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Article

Antimicrobial Properties of New Polyamines Conjugated with Oxygen-Containing Aromatic Functional Groups

by
Mario Inclán
1,2,*,
Neus Torres Hernández
1,
Alejandro Martínez Serra
1,
Gonzalo Torrijos Jabón
3,
Salvador Blasco
1,
Cecilia Andreu
4,*,
Marcel lí del Olmo
3,
Beatriz Jávega
5,
José-Enrique O’Connor
5 and
Enrique García-España
1
1
Institute of Molecular Science, University of Valencia, 46980 Valencia, Spain
2
Escuela Superior de Ingeniería, Ciencia y Tecnología, International University of Valencia—VIU, 46002 Valencia, Spain
3
Departament de Bioquímica i Biologia Molecular, Facultat de Biologia, University of Valencia, 46100 Valencia, Spain
4
Departament de Química Orgànica, Facultat de Farmàcia, University of Valencia, 46100 Valencia, Spain
5
Laboratory of Cytomics, Joint Research Unit CIPF-UVEG, Department of Biochemistry and Molecular Biology, Faculty of Medicine, University of Valencia, 46010 Valencia, Spain
*
Authors to whom correspondence should be addressed.
Molecules 2023, 28(22), 7678; https://doi.org/10.3390/molecules28227678
Submission received: 10 October 2023 / Revised: 9 November 2023 / Accepted: 16 November 2023 / Published: 20 November 2023
(This article belongs to the Special Issue Polyamine Drug Discovery)
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Abstract

:
Antibiotic resistance is now a first-order health problem, which makes the development of new families of antimicrobials imperative. These compounds should ideally be inexpensive, readily available, highly active, and non-toxic. Here, we present the results of our investigation regarding the antimicrobial activity of a series of natural and synthetic polyamines with different architectures (linear, tripodal, and macrocyclic) and their derivatives with the oxygen-containing aromatic functional groups 1,3-benzodioxol, ortho/para phenol, or 2,3-dihydrobenzofuran. The new compounds were prepared through an inexpensive process, and their activity was tested against selected strains of yeast, as well as Gram-positive and Gram-negative bacteria. In all cases, the conjugated derivatives showed antimicrobial activity higher than the unsubstituted polyamines. Several factors, such as the overall charge at physiological pH, lipophilicity, and the topology of the polyamine scaffold were relevant to their activity. The nature of the lipophilic moiety was also a determinant of human cell toxicity. The lead compounds were found to be bactericidal and fungistatic, and they were synergic with the commercial antifungals fluconazole, cycloheximide, and amphotericin B against the yeast strains tested.

Graphical Abstract

1. Introduction

Antimicrobial resistance (AMR) has become a major global health problem. The estimates in 2016 painted a grim picture noting that AMR would become the leading cause of death, with a likelihood of 10 million deaths per year by 2050 [1]. However, other studies published in 2022 were more pessimistic about the situation, demonstrating that the previous prediction was probably an underestimation and that the mortality rate associated with AMR is increasing at a worrying pace: There were already close to 5 million deaths associated with bacterial AMR in 2019 [2]. The classical solution against AMR consists of developing new families of antimicrobials. However, there are several drawbacks for many of the compounds currently under clinical trials, such as their high cost of production, which is related to the complexity of their synthesis, and, in the case of natural products, the scarcity of sources [3].
Polyamines are simple organic molecules with two or more amine groups positively charged at physiological pH. Biogenic polyamines, such as putrescine, spermidine, and spermine, are widely distributed in all organisms in which they develop multiple cellular functions. Their metabolic synthesis and concentration are highly regulated due to their role in cell proliferation and apoptotic processes. Polyamines are also involved in several signalling pathways, can act as neuromodulators, and influence the properties of several neurotransmitter pathways involved in mental disorders [4]. The multiple activities induced by polyamines as a result of their interaction with different biological targets support the proposal highlighting the polyamine skeleton as a universal template model in which appropriate structural modifications would provide selectivity on specific processes [5,6].
Exogenous polyamines are efficiently absorbed by transport systems, and as endogenous ones, they can also affect different biological targets. In recent decades, polyamine research has become an important field for drug development, and their potential application as anticancer and antiproliferative agents, agonist–antagonist receptor ligands, or antiparasitic compounds, among others, has been studied [4]. The activity of novel polyamines against Gram-positive and Gram-negative bacteria has been analysed by different research groups, and they have found promising compounds with antibacterial and/or antibiofilm activity and sometimes with synergic effects on other known antimicrobial compounds. The positive charges of the amino groups have been considered a key factor in their antimicrobial activity [7,8,9,10,11]. Conjugated polyamines with lipophilic organic molecules have also been found effective in this context; in these cases, the structure and characteristics of the organic moiety play an important role in antimicrobial activities [12,13,14,15,16].
1,3-Benzodioxole is a naturally occurring organic group found in many plant-based food products, such as vanilla (piperonal), black pepper (piperine), and cinnamon (safrole), among others. More importantly, its aldehyde (2H-1,3-benzodioxole-5-carbaldehyde) is mass-produced, cheap, and readily available since it is widely used by the industry developing artificial flavours and perfumes. 1,3-benzodioxole is also exploited in the pharmaceutical industry, and it can be found as a component of many bioactive molecules. Among the pharmaceuticals bearing this unit, there are examples in the literature highlighting their use in anticancer drugs [17], HIV treatments [18], antiparkinsonian agents [19], anti-inflammatory or analgesic products [20,21], and anticonvulsant remedies [22]. It is also present in a natural pesticide, acting both as an algicide and a herbicide [23]. Another group of bioactive compounds bearing this moiety is psychoactive and stimulant drugs [24,25]. There are also examples of its derivatives that show antimicrobial activity [26,27,28,29,30].
In this context, with the purpose of developing new antimicrobial compounds, we set out to study the activities of various polyamines containing the 1,3-benzodioxole moiety. The polyamine core varied in the number of amine groups and its topology (linear, tripodal, and macrocyclic). Therefore, we determined the antimicrobial activity against bacteria (Escherichia coli and Staphylococcus aureus) and yeast. The possible synergies between them and commercial antimicrobials and their toxicity against a human cell line were also determined. These results allowed us to conclude that the topology of the polyamine scaffold was a determinant of the activity. We then extended the study to three other derivatives in which we conjugated the most promising polyamine macrocyclic core with three alternative oxygen-containing aromatic groups. It is also worth mentioning that all these compounds were prepared in good yields through a simple one-pot synthetic method, which is robust and easily scalable.

