Open Access Article
This Open Access Article is licensed under a Creative Commons Attribution-Non Commercial 3.0 Unported Licence

Impact of the zinc complexation of polytopic polyaza ligands on the interaction with double and single stranded DNA/RNA and antimicrobial activity

Jorge González-García Dr. *a, Carolina Galiana Dr. b, M. Auxiliadora Dea-Ayuela Prof. b, Marijana Radić Stojković Dr. c, Sonia López-Molina Dr. a, Cristina Galiana-Roselló Dr. a, Salvador Blasco Dr. a, Ivo Piantanida Dr. *c and Enrique García-España Prof. *a
aInstitute of Molecular Science, University of Valencia, Department of Inorganic Chemistry, 46009, Paterna, Spain. E-mail: jorge.gonzalez@uv.es
bDepartment of Pharmacy, CEU Cardenal Herrera University, Ramón y Cajal s/n, 46115 Alfara del Patriarca, Spain
cDivision of Organic Chemistry & Biochemistry, Ruđer Bošković Institute, P. O. Box 180, 10002 Zagreb, Croatia

Received 7th February 2023 , Accepted 27th March 2023

First published on 27th March 2023


Abstract

Metal complexes have gained a huge interest in the biomedical research in the last decade because of the access to unexplored chemical space with regards to organic molecules and to present additional functionalities to act simultaneously as diagnostic and therapeutic agents. Herein, we evaluated the interaction of two polytopic polyaza ligands and their zinc complexes with DNA and RNA by UV thermal denaturation, fluorescence and circular dichroism spectroscopic assays. The zinc coordination was investigated by X-ray diffraction and afforded the structure of the binuclear zinc complex of PYPOD. Thermal denaturation of DNA and RNA and fluorimetry analysis revealed preferential binding of the zinc-PHENPOD complexes towards GC-containing DNA in contrast to the free ligands. On the other hand, PYPOD metal complexes, compared to the free ligand, stabilized AT-based DNA (B-form) better than AU-RNA (A-form). With regards to single stranded RNA, the binuclear complex of PHENPOD and the free ligand can efficiently identify polyadenylic acid (poly A) among other RNA sequences by circular dichroism spectroscopy. The antimicrobial activity in S. aureus and E. coli bacteria showed the highest activity for the free ligands and their trinuclear zinc complexes. This work can provide valuable insights into the impact of the nuclearity of polytopic polyaza ligands in the binding to DNA/RNA and the antimicrobial effect.


Introduction

During the past decades, metal complexes have become essential drugs in a broad range of therapies, covering cancer, pathogenic infections, diabetes, anti-inflammatory, and neurological disorders.1–3 Despite the clinical success of metal complexes for cancer, the landscape of inorganic compounds has been largely ignored for antimicrobial applications.4 Only, bismuth and silver-based complexes are currently used for treating microbial infections for Helicobacter pylori and topical wounds respectively.5–7 Nevertheless, the appearance of multidrug resistant microbes summed to the lack of drug candidates in clinical trials as antibiotics have prompted the scientific community to investigate non-organic compounds such as metal complexes. Recent studies have highlighted the ability of metal complexes to access underexplored chemical space for drug development8,9 and act through novel mechanisms of action.10 Subsequent antimicrobial drug screening campaigns indicated a higher hit-rate of metal complexes towards pathogens in comparison to natural and organic molecules.11,12

The vast majority of the metal complexes for therapeutical applications are mononuclear species, while polynuclear ones are poorly explored. In many cases, multinuclear complexes improved the biological activity of their mononuclear counterparts. For instance, the trinuclear platinum complex BBR3464 can overcome Cisplatin resistance in several cancer cell lines.13 Moreover, polynuclear complexes can show a synergetic and/or complementary effect between the metals when binding to biomolecules such as DNA, RNA, lipids or proteins as well as present additional functionalities such as imaging.14

Our team and other groups have extensively investigated polynuclear complexes, with particular attention to first-row metals such as zinc, copper and manganese.15–21 Recently, we described how the formation of binuclear complexes modulated the interaction of several ligands with DNA/RNA.22 We explored the increase of the antioxidant activity of polyaza binuclear manganese complexes in comparison with the mononuclear counterparts.23

In addition, we developed two polytopic polyaza ligands (PYPOD and PHENPOD, Scheme 1) and explored the zinc,24 copper,25,26 and manganese23 coordination in addition to the interaction with duplex (ds) DNA/RNA.27,28 Herein, we report the interaction of these ligands (see Scheme 1) and their mono- and polynuclear zinc metal complexes with the double and single stranded DNA/RNA by UV thermal, fluorescence emission and circular dichroism spectroscopies. The ligands form mono-, bi- and trinuclear complexes in solution according to potentiometry, photophysical and NMR studies. Moreover, we have characterised the structure of the binuclear zinc complex of PYPOD by X-ray analysis. Finally, the antibacterial activity of all the systems has been assessed in Gram-positive and Gram-negative bacteria.


image file: d3dt00395g-s1.tif
Scheme 1 Studied ligands.

