Synthesis and evaluation of AKR1C inhibitory properties of A-ring halogenated oestrone derivatives.

The enzymes of the aldo-keto reductase (AKR) superfamily catalyse NADPH-dependent reductions in carbonyl-group-containing substrates, to provide their alcohols 1 . There are four human members of the AKR1C subfamily; AKR1C1–AKR1C3 are widely expressed, and AKR1C4 is liver specific. The AKR1C enzymes act as 3-keto, 17-keto, and 20-keto steroid reductases, through which they regulate the actions of androgens, oestrogens, and progestagens at the pre-receptor level 2 . Differential expression of the genes that encode the AKR1C isoforms has been reported for a wide variety of cancers, including breast, prostate, and endometrial cancers, and also in benign pathologies, including endometriosis 2–4 . The AKR1C enzymes are associated with chemoresistance to platin-based drugs (e.g. cisplatin, carboplatin) 5–8 , and they are also involved in resistance to the anthracycline chemotherapeutics daunorubicin, doxorubicin, idarubicin, and epirubicin 9 , 10 . Studies in model cell lines and in explant mouse models have shown that AKR1C inhibitors can reverse the chemoresistance in cervical, colon, bladder, and oral cancers, and that AKR1C3 inhibitors can restore cytotoxicity of daunorubicin and idarubicin in lung, liver, breast, and colon cancers, and in leukaemia cell lines 9 , 11–17 . These actions of the AKR1C enzymes can be explained by their involvement in inactivation of cellular stressors, especially lipid peroxides, through reduction of 4-hydroxy-2-nonenal and inactivation of chemotherapeutics 18 . The AKR genes are up-regulated by stress responses via the Nrf2–Keap1 pathway, which explains the overexpression of AKR1C1–AKR1C3 in chemoresistant cell lines and tumour samples 18 . Chemoresistance is the hallmark of cancers 19 , 20 , and thus specific or pan-AKR1C inhibitors are needed to alleviate the serious and very frequent problems of resistance to platinum-based chemotherapeutics and individual anthracyclines. Inhibitors against enzymes involved in the regulation of the actions of oestrogens at the pre-receptor level can be designed based on their oestrone substrates. However, one of the major risks of oestrone-based inhibitors is their oestrogenic side-effects. This might be avoided by the use of core-modified synthetic oestrone derivatives that lack hormonal activity. Owing to its modified conformation, 13α-oestrone meets these requirements, in terms of low affinity for nuclear oestrogen receptors 21 , 22 . We reported recently on the synthesis and biochemical assessment of oestrone A-ring halogenated derivatives ( Figures 1 and 2 ) 23–25 . The 2- and 4-halogenated, and the 2,4- bis -halogenated derivatives were subjected to biochemical investigations into their effects on the enzymes involved in oestrogen biosynthesis. Important structure–activity relationships were defined, and certain potent inhibitors of 17β-hydroxysteroid dehydrogenase 1 and steroid sulphatase were identified 25 . Structures of the oestrones and their halogenated derivatives considered in the present study. Structure of the halogenated 13α-methyl-oestrone 3-methyl ethers considered in the present study. Previous transformation of substrates 1 and 2 ( Figures 1 and 2 ) with Selectfluor as reagent produced the 10β-fluoro-oestra-1,4-dien-3-ones ( Figure 3 ) 26 . The 10-fluoro and 10-chloro 13-epimeric 1,4-dien-3-ones have also been investigated for inhibition of the human aromatase enzyme, which is responsible for aromatisation of androgens to oestrogens 26 . For this aromatase, the 13β-methyl group of these compounds appeared to be crucial, as only the 13β-methyl compounds were potent inhibitors, with submicromolar or micromolar IC 50 values. Structures of the epimeric 10-fluoro-1,4-dien-3-ones 4 and 5 . Several halogenated 13α-methyl-oestrones have been evaluated for inhibition of organic anion transporting polypeptide 2B1 (OATP2B1), which is involved in cellular transport of oestrone sulphate 24 . The OATP2B1 inhibitory potential greatly depended on the structure of the tested derivative. The most potent derivative showed outstanding OATP2B1 inhibition with submicromolar IC 50 . Considering all of the available data for these A-ring halogenated derivatives, and especially those of 13α-oestrone, this compound group appears to be particularly promising for the design of antitumoral agents with multiple inhibitory actions. Furthermore, based on our recent data, structurally different enzymes might be inhibited by the same synthetic compounds. With these considerations in mind, we aimed here to investigate the inhibitory properties against the enzymes AKR1C1‒3 of the recently and newly synthesised halogenated derivatives of oestrone. The test compound set included the 13β-methyl-oestrone ( 1 ) and 13α-methyl-oestrone ( 2 ) halogenated derivatives and the 17-deoxy-13α-methyl ( 3 ) counterparts, with the halogens at C-2 and/or C-4. Additional to the investigations of these base compounds, a selection of their 3-methoxy derivatives ( 1Me , 2Me , 3Me ) and the 13-epimeric 10-fluoro 1,4-dien-3-ones ( 4 , 5 ) were halogenated and included. Finally, for selected ligands, computational investigations were used to gain insight into the molecular backgrounds of the enzyme selectivities using docking and molecular dynamics (MD). On the assumption that greater biological activity can be achieved through stronger ligand–protein interactions, the ligands with well-defined selectivities were considered for each enzyme. Concerning specific interactions, the selected ligands and the enzymes were analysed initially by docking calculations and then by MD.