2. Results and Discussion

2.1. Synthesis

The structures of the first polyamines used in this work are shown in Figure 1. Considering these compounds, 1b–3b were commercially purchased. The synthesis of 4b and 5b has been optimised in our laboratory, and the compounds are systematically prepared [31,32,33,34]. The conjugated derivatives 1a–5a were obtained in the multigram scale in one-pot reactions and under mild conditions.
For the conjugation of the aromatic moiety, selective condensation between 3,4-methylenedioxybenzaldehyde (commonly known as piperonal or heliotropin) and the primary amino groups of the corresponding polyamine (1b–5b) in the proper stoichiometry was carried out. Then, the intermediate imine was reduced in situ with NaBH4 (Scheme 1). The purification to obtain spectroscopically pure compounds was easily achieved via simple precipitation and the recrystallisation of the hydrochloride salts.
To our knowledge, the synthesis of compounds 1a–5a is reported here for the first time, except for 3a, which was described before by Sumoto’s group [26], but with a different procedure to the one reported here. The 1H, 13C, and ATR-IR spectra of the new compounds, as well as the X-ray diffraction structure of compound 3a, can be found in the Electronic Supplementary Materials.

2.2. Basicity of the Receptors

The capacity of a given compound to interact with its biomolecular target depends heavily on factors such as the overall charge of the molecule and the number of hydrogen bond donor/acceptor atoms. Since the polyamines presented here are polyprotic systems, understanding which species are present in the solution at the experimental pH values is essential. For this reason, potentiometric titrations in water were carried out.
The stepwise protonation constants obtained are shown in Table 1. As expected, in the studied pH range (2.5 < pH < 10.5), the compounds display as many protonation constants as the secondary amino groups present in each molecule. The protonation reactions of the central tertiary nitrogen atoms (in the case of 3a, 4a, and 5a) or the pyridine nitrogen (in 5a) were not detected since they tend to occur at a pH that falls outside the lower range of the analysis technique. This was expected considering the known lower basicity of tertiary amines in water and the electrostatic repulsion of the surrounding ammonium groups [35].
As anticipated, the overall basicity correlates with the number of secondary amino groups, with 4a having the higher value, in terms of its six amino groups. Compounds 1a, 3a, and 5a, with three secondary amino groups in their structures, have similarly low-log β values. By contrast, 2a, with four secondary amino groups, shows an intermediate basicity. These protonation constants allowed us to build the corresponding distribution diagrams (Figure S5 in the Supplementary Materials) and to calculate the percentage of species and the average number of positive charges (n) at pH 7.4 (last row in Table 1).

2.3. Determination of the Antimicrobial Activity

The antimicrobial activity of the polyamines was determined using a Gram-negative bacteria (Escherichia coli JM101), a Gram-positive bacteria (Staphylococcus aureus BH1), and two strains of the yeast Saccharomyces cerevisiae (laboratory strain BY4741 carrying the YEplac195 plasmid or its derived one YEplac195-PDR5, named PDR5 from now on). This plasmid allows for the overexpression of the gene encoding Pdr5, an ATP-binding cassette (ABC) transporter, which can export toxic substances out of the cell (see [36] and references therein). For comparison purposes, commercial antibacterial (doxycycline, gentamicin, ciprofloxacin, and ampicillin) and antifungal (fluconazole, cycloheximide, and amphotericin B) agents were also included as control in our analyses. The organic compound 1,3-benzodioxole was also considered with both kinds of microorganisms. To obtain information about their antimicrobial activities, experiments were carried out to determine the minimal inhibitory concentration (MIC), the minimal microbicidal concentration (MMC), and possible synergies with the control substances.