Results and discussion

Synthesis and zinc coordination

The synthesis and characterisation of both ligands as well as their zinc coordination were reported in ref. 24. In brief, PYPOD and PHENPOD form mono-, bi- and trinuclear zinc complexes depending on the [M][thin space (1/6-em)]:[thin space (1/6-em)][L] molar ratio, the pH and the total concentration of the metal and ligand. We observed the formation of mono- and binuclear species above pH 3 for both ligands using 1[thin space (1/6-em)]:[thin space (1/6-em)]1 and 2[thin space (1/6-em)]:[thin space (1/6-em)]1 molar ratio. When using a 3[thin space (1/6-em)]:[thin space (1/6-em)]1 molar ratio, the trinuclear species are formed above pH 6.0 for PHENPOD and pH 9.0 for PYPOD. Using the stability constants, the speciation was calculated for the different molar ratio M[thin space (1/6-em)]:[thin space (1/6-em)]L used and at pH 7.4. For M[thin space (1/6-em)]:[thin space (1/6-em)]L 1[thin space (1/6-em)]:[thin space (1/6-em)]1, PYPOD has ZnH2L and Zn2HL as major species while PHENPOD shows ZnH2L and Zn2L. The species Zn2L was formed almost quantitatively for both ligands at pH 7.4 in ratio M[thin space (1/6-em)]:[thin space (1/6-em)]L 2[thin space (1/6-em)]:[thin space (1/6-em)]1. For the highest molar ratio M[thin space (1/6-em)]:[thin space (1/6-em)]L 3[thin space (1/6-em)]:[thin space (1/6-em)]1, PYPOD presents only the Zn2L species while PHENPOD presents the Zn2L species and a minor contribution of the dihydroxylated trinuclear Zn3L(OH)2 species. A detailed explanation of the speciation, stability constants and zinc coordination are reported in ref. 24.

Solid state analysis

We obtained suitable crystals for X-ray analysis of the binuclear Zn2+ complex with PYPOD from the slow evaporation in H2O–EtOH solution. In the crystal structure, the ligand PYPOD is forming the complex with formula [Zn2PYPODCl]3+ (Table S1 in ESI) in which each zinc atom is coordinated to one of the macrocyclic cavities. The complex is asymmetric as envisaged by the uneven number (11) of nitrogen donor atoms present in the ligand structure. Zn(1) is coordinated in an octahedral fashion to five nitrogen atoms, and to a chlorine atom, Cl(5) (see Fig. 1). On the other hand, Zn(2) is octahedrally coordinated by six nitrogen atoms, with the involvement of the nitrogen atom of the central pyridine spacer N(6) (Fig. 1). This coordination site exhibits a geometry very close to related mononuclear complexes of ligands containing just one macrocyclic unit and a 2-substituted pyridine linked to the aminoethyl pendant arm through a methylene bridge previously reported by us.29 The coordination to the two zinc atoms imposes a tight geometry to the whole complex, in which PYPOD adopts a twisted conformation. Both zinc atoms present bond lengths and angles very similar to each other, Zn–N bond distances range from 2.06 to 2.28 Å (see Table S2 in ESI). In both cases, the shortest bonds are those involving the pyridine nitrogen. Interestingly, Cl(5) is connected to a sodium atom which connects together two [Zn2PYPODCl]3+ units and one perchlorate moiety which forms the “supercomplex”30–32 {[Zn2PYPODCl]2Na(ClO4)}6+ (see Fig. 2). The asymmetric unit is composed of half of the “supercomplex” along with three perchlorate anions and one water molecule.
image file: d3dt00395g-f1.tif
Fig. 1 Mixed capped sticks/ball representation of the of the structure [Zn2PYPODCl]2·Na·7(ClO4)·2(H2O). Hydrogen atoms, perchlorate, water and sodium moieties omitted for clarity.

image file: d3dt00395g-f2.tif
Fig. 2 (a) Mixed capped sticks/ball representation of the “supercomplex” {[Zn2PYPODCl]2Na(ClO4)}6+ of the structure [Zn2PYPODCl]2·Na·7(ClO4)·2(H2O). Hydrogen atoms, counter ions and water molecules omitted for clarity. (b) Packing of “supercomplex”, coloured by symmetry operation. Hydrogen atoms, anions and water molecules are omitted for clarity.