Electrophilic substitutions with N -halosuccinimides were carried out in our recent studies, starting from the 13β-methyl-oestrone ( 1 ), its 13α-methyl epimer ( 2 ) and the 17-deoxy-13α-methyl-oestrone ( 3 ; Figure 2 ) 26 , 27 . Halogenations occurred at the ortho positions relative to the phenolic OH group. Mono-substituted and bis -substituted derivatives were formed. Starting from the 3-methyl ethers ( 1Me , 2Me , 3Me ), mono-halogenated derivatives were obtained exclusively. Some of these halogenated oestrone derivatives showed potent inhibition of aromatase, oestrone sulphatase, and 17β-hydroxysteroid dehydrogenase, and/or OATP2B1 actions 26 , 27 . Important structure–activity relationships were identified. These studies indicated that the 13α-methyl epimer of the natural oestrone might be superior to its 13β-methyl counterpart, as it is readily available and hormonally inactive and has other promising biological properties. The group of 2,4- bis halogenated compounds provided the most promising inhibitors from the biological point of view. Encouraged by these data, we continued our interest in the synthesis of A-ring halogenated derivatives of 13α-methyl-oestrone here. 2,4-Disubstituted compounds that included different halogens were synthesised ( Scheme 1 ). The order of the halogen introduction had to be defined, whereby the smaller halogen had to be introduced first. Chlorination of 13α-methyl-oestrone ( 2 ) resulted in the 2-chloro and 4-chloro derivatives, which were subjected to bromination. The 4-bromo-2-chloro ( 2 _2Cl,4Br) and 2-bromo-4-chloro ( 2 _2Br,4Cl) compounds were obtained in high yields. Iodination of the chloro derivatives led to the 2-chloro-4-iodo ( 2 _2Cl,4I) and 4-chloro-2-iodo ( 2 _2I,4Cl) derivatives. Bis compounds that included bromo and iodo substituents were synthesised starting from the 2-bromo and 4-bromo substrates. Iodination with N -iodosuccinimide provided the desired 2-bromo-4-iodo ( 2 _2Br,4I) and 4-bromo-2-iodo ( 2 _2I,4Br) products in excellent yields. Synthesis of the 2,4-disubstituted 13α-methyl-oestrone derivatives with the different halogens. Along with the three starting oestrones ( 1 , 2 , 3 ) and their 3-methyl ether derivatives ( 1Me , 2Me , 3Me ), we evaluated 35 halogenated derivatives of oestrone as inhibitors of the recombinant enzymes AKR1C1, AKR1C2, and AKR1C3. There were 29 13α-methyl-oestrones, which included 3-hydroxy,17-keto-oestrones (16 compounds), 3-methoxy, 17-keto-oestrones (seven compounds) and 17-deoxy-oestrones (five compounds). There were also 12 13β-methyl-17-keto-oestrones. The screening data for these oestrones and their derivatives for inhibition of recombinant enzymes AKR1C1-AKR1C3 are presented in Table 1 . Inhibition of the AKR1C enzymes by the halogenated oestrone derivatives. NI: no inhibition. Data in bold, compounds showing ≥80% inhibition for the respective AKR1C. Initial screening at 100 µM oestrones revealed that a number of these acted as potent inhibitors: 13 compounds showed ≥80% inhibition of AKR1C1 (six compounds at 10 µM), 11 compounds showed ≥80% inhibition of AKR1C2 (six compounds at 10 µM), and 10 compounds showed ≥80% inhibition of AKR1C3 (none at 10 µM). When the compounds were screened at 10 μM, additional potent inhibitors of AKR1C2 were revealed that had shown lower inhibitory activities at the higher concentration ( 1 _4Br, 1 _4Cl, 2 _2Br), which was probably caused by solubility issues. Among the 13β-methyl-17-keto-oestrones, five showed potent inhibition of AKR1C1, as ≥80% at 100 μM, with IC 50 values for the two most promising compounds, 1 _2Br,4Br and 1 _2Cl,4Cl, of 5.4 μM and 1.6 μM, respectively. Neither of these two were selective