2.3.1. Determination of the Minimal Inhibitory Concentration (MIC)

The results obtained for the MIC are shown in Table 2. The most relevant observation regarding the antibacterial MIC values was the important differences between the unsubstituted polyamines 1b–4b and the ones combined with 1,3-benzodioxole 1a–4a. Only polyamine 5b had, in some cases, a similar or better behaviour than the conjugated compounds. This fact, together with the higher MIC value measured for the lowest-molecular-mass compound 1,3-benzodioxole seems to indicate that the activity in the conjugated derivatives is mainly due to the polyamine moiety. It is also worth mentioning that for the biogenic polyamines spermidine (1b) and spermine (2b), the obtained results agree with the data found in the literature about their antimicrobial activity. Based on these data and the results presented in this study, spermidine 1b and its conjugated derivative 1a showed MIC values similar to or higher than spermine 2b and its derivative 2a against E. coli [37], S. aureus, and the yeast strains. Considering the conjugated polyamines, the best antibacterial activity was found for 4a and 5a, followed by 3a and 2a. Polyamine 5b was also very effective against E. coli.
In yeast, like in bacteria, conjugated compounds 4a and 5a and polyamine 5b showed the best results. For the commercial drug fluconazole, the susceptibility of the strain overexpressing Pdr5 protein was much higher due to its involvement in the efflux of this drug [38]. However, in the case of the new compounds considered here, no differences between the two yeast strains were found, which demonstrates that Pdr5 is not involved in their efflux.
The fact that, in most cases, the antimicrobial activity was much higher in the conjugated polyamines containing 1,3-benzodioxole than in each one of the pair of components seems to indicate that their association improves some properties, probably related to the increased lipophilicity provided by the 1,3-benzodioxole fraction. Only the results of polyamine 5b are comparable (and even better especially in yeasts) to those obtained with conjugated polyamines. This could also be explained by considering that it is the most lipophilic polyamine, as deduced from its ClogD value (see the last column in Table 2, in which ClogD values at physiological pH are indicated).
According to their topology, the studied polyamines can be classified as linear (1 and 2), tripodal (3 and 4), and macrocyclic (5). Moreover, regarding the whole charge that they have at physiological conditions (pH = 7.4), we found that compounds 1a, 3a, and 5a have between +2.1 and +2.7 charges; 2a has +3.4; and 4a has +4.5. In the case of both tripodal compounds (3a and 4a), or both linear ones (1a and 2a), the activity was higher in the derivative with an upper charge. However, the main factor determining the activity seems to be the topology, because comparing the three compounds with similar charge (1a, 3a, and 5a), higher activity is shown (except for S. aureus) by macrocyclic compound 5a followed by the tripodal one 3a (see Figure 2). Moreover, it was similar or higher for macrocyclic derivative 5a, with a whole charge of +2.4, than for the tripodal 4a and the linear 2a with charges of +4.5 and +3.4, respectively.
Figure 3 represents the MIC value for the conjugated polyamines in each microorganism in relation to its ClogD. Again, the core polyamine structure provides a better explanation for the activity against bacteria and yeast than their lipophilia. For instance, 5a had a ClogD value between 1a and 2a but showed greater antimicrobial activity than both. Moreover, the behaviour of 4a and 5a, as well as the pure polyamine 5b (except for S. aureus), was similar despite the differences in lipophilia. In summary, the presence of a lipophilic component in the drug seems necessary to guarantee the accessibility to the membrane of the microorganisms, but once this is achieved, the most important factor that determines its activity is the topology of the polyamine.

2.3.2. Determination of the Minimal Microbicidal (Bactericidal/Fungicidal) Concentration (MBC or MFC)

The determination of MBC/MFC was carried out for those compounds with superior antimicrobial activity. The results revealed that those displaying antibacterial activity were bactericides for both E. coli and S. aureus strains (the MBC values are indicated in Table 3). In the case of S cerevisiae, compounds 4a, 5a, and 5b were found to be fungistatic: Growth was observed after inoculation on SC-ura plates of an aliquot of a sample resulting from the overnight incubation of yeast cells with each one of these compounds at a concentration of four times the MIC value. The representative images of these results are shown in Figure S6 in the Supplementary Materials.

2.3.3. Determination of the Synergies between Compounds and Control Antifungal and Antibacterial Substances Using the Checkerboard Titration Approach

The synergy effect among different drugs becomes evident when the overall therapeutic action of their combination is greater than the sum of effects caused by each individual component [39]. Synergistic combinations facilitate an increase in beneficial results because the use of lower doses of each constituent can reduce the side effects and toxicity associated with high quantities of individual drugs. Combination therapies are widely used for the treatment of the most severe diseases, such as cancer or AIDS [40] (see also the references therein).
To determine the possibility of synergy between the lead compounds and the commercial antimicrobials essayed, each one was tested using the checkerboard titration method [41,42]. For the interpretation of the results, the criteria of Loewe’s additive theory were followed, and for this purpose, the fractional inhibitory concentration index (FICI) was calculated, as described in the Materials and Methods section. In the case of bacteria, the experiments were conducted between each active polyamine and every one of the commercial antibacterial drugs indicated in Table 1; we only found synergy between 5b and ciprofloxacin in E. coli. Conversely, for yeast strains, positive results were found between compounds 4a and 5a and the known antifungal agent amphotericin B, as well as between 4a, 5a, and 5b and cycloheximide. Additionally, in the BY4741 transformed with the YEplac195 control plasmid, 4a, 5a, and 5b were found to be synergic with fluconazole (Table 4). Figure 4 shows the representative images of the results obtained after growth in the plate of aliquots corresponding to the most meaningful tubes prepared for the checkerboard titration approach.

2.4. Compound Cytotoxicity on Human Cells

Table 5 and Figure S7 in Supplementary Materials show the results of the viability assay carried out to determine the cytotoxicity of the conjugated compounds 1a–5a and the pure polyamine 5b on the human Jurkat cell line. As can be seen in Table 5, the most polar one, compound 5b (ClogD −5.36), showed the lowest cytotoxicity (IC50 1252 μg/mL), while the most lipophilic one, compound 3a (ClogD −1.15), was clearly the most cytotoxic (IC50 1.86 μg/mL). The remaining compounds showed intermediate cytotoxicity, with two different ranges of values, one for linear compounds 1a and 2a and the second one for compounds 4a and 5a. Figure 5 shows the IC50 values (black column) for each compound, together with the corresponding MIC values for the microorganisms considered (light blue, dark blue, and grey columns). Considering all these data together, macrocyclic polyamine 5b is the one that showed the highest therapeutic index in all cases. The conjugated polyamines 4a and 5a also presented acceptable values in E. coli, in contrast to the other compounds (1a, 2a, and 3a), which were found to be very toxic to human cells.