DNA/RNA binding studies of Zn2+ complexes of PYPOD and PHENPOD

UV thermal denaturation experiments. First, we studied the interaction of the mono-, bi- and trinuclear Zn2+ complexes of the polytopic ligands with double-stranded DNA and RNA by UV thermal denaturation. These helical models contain different base composition that result in distinctive groove dimensions. The binding study was carried out with calf thymus DNA (ctDNA), the homopolymer poly dA–poly dT, the alternating polymer poly d(AT)2, as models for B-DNA, and poly rA–poly rU (RNA), as a model for A-form of nucleic acid.33 The potentiometric analysis allowed us to identify the species in solution at the pH value21 in which the assays were conducted, with the mononuclear species being predominant at a 1[thin space (1/6-em)]:[thin space (1/6-em)]1 molar ratio (L[thin space (1/6-em)]:[thin space (1/6-em)]M), the binuclear ones at a 1[thin space (1/6-em)]:[thin space (1/6-em)]2 molar ratio (L[thin space (1/6-em)]:[thin space (1/6-em)]M) and even the trinuclear species formed when using a 1[thin space (1/6-em)]:[thin space (1/6-em)]3 molar ratio for PHENPOD. The thermal denaturation experiments were conducted at two different molar ratios of L[thin space (1/6-em)]:[thin space (1/6-em)]ds-polynucleotide, 1[thin space (1/6-em)]:[thin space (1/6-em)]10 and 1[thin space (1/6-em)]:[thin space (1/6-em)]5 but only the former have been shown because both ratios provide similar results.

In general, both ligands induced a higher stabilisation effect as free ligands except for the interaction of PYPOD with poly dA–poly dT and PHENPOD with ctDNA (Fig. 3). The higher stabilisation effect induced by the ligands in contrast with the metal complexes suggests that the driving force of the interaction is mainly due to hydrogen bonding and/or electrostatics. The highly charged ligands interact strongly with the phosphate backbone and nucleobases (+4.19 and +4.33 for PYPOD and PHENPOD respectively at pH 7) whilst the metal coordination partially hinders the protonated amine groups and exerts a lower electrostatic interaction.


image file: d3dt00395g-f3.tif
Fig. 3 ΔTm values of PYPOD, PHENPOD and the corresponding zinc complexes with ds-polynucleotides.

Intriguingly, the higher stabilisation of the zinc complex of PYPOD with AT-based polynucleotide indicates a different and specific binding interaction with this nucleic acid with regards to ctDNA or AU-RNA. Considering the features of poly dA–poly dT with a narrower and deeper minor groove compared to a common B-form, it could be suggested that the coordination with the zinc ions allows for a better accommodation of the metal complexes within the minor groove and more efficient hydrophobic and van der Waals interactions.

Surprisingly, the trinuclear zinc complexes of PHENPOD modulate the interaction towards the destabilization of both AT- and AU-based polynucleotides (Fig. 3 purple bar), suggesting that the third Zn2+ possesses an unsaturated coordination sphere and interacts with A-only-based duplex probably via coordinative binding. However, thermal denaturation analysis revealed that zinc complexes of PHENPOD stabilised better ctDNA than the free ligand. It is probably the result of the mixed base-pair composition of that natural polynucleotide (42% GC base pairs and 58% AT base pairs). In addition, we performed thermal denaturation experiments with the metal salts to exclude their potential influence on DNA/RNA stabilisation. The analysis showed slight or negligible stabilisation of polynucleotides even at the highest molar ratios compared to those used with the metal complexes.

Fluorescence assays of compounds with DNA/RNA. We then utilised fluorimetric titrations to estimate the strength of the interaction of the zinc-PHENPOD complexes with double- (ds-) and single-stranded (ss-) DNA/RNA. The addition of ds- and ss-polynucleotides to solution containing the mono-, the bi- or the trinuclear zinc complex of PHENPOD yielded the quenching of their fluorescence (see Fig. 4 and S1–8 in ESI). The binding affinity values obtained from fluorescence experiments are shown in Table 1 and are, in general, higher for poly dG–poly dC compared to other DNAs and RNAs. This result is consistent with the better stabilising effect of ctDNA (42% GC base pairs) shown by the metal complexes compared to the free PHENPOD (Fig. 3).
image file: d3dt00395g-f4.tif
Fig. 4 Fluorimetric titration of Zn3PHENPOD with poly dG–poly dC, c = 1 × 10−5 M, λexc = 320 in sodium cacodylate buffer I = 0.05 M, pH = 7.0. Red spectrum corresponds to the initial titration and blue spectrum to last one (left panel). Fitting of the titrations of Zn3PHENPOD with all ds-polynucleotides (right panel).
Table 1 Values of the binding constants (log[thin space (1/6-em)]Ka) of zinc-PHENPOD complexes of with ds- and ss-polynucleotides calculated from the fluorimetric titrations (λexc = 320 nm, λem = 374 nm, c = 1 × 10−5 M) at pH 7.4 (sodium cacodylate buffer, I = 0.05 M)
  ZnPHENPOD Zn2PHENPOD Zn3PHENPOD
a Value error log[thin space (1/6-em)]K ± 0.5. b The value was not determined.
ctDNA 4.63a 4.67 4.73
Poly rA–poly rU 4.47 4.87 4.99
Poly dA–poly dT 4.75 4.74
Poly dG–poly dC 5.43 5.56 4.88
 