inhibitors of AKR1C1, as 1 _2Br,4Br also showed strong inhibition of AKR1C2 (IC 50 =5.6 μM), and 1 _2Cl,4Cl, of AKR1C3 (IC 50 =6.3 μM). Two other 13β-methyl-17-keto oestrones, 1 _4Br and 1 _4Cl, inhibited AKR1C2 in the low micromolar range (IC 50 =7.0, 5.3 μM, respectively), while no inhibition was seen for these at 10 μM with AKR1C1, and low inhibition was seen for AKR1C3 (25% and 50%, respectively). The 13α-methyl-17-keto-oestrones in the 3-methyl ether series generally showed weaker inhibition of the AKR1C enzymes compared to their 3-hydroxy counterparts. Indeed, only two of these showed inhibition ≥80% at 100 μM, for AKR1C3 ( 2Me _2Cl, 2Me _4Cl), with much weaker inhibition of AKR1C1 and AKR1C2. The more potent inhibition by the 13α-methyl-17-keto-oestrones in the 3-hydroxy series included six compounds with ≥80% inhibition of AKR1C1 at 10 μM, where the best two had IC 50 of 0.7 μM and 0.8 μM ( 2 _2I,4Br, 2 _2I,4Cl, respectively). Five of these compounds inhibited AKR1C2 by ≥80% at 10 μM, where the best inhibitor had an IC 50 of 1.5 μM ( 2 _2Br). This group of oestrone derivatives did not include any potent AKR1C3 inhibitors (i.e. none ≥80% inhibition at 10 μM). Finally, we screened five 13α-methyl-17-deoxy derivatives. For the initial testing at 100 μM, some promising results were shown, but only for AKR1C2 (three compounds showed around 75% inhibition). At 10 μM, 3 _2Br,4Br and 3 _2Cl,4Cl showed 68.0% and 66.2% inhibition, respectively, with the best compound, 3 _2Br,4Br, with an IC 50 of 0.9 μM. To further evaluate these oestrone derivatives as inhibitors of the AKR1C enzymes, we conducted detailed kinetic studies on three different compounds, which were chosen as they were the most potent inhibitors of AKR1C1, AKR1C2, and AKR1C3. The first was compound 1 _2Cl,4Cl, or bis -chloro-13β-methyl-17-keto-oestrone, which inhibited both AKR1C1 and AKR1C3 potently, but showed low inhibition of AKR1C2. These inhibition studies revealed a mixed type of inhibition of 1 _2Cl,4Cl for AKR1C1 (Ki = 0.69 μM), which was instead competitive for inhibition of AKR1C3 (Ki = 1.43 μM) ( Table S1 ). The second compound chosen here was 2 _2I,4Br, a 3-hydroxy disubstituted 13α-methyl-17-keto-oestrone, which at 10 μM showed 90.7% inhibition of AKR1C1, 59.5% inhibition of AKR1C2 and 40.0% of AKR1C3. Its IC 50 for AKR1C1 was 0.7 μM, with Ki of 0.57 μM. Here, 2 _2I,4Br showed a mixed type of inhibition of AKR1C1. Finally, the third compound chosen was 3 _2Br,4Br, a 13α-methyl-17-deoxy bis -bromo oestrone, which showed selectivity for AKR1C2, with IC 50 of 0.9 μM. 3 _2Br,4Br also showed mixed type of inhibition, with Ki of 1.98 μM. On the basis of these inhibition data, we were able to postulate the initial structure–activity relationship for all three AKR1C isoforms. The most potent of these AK1C1 inhibitors were a 13β-methyl-17-keto-oestrone ( 1 _2Cl,4Cl) and a 13α-methyl-17-keto-oestrone ( 2 _2I,4Br), with the halogen atoms at both C-2 and C-4 ( Figure 4 ). For the 13β-methyl-17-keto-oestrone, the activity was highest with bromine and chlorine, which indicated that iodine would probably be too large, and would result in lower enzyme inhibition. Here, the most potent inhibitor had chlorine at both positions, for its IC 50 of 1.6 μM. For the equivalent 13α-methyl epimers, the lowest IC 50 were achieved with iodine on C-2 and bromine or chlorine on C-4 (IC 50 : 2 _2I,4Br, 0.7 μM; 2 _2I,4Cl, 0.8 μM). These oestrone derivatives were selective for AKR1C1. The loss of the 17-keto group ( 3 , and its derivatives) or methylation of the 3-hydroxy group ( 2Me , 3Me , and their derivatives) had negative impact on the AKR1C inhibition. Structure–activity relationship