2.5. Antimicrobial Potential of Other Derived Compounds from Polyamine 5b

Although the benzodioxole fragment is a component of some drugs, its inhibitory effect on the activity of CYP (cytochrome P450)-dependent enzymes has been described in mammals and other species [43] (see also the references therein). For this reason, and in order to find the active compounds in which toxicity could be lower than in the conjugated polyamines described here thus far, we extended the study to three other polyamines based in the macrocyclic scaffold conjugated with other groups different from benzodioxole but with similar physicochemical characteristics and properties. Figure 6 shows the structure of these compounds (6a, 7a, and 8a) in which polyamine 5b was condensed, as described in Scheme 1, with 2-hydroxybenzaldehyde, 4-hydroxybenzaldehyde, and 2,3-dihydrobenzofuran-5-carbaldehyde, respectively. The synthesis of compounds 6a and 7a was recently reported by some of us [44], whereas compound 8a is reported here for the first time.
As with the other compounds, the acid-base behaviour of these new derivatives was studied via potentiometric titrations in water. As for 5a and 5b, the protonation of the central tertiary nitrogen atoms and the pyridine ones was not detected. The percentage of species and the average number of positive charges, n, at pH 7.4 were calculated (Table 6).
The susceptibility of the microorganisms to these compounds was measured by determining the minimum inhibitory concentration (MIC) and the minimum microbicidal concentration (MMC) (Table 7 and Table 8). To assess whether the antimicrobial activity of the tested compounds was relevant, it was compared with the value determined previously for 5a and 5b. It could be observed that 6a exhibited the highest antimicrobial activity for yeast and E. coli. In the case of S. aureus, it was similar to that for 5a. On the other hand, 7a and 8a yielded results like those of 5a and 5b only in the case of E. coli and better than 5b in S. aureus.
Next, we investigated possible interactions with commercial antimicrobials using the checkerboard assay. The results of these experiments, displayed in Table 9, showed no synergy in the case of bacteria with 6a, but positive results were found with 7a and gentamicin, as well as with 8a and ampicillin, doxycycline, and gentamicin in E. coli. In the case of yeast strains, 6a yielded positive results with cycloheximide and amphotericin B. Experiments were not carried out in those cases in which the MIC values were very high.
These results were confirmed by plating samples corresponding to the incubation of the microorganisms with concentrations corresponding to half of the MIC of every one of the antimicrobials and with a mixture of one-quarter of the MIC of both.
To understand the level of safety in human cells, the cytotoxicity of polyamines 6a, 7a, and 8a was determined using the Jurkat cell line of human lymphocytic leukaemia (ATCC TIB-152). The data obtained are shown in Table 10 and Figure 7, as well as Figure S7 in the Supplementary Materials.
As observed, 6a and 8a, and especially 7a, were found to be less toxic than 5a. This demonstrates that the substitution of the benzodioxole group by other aromatic groups with similar physicochemical properties (e.g., size and lipophilicity) has a significant and positive impact. This fact may be attributed to the inhibitory effect of 1,3-benzodioxole on CYP-dependent enzymes, as mentioned above and demonstrated with other drugs, although further experiments are necessary to confirm this [28].
In all cases, and particularly against the bacterium E. coli, the increase in the therapeutic index points to the potential utility of all these compounds. It is important to note that although 5b and 7a may appear to be less suitable based on their higher MIC values, when considering the whole data, they appear to be very promising candidates.

2.6. Intracellular ATP Concentrations and Microbiolytic Activity

To gain further insight into the effect of the compounds described in this work that have relevant antimicrobial activity and contain the same polyamine scaffold, we carried out two additional experiments with compounds 5a and 6a: one for the determination of the intracellular ATP values and the other for the analysis of their capacity to induce cell lysis.

2.6.1. Analysis of the Intracellular ATP Concentration in Cells Treated with the Most Active Compounds Considered in This Work

Lehtinen et al. [45] described the use of bioluminescence-based techniques for measuring bacterial viability. Since ATP can be produced only in catabolically active cells, in the absence of external ATP, bioluminescence generated in an ATP-dependent reaction provides information about cell metabolic conditions.
Following the procedure described in the Materials and Methods section, luciferase activity was used to determine the intracellular ATP concentration in the bacterial and yeast cells treated with polyamines 5a and 6a. Studies were carried out in parallel with other compounds with antimicrobial activity (ampicillin and doxycycline in bacterial strains; fluconazole, amphotericin B, and SDS in the case of yeasts).
According to the results shown in Figure 8, in yeast cells treated with a concentration 50-fold the MIC value of amphotericin B, a dramatic decrease in ATP intracellular levels was observed after overnight treatment. Under the same conditions, treatment with 5a and 6a resulted in higher ATP levels, which were similar to the ones measured in the presence of SDS at a concentration of 0.1% (w/v). In these cases, ATP amounts were reduced to approximately 50–70% relative to untreated cells. The effect of fluconazole in the depletion of nucleotide intracellular levels was very reduced, although it is worth mentioning that a concentration 30-fold the MIC value was used due to its lower solubility in aqueous solutions.
Regarding E. coli cells, the effect of all the compounds at five-fold MIC concentrations was a reduction in the ATP intracellular levels to 40% or less. This decrease was especially relevant in the case of the treatments with ampicillin and 5a, followed by doxycycline and 6a. For S. aureus, similar results were obtained, although in this case, 6a displayed a higher effect than 5a and doxycycline. These results confirm the important effect of 5a and 6a on cell metabolic activity in bacterial cells.