Poly A 5.06 5.13 5.33
Poly G 4.76 4.67 5.27
Poly C 2.99 3.71 3.58
Poly U N.C.b 5.22 6.25


In addition, the values obtained ranged within the same order of the free ligand obtained at slightly lower pH (see ref. 24) indicating that the coordination do not enhance the binding affinity towards duplexes.

We also explored the interaction with single-stranded RNA polymers (poly A, poly G, poly C and poly U). All of them, except poly U, form well-organised helical structures in solution (Na Cacodylate, I = 0.05 M, pH = 7.4) due to the stacking between bases.

Addition of all ss-polymers induced a decrease in the fluorescence emission as it occurred with ds-polynucleotides (Fig. 4 and S5–8) and the binding affinities were determined and collected in Table 1. The values of binding affinity of mono-, bi- and trinuclear complexes are comparable for poly A and poly G. However, those become higher upon increasing the nuclearity for poly C and poly U suggesting that the metal confers additional interactions towards these specific ss-polynucleotides. Zn3PHENPOD displayed the highest affinity towards poly U (at least one order of magnitude) compared to other single-stranded RNAs.

Circular dichroism studies of the compounds with DNA/RNA. In order to get insight into the conformational changes of the secondary structure of polynucleotides, circular dichroism studies were performed with the most representative binuclear species of PHENPOD (Zn2PHENPOD) and the ligand alone (PHENPOD). Additionally, the appearance of induced CD signals (ICD) provides information about the binding mode between the ligands and the binuclear zinc complexes to polynucleotides.

Addition of either PHENPOD or Zn2PHENPOD to a solution of ctDNA showed similar changes in the CD spectra, namely, a decrease in the CD band intensity at 275 nm and a bathochromic shift of this positive band with an increase of the ratio, r (Fig. S9).

Intriguingly, experiments performed with AT-based polynucleotides showed different behaviour upon addition of the ligand or the zinc complex (Fig. 5). In the titration of poly dA–poly dT with PHENPOD at a higher ratio, r (r > 0.2, Fig. 5), a negative ICD band centred around 300 nm appeared in addition to an increase of the CD band at 260 nm. Similar changes indicative of mild polynucleotide condensation were visible in the titration of the same polynucleotide with PYPOD (see ref. 25).


image file: d3dt00395g-f5.tif
Fig. 5 CD titration of poly dA–poly dT with (a) PHENPOD and (b) Zn2PHENPOD or poly d(A–T)2 with (c) PHENPOD and (d) Zn2PHENPOD at different molar ratios r = [compound]/[polynucleotide] ([polynucleotide] = 1.0 × 10−5 M, buffer sodium cacodylate, I = 0.05 M at pH 7.4, compound is PHENPOD or Zn2PHENPOD.

The zinc complex Zn2PHENPOD showed minor changes in the polynucleotide CD maxima at 260 and 280 nm (see Fig. 5), suggesting that the conformation adopted by the metal complex hampers the interaction with this polynucleotide. In contrast to AT homopolymer, addition of either the ligand or the metal complex to solutions of alternating poly d(A–T)2 caused an inversion of the CD polynucleotide band at 260 nm. This could be the result of either a significant impact on DNA conformation or a strongly negative ICD spectrum of PHENPOD in that range (see Fig. 5).

Both GC-based polynucleotides showed minor and similar variations in the CD spectra (a small decrease (see Fig. S12) or increase (Fig. S13) in intensity of the CD band at 260 nm) upon addition of PHENPOD or Zn2PHENPOD. It is worth mentioning that poly A–poly U did not experience any variation of the CD spectra upon addition of either the ligand or the metal complex (Fig. S10).

To obtain further information about the binding mode of the metal complexes towards single-stranded polynucleotides, we performed CD experiments with PHENPOD and its binuclear complex. CD titrations with poly C, poly G and poly U exhibited a decrease in the CD band intensity at 260 nm suggesting minor changes in their conformation (Fig. S14–S16). Contrarily, both ligand and metal complex induced almost the complete loss of conformation of poly A (see a collapse in CD band intensities at 260 and 245 nm in Fig. S17). This could result from different binding interactions (potential for hydrogen bonds, van der Waals forces) compared to the other used ss-polynucleotides.

Bacterial activity. To assess the antibacterial capacity of the ligands and the metal complexes, we evaluated bacterial viability by monitoring the bacterial growth through the optical density at 600 nm. We selected two bacteria strains of different origins, the Gram-positive S. aureus and the Gram-negative E. coli.