for inhibition of the AKR1C1-3 enzymes. We established here that with the 13β-methyl epimers, no substitution or bromine substitution at C-2 was effective for inhibition of AKR1C2, while bromine or chlorine at C-4 was beneficial, but not iodine ( Figure 4 ). The larger halogens at C-4 thus appeared to be advantageous. The loss of the keto group at position 17 halved the IC 50 . The best two AKR1C2 inhibitors among the 13α-methyl-17-keto-oestrone epimers had only a bromine at the C-2 position and only a chlorine at the C-4 position (IC 50 : 2 _2Br, 1.5 μM; 2 _4Cl, 1.8 μM). These two compounds also showed high selectivity for the AKR1C2 isoform. These structure–activity relationship studies also revealed that chlorine substitution of 13β-methyl-17-keto oestrones at C-2 and/or C-4 was required for AKR1C3 inhibition, with improvement for both at the same time (IC 50 : 1_2Cl,4Cl, 6.3 µM; Figure 4 ). With bromine substitution showing low inhibition of AKR1C3, all inhibition was lost with either no substitution or iodine substitution. For 13α-methyl-3-methoxy-17-keto-oestrones, bromine or chlorine substitution at C-2 and the larger halogens at C-4 (i.e. chlorine, iodine) were required for AKR1C3 inhibition, while this inhibition of AKR1C3 was almost completely lost when the 17-keto group was removed. Methylation of 3-hydroxy group greatly improved the potency of the AKR1C3 inhibition. For an atomic level investigation of the structural background of the biological activities, computational simulations were carried out for the ligands that showed well-defined enzyme selectivities. First, docking calculations were performed using the Glide programme 29–31 , where receptor models were based on experimental X-ray crystal structures from the PDB database ( http://www.rcsb.org ). The following structures were selected for AKR1C1, AKR1C2, and AKR1C3: 1MRQ (AKR1C1 in complex with NADPH and 20α-hydroxyprogesterone); 4L1W (AKR1C2 in complex with NADP +  and progesterone); and 1XF0 (AKR1C3 in complex with NADP +  and androstenedione). The structures were prepared for docking calculations according to the details in the “Materials and methods” section. It is worth noting that various structures can be retrieved for each enzyme in the PDB database, but the crystal structures were always selected here, with co-crystallisation with a steroid ligand. The precision of the docking protocol was verified by redocking the original crystal ligand into the binding pocket, where the XP method with the applied settings accurately reproduced the binding poses of the original co-crystallised ligands. Then, all the selected ligands ( 2 _2I,4Br, 2 _4Cl, 2 _4I) were docked into each relaxed target, where the scoring function of the docking program (glide-score) correlates with the binding free energy (Δ G ) and therefore with the enzyme activity. Unfortunately, even the ligand with the highest biological activity for the relevant receptor could not be properly predicted by the docking calculations (see Glide score values in Table 2 ). Scoring values of docking calculations, mean and standard error of means (SEM) of binding energies (in kcal/mol) determined by MMGBSA calculations, as well as biological inhibition (at 100 μM) for the tested compounds are presented. The enzyme structures in docking studies were based on X-ray crystal structures from the pdb database ( http://www.rcsb.org ; AKR1C1, 1MRQ; AKR1C2, 4L1W; AKR1C3, 1XF0). Thus, a more advanced Δ G calculation scheme was applied, namely the MMGBSA method, which used 500-ns-long MD trajectories for all the nine ligand–target complexes. The starting structures of the MD simulations were always the best pose geometries