2.6.2. Determination of the Microbiolytic Activity of the Microbicidal Compounds Considered in This Work Using Time-Kill Kinetics

Although the precise mechanism of action of antibacterial polyamines has not been fully elucidated, the similarity found between the structural requirements for them and the known antimicrobial peptides (AMPs) seems to indicate that both kinds of compounds share the same pharmacophore model (the presence of several positive charges and hydrophobic fragments) [46]. This suggests that, at least in bacteria, both could have a similar mechanism of action, in which the negatively charged bacterial membrane is the primary target, and the electrostatic interaction between this membrane and the positively charged polyamine backbone is the major driving force that finally leads to the disruption of membrane integrity [15,16].
The experiments carried out with the studied polyamines revealed bactericidal behaviour for most of them (Table 3 and Table 8). In order to determine if these compounds were capable of inducing cell lysis in bacteria, time-kill assays were performed, following the procedure described in the Materials and Methods section. For these experiments, compounds 5a and 6a were used again. Cell growth was followed by the OD600 measurement in the absence and presence of polyamines of interest and also using control agents with known lytic effects (ampicillin) [47] and non-lytic properties (doxycycline) [48] (see also references therein) (Figure 9).
In the case of E. coli, when cells were treated with ampicillin, and in accordance with its lytic activity, growth was not observed over time; in fact, OD600 significantly decreased as incubation time increased. The obtained results for 5a and 6a demonstrate that they do not have a lytic effect on this bacterium and behave similarly to doxycycline. Regarding S. aureus, the ampicillin treatment results were also obtained for cellular lysis, which was not the case for doxycycline and the polyamines considered in this study. However, with the methodology used in these experiments, some degree of effect on membrane integrity cannot be completely ruled out.
Experiments were also carried out with yeast cells and, as expected considering its fungistatic character, the results demonstrate that these compounds do not induce lysis, despite what occurred with amphotericin B.