We observed a concentration dependent activity for all the systems in E. coli (Fig. 6). As shown in Fig. 6, the most active systems were the free ligands and the zinc complexes of both ligands at the highest concentration used (100 μM). At a fixed treatment concentration of 25 μM, PHENPOD shows the highest inhibitory effect with 17% of cell viability followed by its mononuclear zinc complex (29%), binuclear complex (33%) and trinuclear complex (37%). The same trend was observed for PYPOD and their corresponding zinc complexes, suggesting that the increase of the zinc nuclearity in these polyaza complexes reduces the inhibitory effect in E. coli. However, PHENPOD and its trinuclear zinc complex showed a higher inhibitory effect at 50 μM than the mono- and binuclear complex of PHENPOD (Fig. 6b).


image file: d3dt00395g-f6.tif
Fig. 6 Cell viability analysis in E. coli based on the optical density at 600 nm for PYPOD, ZnPYPOD, Zn2PYPOD and Zn3PYPOD (top panel) and for PHENPOD, ZnPHENPOD, Zn2PHENPOD and Zn3PHENPOD. Legends represent the concentration in μM.

In contrast to E. coli, assays with S. aureus showed cell inhibition of all, free ligands and their mono-, bi- and trinuclear zinc complexes, only at 100 μM (see Fig. S18 and S19), suggesting that this bacteria strain is less sensitive than E. coli. Considering the type of bacteria, polyamine-based ligands and the zinc complexes exhibit a higher antibacterial effect on Gram-negative bacteria, although the bacteria present the outer membrane of glycerophospholipids, which hinders the uptake and effect of the antibiotics.

Conclusions

Metal complexes have gained a huge interest in the biomedical research in the last decade because they provide access to chemical space unexplored by organic molecules. Here we have studied the interaction of mono- and polynuclear zinc complexes of two polytopic polyaza ligands (PYPOD and PHENPOD) with double and single stranded DNA/RNA and evaluated their antibacterial inhibitory effect.

The crystal structure of the binuclear zinc complex of PYPOD ([Zn2PYPODCl]3+) shows asymmetric coordination sites, in agreement with the analysis of the stability constants obtained in previous works.21 Both zinc centres are coordinated to the four nitrogen atoms of each macrocyclic moiety and the nitrogen of the pendant arm, while one zinc is coordinated to the central pyridine spacers and the other one to a chloride.

In general, the free ligands show a higher stabilisation effect on DNA and RNA duplexes than the mono-, bi- and trinuclear zinc complexes. It indicates that the interaction is governed by the net charge of the systems since the ligands possess a higher net charge than the metal complexes at the pH of study. Only the polynuclear zinc complexes of PYPOD exhibit a stronger stabilisation for poly dA–poly dT, which can be rationalised because the zinc complexes are better accommodated into the narrower and deeper minor groove of this B-form of DNA.

By using fluorimetric experiments, the zinc complexes show a higher affinity for GC-duplex which is not affected by the nuclearity of the complexes. Concerning single stranded RNA, poly A has comparable affinity for complexes of different nuclearity whereas poly C, poly G and poly U show an increase in affinity as the number of zinc centres in the complex increases. Circular dichroism spectra show that the binuclear complex of PHENPOD and the free ligand permit to identify poly A from other single stranded RNA sequences.

Lastly, antibacterial studies of the free ligands and the metal complexes in S. aureus and E. coli yield a higher inhibitory effect of the free ligands than the mono-, bi- and trinuclear zinc complexes. In addition, the ligands have higher antibacterial activity on the Gram-negative E. coli than on the Gram-positive bacteria S. aureus. It can be associated to the more negative charged membrane of E. coli, which can thus bind stronger to the highly positively charged ligands.

Thus, this work provides important insights into the interaction of free polyaza ligands and their corresponding zinc complexes with double and single stranded DNA/RNA as well as on the antimicrobial effect on two bacteria. The provided results will assist to constructing new systems to tackle contemporary issues such as antimicrobial resistance or DNA/RNA sensing using polynuclear metal complexes.