from the docking calculations, and the MMGBSA binding free energies were computed as 2500 snapshots for each trajectory. Statistical descriptors were calculated for all the nine ligand–target complexes, including means and standard error of means of Δ G , with these data shown in Table 2 . It can be seen that the MMGBSA calculations always defined the most active ligand with the strongest binding affinity for each enzyme. So, these 500-ns-long MD simulations can correctly represent the ligand–target interactions. It can also be mentioned that the tertiary structures of the three enzymes were very similar; each of them contained a central β-barrel structure that was surrounded by eight α-helices and a nicotine-adenosine-diphosphate co-factor on one of the tops of the barrel. The steroid binding site was located on the top side of the β-barrel, adjacent to the co-factor. The binding pocket was formed by flexible loops in all three cases, which emphasises the dynamic nature of the ligand binding. On the basis of these impressions of the binding geometry of a steroid in an AKR1C enzyme, we have presented here the starting poses of the MD calculations for all of the three ligands in their “preferred” enzyme in the Supplementary Information ( Figure S1 ). As the MMGBSA calculations successfully identified the most active ligands as the strongest binding ones, we examined all of the nine 500-ns-long trajectories using the Simulation Interaction Diagram tool from the Schrodinger suite. Here, among the other analyses, the protein–ligand interaction diagram was obtained in each case, where the occurrence of all of the important interactions were determined along the trajectories concerned (hydrogen bonds, hydrophobic interactions, water bridges, etc.). Moreover, the positions of the significant interactions on the ligands were also demonstrated in simplified 2D diagrams ( Supplementary Figures S2–S4 , boxed insets), as shown together with the interaction diagrams in the Supporting Information ( Figures S2–S4 ). Comparisons were also made between the interaction diagrams of the selective compounds and the diagrams of the less active compounds at each enzyme. However, neither a new secondary bond formation nor a unique interaction that might be solely responsible for the selectivity were found for any of the enzymes. It seemed that the patterns of the different interactions can help to explain the possible sources of the selectivity here. For example, for AKR1C1, the π–π staking of the A-ring of compound 2 _2I,4Br and the significant hydrophobic interactions, as well as the largest number of water-bridge connections, might together have resulted in 2 _2I,4Br having the strongest interaction with the AKR1C1 enzyme ( Supplementary Figure S2 ). For AKR1C2, with 2 _4Cl, the greater hydrophobic interactions with residue Trp86 and the larger number of water bridges might together override the similar interaction patterns of 2 _4I and 2 _2I,4Br, although these last two also show extra π–π stacking ( Supplementary Figure S3 ). Finally, for AKR1C3, the stabile interaction of the keto-oxygen in the D-ring with residue Ser118, and the less stable, but probably stronger, interaction with the negatively charged residue Asp224 might have been responsible for the strong binding. In summary here, we can say that there was no formation of new hydrogen or halogen bonds with the flexible loops that might have been responsible for the selectivity, although hydrophobic interactions might have particularly important roles in the selectivities of these compounds. Hence, the variations of atoms at positions 2 and 4 in the sterane skeletons might fine-tune these effects.