3. Materials and Methods

3.1. Synthesis

All reagents and chemicals were obtained from commercial sources and were used as received. The solvents employed for the chemical synthesis were of analytical grade and were utilised without further purification. Polyamines 1b–3b were commercially purchased, whereas 4b, 5b, 6a, and 7a were prepared following procedures previously described [24,32,33,34,44]. All compounds were characterised via 1H and 13C NMR spectroscopy and elemental analysis.
For the synthesis of conjugated polyamines 1a–8a, the corresponding polyamine (between 0.5 and 1 g) was first dissolved in 30–60 mL of methanol and placed in a 250 mL round flask with magnetic stirring. The number of equivalents of each aldehyde (2H-1,3-benzodioxole-5-carbaldehyde, 2-hydroxybenzaldehyde, 4-hydroxybenzaldehyde, or 2,3-dihydrobenzofuran-5-carbaldehyde) corresponding to the number of primary amines was dissolved in another 30 mL of methanol and added dropwise to the reaction flask. The temperature was then slowly increased to 50 °C and maintained under magnetic stirring for 24 h. After this time, it was lowered to 0 °C, and an excess of NaBH4 was slowly added (8 equivalents × No. of imines). The solution was continuously stirred until it reached room temperature, and then the solvent was eliminated. The crude product of the reaction was dissolved in 100 mL of water and extracted four times with 25 mL of dichloromethane. The product was recrystallised by adding an excess of HCl 4 M in dioxane, centrifuged, and dried under vacuum (60–90% yields).
N1-(benzo[d][1,3]dioxol-5-ylmethyl)-N4-(3-((benzo[d][1,3]dioxol-5-ylmethyl)amino)propyl)butane-1,4-diamine (1a). 1H RMN (D2O, 300 MHz): δH 6.88 (m, 3H); 5.91 (s, 6H); 4.09 (s, 6H); 3.05 (m, J = 5, 6H); 2,03 (m, 6H); 1.68 (m, 6H). 13C RMN (D2O, 75 MHz): δC 148.8, 148.1, 124.2, 109.9, 108.9, 101.6, 51.0, 46.9, 45.5, 44.1, 43.1, 22.1. Anal. Calc. for C23H34N3O4Cl3: C, 52.8; H, 6.6; N, 8.0; O, 12.2; Cl, 20.4. Exp.: C, 51.9; H, 6.3; N, 7.2; O, 12.6; Cl, 22.0.
N1,N1′-(butane-1,4-diyl)bis(N3-(benzo[d][1,3]dioxol-5-ylmethyl)propane-1,3-diamine) (2a). 1H RMN (D2O, 300 MHz): δH 6.88 (m, 3H); 5.92 (s, 6H); 4.11 (s, 6H); 3.06 (m, 6H); 2,03 (m, 6H); 1.70 (m, 6H). 13C RMN (D2O, 75 MHz): δC 148.3, 147.7, 124.2, 123.9, 118.1, 109.9, 108.9, 101.6, 51.1, 47.0, 44.4, 43.6, 22.7. Anal. Calc. para C26H42N4O4Cl4·H2O: C, 49.9; H, 6.9; N, 9.0; O, 11.5; Cl, 22.7. Exp.: C, 50.0; H, 6.7; N, 8.3; O, 11.1; Cl, 23.9.
N1-(benzo[d][1,3]dioxol-5-ylmethyl)-N2,N2-bis(2-((benzo[d][1,3]dioxol-5-ylmethyl)amino)ethyl)ethane-1,2-diamine (3a) 1H RMN (D2O, 300 MHz): δH 6.86 (m,10H); 5.92 (s, 6H); 4.06 (s, 6H); 3.04 (m, J = 6, 6H); 2.86 (t, J = 6, 5H). 13C RMN (D2O, 75 MHz): δC 148.2, 147.7, 124.3, 123.9, 109.5, 109.1, 101.6, 51.0, 49.1, 44.7, 44.5, 43.8, 22.4. Anal. Calc. for C30H39N4O6Cl3(H2O): C, 53.3; H, 6.11; N, 8.29. Exp.: C, 53.0; H, 8.7; N, 8.1.
N1-(benzo[d][1,3]dioxol-5-ylmethyl)-N3-(2-((2-((3-((benzo[d][1,3]dioxol-5-ylmethyl)amino)propyl)amino)ethyl)(2-((3-(((2,3-dihydrobenzofuran-6-yl)methyl)amino)propyl)amino)ethyl)amino)ethyl)propane-1,3-diamine (4a). 1H RMN (D2O, 300 MHz): δH 6.86 (m,10H); 5.87 (s, 6H); 4.07 (s, 6H); 3.1 (m, J = 6, 16H); 2.79 (t, J = 6, 5H); 2.11 (m, 6H). 13C RMN (D2O, 75 MHz): δC 148.2, 147.7, 124.3, 123.9, 109.5, 109.1, 101.6, 51.0, 49.1, 44.7, 44.5, 43.8, 22.4. Anal. Calc. for C39H63N7O6Cl6(H2O): C, 49.90; H, 6.77; N, 10.45; O, 10.23. Exp.: C, 48.74; H, 6.63; N, 9.67; O, 11.73.
2-(3,6,9-triaza-1(2,6)-pyridinacyclodecaphane-6-yl)-N-(benzo[d][1,3]dioxol-5-ylmethyl)ethan-1-amine (5a). 1H NMR (D2O, 300 MHz): δH 7.97 (t, J = 7.80, 1H); 7.46 (d, J = 7.80, 2H); 6.99 (m, 3H); 6.03 (s, 2H); 4.64 (s, 4H); 4.21 (s, 2H); 3.28 (m, 6H); 3.06 (t, J = 5.3, 2H); 2.92 (t, J = 5.3, 4H). 13C NMR (D2O, 75 MHz): δC 148.96, 148.20, 147.68, 139.62, 124.42, 124.00, 122.02, 110.11, 106.91, 101.51, 51.12, 50.93, 50.43, 49.51, 45.84, 42.21. Anal. Calc. for C21H32N5O2Cl3(H2O): C, 49.37; H, 6.71; N, 13.71; O, 9.39. Exp.: C, 47.87; H, 6.33; N, 11.96; O, 9.60.
2-(3,6,9-triaza-1(2,6)-pyridinacyclodecaphane-6-yl)-N-((2,3-dihydrobenzofuran-5-yl)methyl)ethan-1-amine (8a). 1H NMR (D2O, 300 MHz): δH 7.89 (t, J = 7.80, 1H); 7.37 (d, J = 7.80, 2H); 7.30 (s, 1H); 7.18 (dd, J= 8.3, 1H); 6.79 (d, J = 8.3, 1H); 4.56 (m, 5H); 4.14 (s, 2H); 3.17 (m, 6H); 2.97 (m, 2H); 2.84 (t, J = 5.3, 4H). 13C NMR (D2O, 75 MHz): δC 160.06, 148.84, 139.73, 130.19, 128.96, 127.04, 122.77, 122.14, 109.51, 72.10, 66.53, 51.28, 50.85, 50.44, 49.42, 45.85, 42.07. Anal. Calc. for C22H34N5OCl3(H2O)2: C, 50.14; H, 7.27; N, 13.29; O, 9.11. Exp.: C, 49.69; H, 6.61; N, 12.58; O, 8.19.

3.2. Potentiometric Titrations

The potentiometric titrations were carried out at 298.1 ± 0.1 K using NaCl 0.15 M as a supporting electrolyte. The experimental procedure (burette, potentiometer, cell, stirrer, microcomputer, etc.) has been fully described elsewhere [49]. The acquisition of the EMF data was performed with the computer program PASAT [50]. The reference electrode was a Ag/AgCl electrode in a saturated KCl solution. The glass electrode was calibrated as a hydrogen-ion concentration probe via the titration of previously standardised amounts of HCl with CO2-free NaOH solutions and the equivalent point determined using the Gran method [51,52], which provides the standard potential, Eθ′, and the ionic product of water (pKw = 13.73(1)).
The computer program HYPERQUAD was used to calculate the protonation constants [53]. The pH range investigated was 2.5–11.0, and the concentration of the ligands ranged from 5 × 10−4 to 5 × 10−3 mol/dm. The different titration curves for each system (at least two) were treated either as a single set or as separated curves without significant variations in the values of the stability constants. Finally, the sets of data were merged and treated simultaneously to give the final stability constants.