Experimental

Materials and apparatus

The UV-vis spectra and fluorescence spectra were recorded with a Varian Cary 100 Bio spectrometer and an Eclipse fluorimeter, respectively. The CD spectra were registered with a JASCO J815 spectropolarimeter at 25.0 °C. Appropriate quartz cuvettes (path length: 1 cm) were used in all cases. Polynucleotides poly d(AT)2, poly A–poly U, poly dA–poly dT, poly d(AT)2, poly dG–poly dC, calf thymus ctDNA, poly A, poly C, poly G and poly U were purchased from Merck, and dissolved in sodium cacodylate buffer, I = 0.05 M, pH = 7.0. The ctDNA was additionally sonicated and filtered through a 0.45 mm filter to obtain mostly short (ca. 100 base pairs) rod-like β-helical DNA fragments.34 The polynucleotide concentration was determined spectroscopically as the concentration of phosphates (corresponds to c(nucleotide)).35

Fluorimetric titrations and calculation of binding constants

Fluorimetric titrations were performed by adding aliquots of polynucleotide stock solutions to a solution of PHENPOD and Zn2PHENPOD (c = 1 × 10−5 M), using λexc = 320 nm and monitoring the change in emission (λem = 374 nm) in sodium cacodylate buffer I = 0.05 M, pH = 7.0. The titrations were analysed according to the independent-site model by non-linear fitting to eqn (1),36 in which F0 is the initial fluorescence intensity in the absence of DNA, Q is the fluorescence enhancement upon saturation, A = [Kac(complex)]−1 and x = nc(DNA)c(complex)−1, n is the putative number of binding sites on a given polynucleotide matrix. The parameters Q and A were found by a Levenberg–Marquardt fitting routine using the Origin 8.5 software, whereas n was varied to obtain the best fit.
 
image file: d3dt00395g-t1.tif(1)

Circular dichroism spectroscopy

Circular dichroism (CD) spectra were recorded with a scanning speed of 200 nm min−1 (an average of three accumulations). The buffer background was subtracted from each spectrum. CD experiments were performed by adding portions of the compound stock solution into a solution of polynucleotide (c(DNA) = 1 × 10−5 M).

UV thermal denaturation experiments

Thermal melting curves for ds-DNA, ds-RNA, with and without the complexes were determined by following the absorption change at 260 nm as a function of temperature.37 The initial absorbance of the ligands was subtracted from every curve, and the absorbance scale was normalized. Tm values are the midpoints of the transition curves determined from the maximum of the first derivative and checked graphically by the tangent method. The ΔTm values were calculated by subtracting the Tm of the free nucleic acid from the Tm of the complex. Every ΔTm value reported is the average of at least two measurements. The error in ΔTm is ±0.5 °C.

Crystallographic structure determination

Crystals of [Zn2PYPODCl]Na0.53.5(ClO4)H2O suitable for single crystal X-ray diffraction were measured in an Enraf-Nonius KAPPA CCD single-crystal diffractometer using MoKα radiation (λ = 0.71073 Å). The structure was solved by direct methods using SIR2004.38 The structure obtained was refined using least-squares refinement, isotropically at the beginning and then anisotropically by means of the program SHELXL-2018.39 An empirical absorption correction was applied using PLATON's MULABS routine.40 Hydrogen atoms were placed using a riding model with the appropriate restraints, except for the solitary water molecule for which the hydrogen atoms were fixed taking into account the surrounding hydrogen bond network. Crystal data, data collection parameters, and results of the analyses are listed in Tables S1 and S2. The crystal data has been deposited in the CSD database with deposition number 2191006.

Assessment of the antibacterial activity

S. aureus CECT 239 and E. coli CECT 405 were maintained in Mueller-Hinton (MH) broth or agar at 37 °C. The antibacterial activity was evaluated by the broth microdilution plate method according to CLSI criteria against ESKAPE pathogens. Briefly, serial dilutions of the compounds were prepared in MHB (1[thin space (1/6-em)]:[thin space (1/6-em)]2 dilutions) in 96-well plates. Ciprofloxacin was used as the positive control. An initial inoculum of every strain was prepared at 0.5 McFarland in water and immediately diluted in MHB (1[thin space (1/6-em)]:[thin space (1/6-em)]20). Then, plates were inoculated with 5 μL of the bacterial dilution leading to a concentration of 5 × 105 CFU mL−1 and incubated at 37 °C for 18–20 h. The uninoculated broth was used as the sterility control and the inoculated broth without drugs was used as the growth control.

Author contributions

J. G.-G. performed the nucleic acids experiments. S. L.-M., C. G., C. G.-R. and M. A. D.-A. conducted the bacterial assays. S. B. diffracted and analysed the X-ray structure. I. P., E. G.-E., M. R. S. and J. G.-G. supervised and obtained the funding. J. G.-G. wrote the original manuscript. I. P., E. G.-E., M. R. S. and J. G.-G. reviewed and edited the final draft.

Conflicts of interest

There are no conflicts to declare.

Acknowledgements

This research was funded by the Spanish Ministry for Science and Innovation, The National Research Agency and FEDER funds from the EU (grants PID2019-110751RB-I00, PID2019-108643GA-I00, EIN2020-112428, MFA/2022/014, RED2018-102331-T and CEX2019-000919) and the Conselleria de Innovación, Universidades, Ciencia y Sociedad Digital of the Generalitat Valenciana (CIDEGENT/2018/015 y PROMETEO Grant CIPROM/2021/030). This contribution is also based upon work from COST Action CA18202, NECTAR - Network for Equilibria and Chemical Thermodynamics Advanced Research, supported by COST (European Cooperation in Science and Technology). This study forms part of the Advanced Materials programme and was supported by MCIN with funding from European Union NextGenerationEU (PRTR-C17.I1) and by Generalitat Valenciana.