Melting points were determined with a Kofler hot-stage apparatus, and are uncorrected. Elemental analysis was performed with an organic elemental analyser (2400 CHN; Perkin-Elmer, Waltham, MA). Thin-layer chromatography was run on silica gel 60 F254 plates (layer thickness, 0.2 mm; Merck, Darmstadt, Germany) with 30% ethyl acetate/70% hexane as eluent. Detection was with I 2 or UV light (365 nm) after spraying with 5% phosphomolybdic acid in 50% aqueous phosphoric acid, and heating to 100–120 °C for 10 min. Flash chromatography was run on silica gel 60 plates (40–63 μm; Merck, Darmstadt, Germany). 1 H nuclear magnetic resonance (NMR) spectra were recorded in dimethylsulphoxide (DMSO)-d 6 or CDCl 3 solution (DRX-500; Bruker, Billerica, MA) at 500 MHz, with Me 4 Si as internal standard. 13 C NMR spectra were recorded with the same instrument at 125 MHz, and under the same conditions. Mass spectrometry provided the full scan mass spectra of the compounds using a triple quadrupole mass spectrometer (TSQ-7000; Finnigan-MAT, San Jose, CA), and were acquired in the range of 50 m/z to 1000 m/z , using an electrospray ionisation source (Finnigan, San Jose, CA). The analyses were performed in negative ion mode using flow injection mass spectrometry, with a mobile phase of 50% aqueous acetonitrile. The flow rate was 0.3 mL/min. Five microlitre aliquots of the samples were loaded into the flow. The electrospray ionisation capillary was adjusted to 4.5 kV, and N 2 was used as the nebuliser gas. The oestrone derivatives were synthesised as described elsewhere, except for those bearing different halogens at positions C-2 and C-4 23 , 27 . 4-Chloro-13α-methyl-oestrone 2 _4Cl (152 mg, 0.50 mmol) or 2-chloro-13α-methyl-oestrone 2 _2Cl (152 mg, 0.50 mmol) was dissolved in dichloromethane (5 mL), and N -bromosuccinimide (0.50 mmol) was added. The mixture was stirred at room temperature for 2 h, the solvent was evaporated off, and the crude product 2 _2Br,4Cl or 2 _2Cl,4Br was subjected to flash chromatography, with 10% ethyl acetate/90% hexane as eluent. Product 2 _2Br,4Cl (175 mg, 91%) was obtained as an oil. R f =0.46. Anal Calcd. for C 18 H 20 BrClO 2 : C, 56.34; H, 5.75. Found C, 56.47, H, 5.82%. 1 H NMR (DMSO-d 6 ) δ ppm: 0.96 (s, 3H, H-18), 2.55 and 2.81 (2xm, 2x1H, H-6), 7.38 (s, 1H, H-1), 9.64 (s, 1H, 3-OH). 13 C NMR (DMSO-d 6 ) δ ppm: 20.4 (CH 2 ), 24.4 (C-18), 27.1 (CH 2 ), 27.9 (CH 2 ), 28.1 (CH 2 ), 31.4 (CH 2 ), 32.8 (CH 2 ), 40.6 (CH), 48.1 (2C, 2x CH), 49.2 (C-13), 108.8 (C), 121.9 (C), 128.3 (C-1), 134.0 (C), 135.0 (C), 147.4 (C-3), 220.5 (C-17). MS: [M–H] – 381 (35Cl/79Br) and 383 (35Cl/81Br). Product 2 _2Cl,4Br (171 mg, 89%) was obtained as an oil. R f =0.46. Anal Calcd. for C 18 H 20 BrClO 2 : C, 56.34; H, 5.75. Found C, 56.49, H, 5.84%. 1 H NMR (DMSO-d 6 ) δ ppm: 0.96 (s, 3H, H-18), 2.56 and 2.82 (2xm, 2x1H, H-6), 7.38 (s, 1H, H-1), 9.65 (s, 1H, 3-OH). 13 C NMR (DMSO-d 6 ) δ ppm: 20.4 (CH 2 ), 24.4 (C-18), 27.1 (CH 2 ), 27.9 (CH 2 ), 28.1 (CH 2 ), 31.4 (CH 2 ), 32.8 (CH 2 ), 40.6 (CH), 48.1 (2C, 2x CH), 49.2 (C-13), 108.8 (C), 121.9 (C), 128.3 (C-1), 134.1 (C), 135.0 (C), 147.5 (C-3), 220.5 (C-17). MS: [M–H] – 381 (35Cl/79Br) and 383 (35Cl/81Br). 4-Chloro-13α-methyl-oestrone 2 _4Cl (152 mg, 0.50 mmol) or 2-chloro-13α-methyl-oestrone 2 _2Cl (152 mg, 0.50 mmol) was dissolved in trifluoroacetic acid (5 mL), and N -iodosuccinimide (0.50 mmol) was added. The mixture was stirred at room temperature for 2 h, and then poured into 100 mL water, and extracted with dichloromethane. The organic phase was separated, neutralised with ammonia solution, and washed with a saturated solution of sodium thiosulphate in water. The organic phase was dried over anhydrous sodium sulphate, filtered, and evaporated. The crude product was subjected to flash chromatography with 10% ethyl acetate/90% hexane as eluent. Product 2 _2I,4Cl (198 mg, 92%) was obtained as an oil. R f =0.50. Anal Calcd. for C 18 H 20 ClIO 2 : C, 50.19; H, 4.68. Found C, 50.26, H, 4.78%. 