3.3. Antimicrobial Activity

3.3.1. Bacterial and Yeast Strains and Growth Conditions

The microorganisms used for the susceptibility tests were the bacteria Escherichia coli JM101 and Staphylococcus aureus BHI, and the yeast Saccharomyces cerevisiae strains BY4741 (MAT a his3Δ1 leu2Δ0 met15Δ0 ura3Δ0 (EUROSCARF)) carrying YEplac195 (from EUROSCARF) or YEPlac195-PDR5 (provided by Ayse Banu Demir, Izmir University of Economics, Turkey) plasmids.
Bacterial strains were usually maintained and grown in an LB medium (0.5% (w/v) yeast extract, 1% (w/v) bactotryptone, and 1% (w/v) NaCl) at 37 °C. For MIC (minimal inhibitory concentration) and MMC (minimal microbicidal concentration) assays, and for the determination of synergies, overnight growth was carried out in 2% (w/v) bactopeptone (BP), and then the cultures were diluted and incubated for several hours in 2% (w/v) BP for ensuring logarithmic growth. Yeast strains were grown in an SC-ura medium (0.17% (w/v) yeast nitrogen base without amino acids and ammonium sulphate, 0.2% (w/v) drop-out without uracil, 0.5% (w/v) (NH4)2SO4, and 2% (w/v) glucose) at 30 °C. Liquid cultures were incubated with shaking (200 rpm). Solid media also contained 2% (w/v) agar.

3.3.2. Preparation of Stock Solutions of Test and Control Compounds

The control drugs used in our experiments were the commercial antibacterial doxycycline, gentamicin, ciprofloxacin, and ampicillin, and the antifungal fluconazole, amphotericin B, and cycloheximide. All of them were purchased from Sigma-Aldrich (Darmstadt, Germany). Stock solutions of these drugs and the compounds to be tested were prepared in phosphate buffer 20 mM pH 7.4.

3.3.3. Determination of the Minimum Inhibitory Concentration (MIC)

For the analysis of the antimicrobial activity, the strategies and indications of Cushnie et al. were considered [54]. The standardised method of microdilution in a culture medium was followed to determine the MIC [55]. In bacterial strains, serial dilutions of the compounds to be tested and the control antibiotics were prepared in phosphate buffer (20 mM, pH 7.4, 0.5 mL) and were mixed with a suspension of bacterial cells in a logarithmic growth phase (in 1% BP, 0.5 mL). The final OD600 of the whole solutions were 0.004 and 0.008 for E. coli and S. aureus cultures, respectively. After 20 h of incubation at 37 °C with shaking, the MIC was determined as the lowest concentration of each compound in which no visible bacterial growth was observed.
The determination of the MIC for yeast strains was carried out following a similar procedure to that of the polyamines and antifungal reference agents: Serial dilutions of each one in phosphate buffer (20 mM, pH 7.4, 0.5 mL) were prepared and mixed with a suspension of yeast cells (OD600 0.04 in SC-ura 2X (VWR, Atlanta, GA, USA), 0.5 mL). After 24 h of incubation at 30 °C with shaking, the MIC was determined as the lowest concentration of each compound that resulted in the same optical density of the solution as that observed prior to the incubation. Experiments were carried out at least three times in all cases.

3.3.4. Determination of the Minimum Microbicidal Concentration (MMC)

Once the MIC was known, the samples were prepared as described in the previous section with polyamine concentrations corresponding to the MIC and half, double, and four times its value. After overnight incubation with the microorganisms, 30 μL of a ten-fold dilution of each one was spread in LB (in the case of bacterial strains) or SC-ura (for yeast strains) plates. They were incubated for 20 h at 37 °C (bacteria) or 48 h at 30 °C (yeasts), and the level of growth was determined. Since the microbiostatic activity has been defined as an MMC-to-MIC ratio of >4 [56], we classified compounds as microbiostatic if growth was observed in the plates from samples containing 4 times the MIC concentration, and in microbicides, those in which no growth was detected at this concentration were considered microbiostatic. In the case of microbicidal substances, the minimal fungicidal/bactericidal concentration (MFC/MBC) was determined as the lowest concentration of the tested agent that either completely prevented growth or resulted in a >99.9% decrease in the inoculum. Experiments were carried out at least three times.

3.3.5. Determination of the Synergies between the Polyamines and Control Antifungal and Antibacterial Substances Using the Checkerboard Titration Approach

The combined antimicrobial activity of the test compounds with the antibacterial or antifungal control agents was performed under the same conditions used for the MIC determination and following the procedures described by Carton Herrán [57], Reis de Sá et al. [58] and Zharkova et al. [55]. For each experiment, 16 samples (4 rows × 4 columns) in a total volume of 0.5 mL were prepared in tubes using an array of combinations between the MIC value and 0 μg/mL of the compound to be tested in each row, and between the MIC value and 0 μg/mL of the reference drug in each column. In this way, a variety of mixtures with different concentrations of them alone or in combination was obtained. Briefly, 0.5 mL of a microorganism culture was added to each one of the samples, and after incubation for 24 h with shaking at the appropriate temperature (37 °C or 30 °C), the tubs were visually inspected, and the OD600 was measured. From this information, the fractional inhibitory concentration index (FICI) was calculated according to the formula FIC index = ([A]/[CMI A]) + ([B]/[CMI B]), where [A] and [B] are respective concentrations of tested polyamine and reference drug in their combination effectively inhibiting the growth of bacteria or yeast, and [MIC A] and [MIC B] are the individual MICs of the tested polyamine and reference drug when they are used alone. An interaction is considered synergistic when the FICI value is ≤0.5 [41,42].
To confirm the data obtained in the checkerboard assay, 30 μL of a ten-fold dilution of the tubes containing concentrations of half of the MIC of each one of the compounds alone (polyamine to be tested and reference drug) and one fourth of the MIC of each one in combination were also spread in LB or SC-ura plates (according to the microorganism considered in each case) and incubated at 37 °C or 30 °C. The visualisation of these plates was performed after 24 or 48 h, respectively. All these experiments were carried out in triplicate.