References

  1. K. D. Mjos and C. Orvig, Chem. Rev., 2014, 114, 4540–4563 CrossRef CAS PubMed.
  2. S. Medici, M. Peana, V. M. Nurchi, J. I. Lachowicz, G. Crisponi and M. A. Zoroddu, Coord. Chem. Rev., 2015, 284, 329–350 CrossRef CAS.
  3. T. W. Hambley, Dalton Trans., 2007, 43, 4929–4937 RSC.
  4. E. J. Anthony, E. M. Bolitho, H. E. Bridgewater, O. W. L. Carter, J. M. Donnelly, C. Imberti, E. C. Lant, F. Lermyte, R. J. Needham, M. Palau, P. J. Sadler, H. Shi, F.-X. Wang, W.-Y. Zhang and Z. Zhang, Chem. Sci., 2020, 11, 12888–12917 RSC.
  5. D. M. Griffith, H. Li, M. V. Werrett, P. C. Andrews and H. Sun, Chem. Soc. Rev., 2021, 50, 12037–12069 RSC.
  6. R. Wang, H. Li, T. K.-Y. Ip and H. Sun, Adv. Inorg. Chem., 2020, 75, 183–205 CrossRef CAS.
  7. W. Sim, R. T. Barnard, M. A. T. Blaskovich and Z. M. Ziora, Antibiotics, 2018, 7, 93 CrossRef CAS PubMed.
  8. J.-Y. Maillard and P. Hartemann, Crit. Rev. Microbiol., 2013, 39, 373–383 CrossRef CAS PubMed.
  9. C. N. Morrison, K. E. Prosser, R. W. Stokes, A. Cordes, N. Metzler-Nolte and S. M. Cohen, Chem. Sci., 2020, 11, 1216–1225 RSC.
  10. T. GIanferrara, I. Brastos and E. Alessio, Dalton Trans., 2009, 7588–7598 RSC.
  11. A. Frei, J. Zuegg, A. G. Elliott, M. Baker, S. Braese, C. Brown, F. Chen, C. G. Dowson, G. Dujardin, N. Jung, A. P. King, A. M. Mansour, M. Massi, J. Moat, H. A. Mohamed, A. K. Renfrew, P. J. Rutledge, P. J. Sadler, M. H. Todd, C. E. Willans, J. J. Wilson, M. A. Cooper and M. A. T. Blaskovich, Chem. Sci., 2020, 11, 2627–2639 RSC.
  12. A. Frei, Antibiotics, 2020, 9, 90 CrossRef CAS PubMed.
  13. J. Wheate and J. G. Collins, Coord. Chem. Rev., 2003, 241, 133–145 CrossRef.
  14. R. Lengacher, A. Marlin, D. Smilowics and E. Boros, Chem. Soc. Rev., 2022, 51, 7715–7731 RSC.
  15. L. Guijarro, M. Inclan, J. Pitarch-Jarque, A. Domenech-Carbo, J. U. Chicote, S. Trefler, E. Garcia-Espana, A. Garcia-Espana and B. Verdejo, Inorg. Chem., 2017, 56, 13748–13758 CrossRef CAS PubMed.
  16. A. Martinez-Camarena, M. Savastano, S. Blasco, E. Delgado-Pinar, C. Giorgi, A. Bianchi, E. Garcia-España and C. Bazzicalupi, Inorg. Chem., 2022, 61, 368–383 CrossRef CAS PubMed.
  17. L. Acosta-Rueda, E. Delgado-Pinar, J. Pitarch-Jarque, A. Rodriguez, S. Blasco, J. Gonzalez, M. G. Basallote and E. Garcia-Espana, Dalton Trans., 2015, 44, 8255–8266 RSC.
  18. M. Inclán, M. T. Albelda, J. C. Frías, S. Blasco, B. Verdejo, C. Serena, C. Salat-Canela, M. L. Díaz, A. García-España and E. García-España, J. Am. Chem. Soc., 2012, 134, 9644–9656 CrossRef PubMed.
  19. G. Ambrosi, M. Formica, V. Fusi, L. Giorgi, A. Guerri, M. Micheloni, P. Paoli, R. Pontellini and P. Rossi, Inorg. Chem., 2007, 46, 4737–4748 CrossRef CAS PubMed.
  20. G. Ambrosi, M. Formica, V. Fusi, L. Giorgi, E. Macedi, M. Micheloni, P. Paoli and P. Rossi, Inorg. Chem., 2009, 48, 10424–10434 CrossRef CAS PubMed.
  21. G. Ambrosi, C. Battelli, M. Formica, V. Fusi, L. Giorgi, E. Macedi, M. Micheloni, R. Pontellini and L. Prodi, New J. Chem., 2009, 33, 171–180 RSC.
