B-mediated DNA damage rather than by oxidative stress [
17].
To verify these conclusions mechanistically for the clinically relevant bisdioxopiperazine DRZ, we took advantage of the existing TOP2 DRZ resistance mutants. Strikingly, although not surprisingly, these mutants localize to the bisdioxopiperazine binding site in the N-terminal domain of TOP2 [
26]. All but one mutant prevented the depletion of TOP2B. Simultaneously, these mutants reduced the protective effect of DRZ against DOX-induced DNA damage. This result constitutes currently the strongest evidence that DRZ prevents DNA damage by depleting TOP2B, which is mediated through the bisdioxopiperazine binding site.
Taken together with the protective effect of a genetic Top2b deletion against DOX-induced cardiotoxicity [
17], our results suggest the following model of DRZ-mediated cardioprotection. DRZ depletes cardiac TOP2B, thereby reducing the substrate for DOX poisoning. Subsequent administration of an anthracycline results in lower levels of DNA damage than without DRZ pretreatment, i.e. in the presence of normal TOP2B levels. The depletion of TOP2B is transient, which reduces the risk or at least the duration of any adverse effects of this enzyme’s deficiency. Although we have failed to measure DSB in vivo, this model is fully consistent with the reducing effect of DRZ on Top2b levels and Top2b-mediated DSB in cultured rat cardiomyocytes. Moreover, it is consistent with the observation that DRZ is no longer cardioprotective when given after anthracyclines [
32], i.e. when DNA damage has already occurred.
The depletion of TOP2B by DRZ characterized in this study may also help to resolve the persisting concern of this drug’s interference with antitumor efficacy of anthracyclines. This concern has its seeds in a randomized, double-blind study of patients with advanced breast cancer treated with fluorouracil, DOX, and cyclophosphamide with or without DRZ [
3]. Although time to progression and survival were not significantly different, DRZ-treated patients showed a lower tumor response rate, in addition to the expected reduction of cardiotoxicity. The reduction of the response rate is no longer statistically significant in the latest update of the pertinent Cochrane meta-analysis, but a trend remains [
33].
Based on the growing evidence of TOP2B depletion by DRZ and its molecular characterization in the present study, we would like to argue that DRZ may lower the response rate by depleting TOP2B. Although the anti-tumor effects of TOP2 poisons are usually attributed to TOP2A rather than TOP2B, the application of TOP2A level as a therapeutic predictor has been unsuccessful [
34]. Quite the contrary, breast cancer survival can be predicted by TOP2B rather than TOP2A expression level [
35]. This could be explained by the TOP2B expression in >90% of cells in breast tumors. In contrast, TOP2A expression is restricted to the much smaller subset of proliferating (i.e. Ki67-positive) cells of breast tumors [
35]. A predominance of TOP2B in the combined TOP2A/TOP2B activity has been also described in ovarian tumors [
36].
As confirmed in the present study, both TOP2 isoforms mediate DOX-induced DNA damage in tumor cells. DRZ-driven depletion of TOP2B would be expected to reduce this damage and thereby the elimination of tumor cells. The DRZ-driven depletion of TOP2B is apparently transient, which would likely minimize any long-term effects deleterious to tumor cell survival. In consequence, DRZ would be expected to reduce tumor shrinkage, a key component of the tumor response. These considerations are in agreement with the reduction of therapy response by DRZ detected in breast cancer patients [
3].
Importantly, the reduction of tumor response by DRZ has been observed when DRZ was applied beginning with the first therapy course [
3]. When given to breast cancer patients first when they had reached a cumulative DOX dose of 300 mg/m2, DRZ almost doubled the survival [
6]. This effect is more difficult to explain in mechanistic terms, but it is important to remember that DRZ has some weak antitumor effects [
14]. These effects could become manifest only when a certain tumor shrinkage has been achieved. In other words, initially better tumor shrinkage in the absence of DRZ could sensitize the tumor to this drug’s anti-tumor effect when included into later therapy courses. Incidentally, this situation corresponds to the currently approved application of DRZ in breast cancer patients.
Finally, we verify and expand the original observation that DRZ may deplete TOP2A in addition to TOP2B [
14]. This effect may be mediated by a mechanism different from that of TOP2B depletion, as it is independent from the proteasome activity but accompanied by lower TOP2A mRNA levels [
14]. The depletion of TOP2A is less ubiquitous in comparison to TOP2B, as it has been detected only in some cell lines. The discrepancy of DRZ effects on TOP2A in H9C2 cells in this and a previous work [
15] may have been caused by our longer incubation times and by utilization of differentiated cells which express lower TOP2A levels. It is tempting to speculate that TOP2A depletion could account for the only side-effects of DRZ detected in current meta-analyses, i.e. low white blood count at nadir and anemia [
33]. Indeed, TOP2A is expressed predominantly in proliferating compartments such as bone marrow [
18,
37]. The effects of DRZ on the stability and expression of TOP2 isoforms in normal tissues deserve detailed investigations.
Competing interests
The authors declare that they have no competing interests.
Authors’ contributions
SD conceived of the study, carried out RNA-Seq data analysis and drafted the manuscript. TY carried out mutagenesis, plasmid preparation and Western blot. AN participated in the experiments with small RNA interfering. CJ, MV and UG carried out Western blot. LW conceived of the study and helped to draft the manuscript. All authors read and approved the final manuscript.