1 H NMR (DMSO-d 6 ) δ ppm: 0.96 (s, 3H, H-18), 2.56 and 2.82 (2xm, 2x1H, H-6), 7.55 (s, 1H, H-1), 9.64 (s, 1H, 3-OH). 13 C NMR (DMSO-d 6 ) δ ppm: 20.4 (CH 2 ), 24.4 (C-18), 27.2 (CH 2 ) , 28.0 (CH 2 ), 28.2 (CH 2 ), 31.4 (CH 2 ), 32.8 (CH 2 ), 37.1 (CH 2 ), 40.5 (CH), 48.1 (2C, 2x CH), 49.2 (C-13), 84.1 (C-4), 120.3 (C-2), 134.2 (C-1), 134.9 (C), 135.7 (C), 149.8 (C-3), 220.5 (C-17). MS m/z (%): 429 (100, [M–H] – ). Product 2 _2Cl,4I (194 mg, 90%) was obtained as an oil. R f =0.52. Anal Calcd. for C 18 H 20 ClIO 2 : C, 50.19; H, 4.68. Found C, 50.27, H, 4.76%. 1 H NMR (DMSO-d 6 ) δ ppm: 0.96 (s, 3H, H-18), 2.56 and 2.75 (2xm, 2x1H, H-6), 7.30 (s, 1H, H-1), 9.75 (s, 1H, 3-OH). 13 C NMR (DMSO-d 6 ) δ ppm: 20.4 (CH 2 ), 24.3 (C-18), 28.1 (CH 2 ), 28.3 (CH 2 ), 31.5 (CH 2 ), 32.8 (CH 2 ), 37.1 (CH2), 40.9 (CH), 48.1 (2C, 2x CH), 49.3 (C-13), 96.2 (C), 117.2 (C), 126.8 (C-1), 134.2 (C), 139.2 (C), 149.6 (C-3), 220.5 (C-17). MS m/z (%): 429 (100, [M–H] – ). 4-Bromo-13α-methyl-oestrone 2 _4Br (174 mg, 0.50 mmol) or 2-bromo-13α-methyl-oestrone 2 _2Br (174 mg, 0.50 mmol) was dissolved in trifluoroacetic acid (5 mL), and N -iodosuccinimide (0.50 mmol) was added. The mixture was stirred at room temperature for 2 h, and then poured into 100 mL water and extracted with dichloromethane. The organic phase was separated, neutralised with ammonia solution, and washed with a saturated solution of sodium thiosulphate in water. The organic phase was dried over anhydrous sodium sulphate, filtered, and evaporated. The crude product was subjected to flash chromatography with 10% ethyl acetate/90% hexane as eluent. Product 2 _2I,4Br (216 mg, 91%) was obtained as an oil. R f =0.50. Anal Calcd. for C 18 H 20 BrIO 2 : C, 45.50; H, 4.24. Found C, 45.62, H, 4.33%. 1 H NMR (DMSO-d 6 ) δ ppm: 0.96 (s, 3H, H-18), 2.56 and 2.76 (2xm, 2x1H, H-6), 7.59 (s, 1H, H-1), 9.41 (s, 1H, 3-OH). 13 C NMR (DMSO-d 6 ) δ ppm: 20.4 (CH 2 ), 24.4 (C-18), 27.5 (CH 2 ), 28.1 (CH 2 ), 31.5 (CH 2 ), 32.8 (CH 2 ), 39.5 (CH), 40.5 (CH), 48.1 (CH), 49.2 (C-13), 84.4 (C-2), 113.6 (C-4), 135.0 (C-1), 135.6 (C-10), 137.4 (C-5), 150.6 (C-3), 220.5 (C-17). MS: [M–H] – 472 (79Br) and 474 (81Br). Product 2 _2Br,4I (221 mg, 93%) was obtained as an oil. R f =0.52. Anal Calcd. for C 18 H 20 BrIO 2 : C, 45.50; H, 4.24. Found C, 45.60, H, 4.30%. 1 H NMR (DMSO-d 6 ) δ ppm: 0.96 (s, 3H, H-18), 2.54 and 2.73 (2xm, 2x1H, H-6), 7.43 (s, 1H, H-1), 9.52 (s, 1H, 3-OH). 13 C NMR (DMSO-d 6 ) δ ppm: 20.4 (CH 2 ), 24.3 (C-18), 28.2 (CH 2 ), 28.3 (CH 2 ), 31.5 (CH 2 ), 32.8 (CH 2 ), 37.2 (CH 2 ), 40.8 (CH), 48.1 (2C, 2x CH), 49.3 (C-13), 96.7 (C-2), 107.3 (C-4), 129.9 (C-1), 134.9 (C-10), 139.9 (C-5), 150.5 (C-3), 220.5 (C-17). MS: [M–H] – 472 (79Br) and 474 (81Br). The AKR1C1-3 recombinant enzymes were prepared as described previously 28 . The in vitro catalytic activities of AKR1C1–3 were determined spectrophotometrically by measuring increased NADH absorbance ( ε λ340 =6220 M −1 cm −1 ) in the presence of the chiral artificial substrate 1-acenaphthenol. The enzymatic reactions (300 µL) were performed in 0.09 M potassium phosphate buffer (pH 9.0), 0.005% (v/v) Triton X-114, 0.05% (v/v) DMSO, 2.3 mM NAD + , and 1-acenaphthenol (all Sigma). The final substrate concentrations (i.e. 1-acenaphthenol) were 90 µM, 180 µM, and 250 µM, for AKR1C1, AKR1C2, and AKR1C3, respectively. Five