  22. L. Guijarro, A. Martinez-Camarena, J. U. Chicote, A. Garcia-Espana, E. Garcia-Espana, M. Inclan, B. Verdejo and J. Gonzalez-Garcia, Molecules, 2021, 26, 3957 CrossRef CAS PubMed.
  23. J. González-García, Á. Martínez-Camarena, B. Verdejo, M. P. Clares, C. Soriano, E. Garcia-España, H. R. Jimenez, A. Domenech-Carbo, R. Tejero, E. Calvo, L. Briansó-Llort, C. Serena, S. Trefler and A. Garcia-España, J. Inorg. Biochem., 2016, 163, 230–239 CrossRef PubMed.
  24. J. González, J. M. Llinares, R. Belda, J. Pitarch, C. Soriano, R. Tejero, B. Verdejo and E. García-España, Org. Biomol. Chem., 2010, 8, 2367–2376 RSC.
  25. C. E. Castillo, M. A. Máñez, J. González, J. M. Llinares, H. R. Jimenez, M. G. Basallote and E. García-España, Chem. Commun., 2010, 46, 6081–6083 RSC.
  26. C. E. Castillo, J. González-García, J. M. Llinares, M. A. Máñez, H. R. Jimenez, E. García-España and M. G. Basallote, Dalton Trans., 2013, 42, 6131–6141 RSC.
  27. J. González-García, L. Uzelac, M. Kralj, I. Piantanida and E. García-España, Org. Biomol. Chem., 2013, 11, 2154–2161 RSC.
  28. M. R. Stojkovic, J. Gonzalez-Garcia, F. Supljika, C. Galiana-Rosello, L. Guijarro, S. A. Gazze, L. W. Francis, I. Piantanida and E. Garcia-España, Int. J. Biol. Macromol., 2018, 109, 143–151 CrossRef CAS PubMed.
  29. S. Blasco, B. Verdejo, M. P. Clares, C. E. Castillo, A. G. Algarra, J. Latorre, M. A. Máñez, M. G. Basallote, C. Soriano and E. García-España, Inorg. Chem., 2010, 49, 7016–7027 CrossRef CAS PubMed.
  30. A. Bencini, A. Bianchi, E. Garcia-Espana, M. Giusti, S. Mangani, M. Micheloni, P. Orioli and P. Paoletti, Inorg. Chem., 1987, 26, 3902–3907 CrossRef CAS.
  31. A. Bencini, A. Bianchi, P. Dapporto, E. García-España, M. Micheloni, J. A. Ramirez, P. Paoletti and P. Paoli, Inorg. Chem., 1992, 31, 1902–1908 CrossRef CAS.
  32. J. Aragó, A. Bencini, A. Bianchi, A. Domenech and E. García-España, J. Chem. Soc., Dalton Trans., 1992, 319–324 RSC.
  33. S. Neidle, Oxford handbook of nucleic acid structure, Oxford University Press, Oxford, UK, 1999 Search PubMed.
  34. I. Orehovec, D. Glavac, I. Dokli, M. Gredicak and I. Piantanida, Croat. Chem. Acta, 2017, 90, 603–611 CrossRef.
  35. J. D. McGhee and P. H. Von Hippel, J. Mol. Biol., 1974, 86, 469–489 CrossRef CAS PubMed.
  36. F. H. Stootman, D. M. Fisher, A. Rodger and J. R. Aldrich-Wright, Analyst, 2006, 131, 1145–1151 RSC.
  37. J. L. Mergny and L. Lacroix, Oligonucleotides, 2003, 13, 515–537 CrossRef CAS PubMed.
  38. M. C. Burla, R. Caliandro, M. Camalli, B. Carrozzini, G. L. Cascarano, L. De Caro, C. Giacovazzo, G. Polidori and R. Spagna, J. Appl. Crystallogr., 2005, 38, 381–388 CrossRef CAS.
  39. G. M. Sheldrick, Acta Crystallogr., Sect. C: Struct. Chem., 2015, 71, 3–8 Search PubMed.
  40. R. H. Blessing, Acta Crystallogr., Sect. A: Found. Crystallogr., 1995, 51, 33–38 CrossRef PubMed.

Footnote

Electronic supplementary information (ESI) available. CCDC 2191006. For ESI and crystallographic data in CIF or other electronic format see DOI: https://doi.org/10.1039/d3dt00395g

This journal is © The Royal Society of Chemistry 2023
Click here to see how this site uses Cookies. View our privacy policy here.