microlitres of each tested compound in DMSO was added to the reaction mixture, with the reactions started by addition of the enzymes, at 0.1 µM, 0.3 µM, and 1.5 µM for AKR1C1, AKR1C2, and AKR1C3, respectively. The measurements were performed in duplicate and were repeated as two independent experiments, using a microplate reader (PowerWave XS; Biotek, Winooski, VT). The initial velocities were calculated and the IC 50 values were determined from the plots of residual activity (RA) versus log 10 (inhibitor concentration), using GraphPad Prism, version 7.00 (GraphPad Software, Inc., San Diego, CA). Type of inhibition, K M , K I , and α were determined using either GraphPad Prism, version 7.00 (GraphPad Software, Inc., San Diego, CA) or SigmaPlot, version 14.0 (Systat Software, Inc., San Jose, CA). Docking calculations were performed with the Glide programme 29–31 from the Schrodinger suite 32 , using the XP protocol. Docking grid generation was based on the X-ray crystal geometry from the protein database ( http://www.rcsb.org ), and the graphical user interface Protein Preparation Wizard tool in Maestro 33 was applied to determine the positions of the missing hydrogens, side chains, and loops. The Protein Preparation Wizard step was augmented with 5-ns-long MD running with the Desmond module 34 from the Schrodinger suite 32 . The last frame of the MD calculation was considered as the target protein in the docking investigations. The XP docking protocol was applied in each case with the enhanced sampling method, and the energy window for the ring sampling was also increased to 100 kcal/mol, and the number of final outputs per ligand was increased to 10. Following the docking calculations, the best docking pose of each ligand was considered as the starting structure for a 500-ns-long MD simulation. To calculate the binding free energy (Δ G ) of the ligand–protein complex, the molecular mechanics generalised Born surface area (MMGBSA) method was applied for each MD trajectory, for 2500 dynamic trajectory points. The OPLS3e force field and simple point charge water model were applied in all of the MD calculations, and the MMGBSA values were determined by the thermal_mmgbsa python script from the Schrodinger suite. Standard error of means and mean Δ G values of a complex were determined by bootstrap calculations using an in-house script, where 100,000 bootstrap iterations were performed with eight randomly selected datapoints from the Δ G values. All of the figures were prepared with the Maestro programme 33 , which is the GUI part of the Schrodinger programme package.

The AKR1C enzymes are promising drug targets, as they are involved in the development of different cancers and several benign pathologies, and they are also associated with chemoresistance to platin and anthracycline-based drugs. Here, we synthesised 35 halogenated oestrone derivatives with low affinities for the nuclear oestrogen receptors, and evaluated their inhibitory actions against AKRC1, AKR1C2, and AKR1C3. Some potent inhibitors were identified, with occasional dual or triple inhibitory properties. Selective compounds were found against each of these three enzymes. Atomic level computational simulations showed that neither a well-defined unique chemical connection nor a specific interaction with a single amino acid could be identified in search of a source of selectivity regarding potent ligands. Overall, these data indicate that these halogenated oestrones represent a new class of potent and selective AKR1C inhibitors, and thus have the potential for development of new antitumour agents.

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