3.3.6. Analysis of the Intracellular ATP Concentration in Bacterial and Yeast Cultures Treated with the Tested Compounds

The procedure described by Lehtinen et al. was followed [45], with the modifications indicated herein. In the case of bacteria, 1.5 OD600 units were incubated overnight in 1 mL of final volume with 5-fold MIC concentrations. Then, the cells were collected, washed 3 times in 20 mM phosphate buffer pH 7.4, and lysed in 200 μL of LS1 (50 mM of glucose, 25 mM of Tris-HCl pH 8.0, and 10 mM of EDTA pH 8.0) containing 5 mg/mL of lysozyme and the same volume of glass beads (425–600 μm), by stirring 10 times for 15 s each. Then, the solution was centrifuged at 14,800× g for 15 min, and the supernatant was used for a luciferase assay. For this purpose, in each well of a microtiter plate, 100 μL of luciferase assay buffer (0.015 M of MgSO4, 0.015 M of KH2PO4 pH 8, 0.004 M of EGTA pH 8, and 2 mM of DTT) was added together to a 50 μL of 0.3 mg/mL luciferin solution in 0.01% (w/v) Triton X-100 and 50 μL of the cell extract. Finally, 15 μL of a 67 μg/mL aqueous solution of luciferase was added. Light emission was immediately detected using a Luminoskan Ascent instrument (Thermo Scientific, Waltham, MA, USA) for 1 s per well. Glass beads, lysozyme, luciferin, and luciferase were purchased from Sigma-Aldrich.
In the case of yeasts, 50 OD600 units were incubated overnight in 1 mL of final volume with 50-fold MIC concentrations. Then, cells were collected and washed as above and resuspended in 500 μL of LS2 (140 mM of NaCl, 1.5 mM of MgCl2, 10 mM of Tris-HCl pH 8.0, and 0.5% (v/v) NP40). Cells were lysed in the presence of 1 volume of glass beads as described above. The next steps were carried out as in the case of bacterial samples.
Experiments were carried out at least in triplicate in all cases, and control drugs and SDS (0.1% (w/v) of the final concentration) were also included.

3.3.7. Analysis of the Lytic Activity of Microbicidal Compounds

To determine if the compounds showing microbicidal activity induce cell lysis, the procedure described by Fleeman et al. was followed [59], with the modifications indicated below. The E. coli and S. aureus strains were grown as in the experiments described earlier. The cells corresponding to 1.5 units of OD600 were collected and resuspended in 1% BP after washing in the same medium. They were incubated in a final volume of 1 mL with concentrations 5 times higher than the MIC of the analysed compounds, and OD600 was monitored over time. Other antimicrobial compounds were also used in this study as controls. The experiments were performed in triplicate.

3.4. Determination of Compound Cytotoxicity on Human Cells

The cytotoxicity of the compounds was assessed via flow cytometry with a viability assay using propidium iodide (PI), a DNA-binding fluorescent probe not permeant to live cells, which is commonly used to detect dead cells in a population [60]. The human lymphocytic leukaemia Jurkat cell line (ATCC TIB-152) was obtained from the American Type Cell Culture (Sigma-Aldrich) and grown in suspension in an RPMI 1640 medium (Thermo Fisher Scientific, Waltham, MA, USA) supplemented with L-glutamine, antibiotics, and 10% heat-inactivated foetal calf serum (FCS, Thermo Fisher Scientific, Waltham, MA, USA). For the viability assay, cells were seeded in plastic 96-well plates at 250,000 cells/μL in an RPMI 1640 medium supplemented with 5% FCS. The cells were treated for 24 h with a range of concentrations of the test compounds or with the same volume of phosphate buffer (PBS) in control wells. After incubation, cell suspensions were washed, resuspended in 400 μL fresh medium, and incubated for 5 min at room temperature in the dark with 3.75 μM PI (Sigma-Aldrich). Cell viability was determined via flow cytometry using a Gallios flow cytometer (Beckman Coulter). PI fluorescence was excited with an argon-ion laser at 488 nm and collected through a 620/630 nm band-pass emission. Cellular events were discriminated from debris using forward scatter (FS) and side scatter (SS) signals. Cell aggregates were excluded from analysis based on FS-integral and FS-peak. The gates applied for population discrimination were set manually based on control samples. For each sample, 10,000 events were collected. For further analysis, the cytometric data were exported to Kaluza 2.1 software (Beckman Coulter, Brea, CA, USA). Dead cells were identified and quantified as PI-positive events. The cytotoxic potency of test compounds was quantified using their IC50 values, i.e., the compound concentration at which cell viability is inhibited by 50%, as calculated via curve fitting and determined with the correlation coefficient (R2) using GraphPad Prism 9.0 software. Experiments were carried out in triplicate.

4. Conclusions

In this work, we describe a collection of new compounds based on different polyamine scaffolds functionalised with different oxygen-containing aromatic groups that are easily synthesised and display antibacterial/antifungal activity. As an overall conclusion, it was demonstrated that the addition of a lipophilic moiety to the polyamine backbone enhances the efficacy of the resulting compounds. Structural characteristics such as total charge and the polyamine topology seem to be determinative in the antimicrobial activity. Moreover, these substances are interesting antifungal agents in combination with other known drugs, such as cycloheximide and amphotericin. Macrocyclic polyamine 5b, its derivatives 5a and 6a, and tripodal compound 4a were found to be the most effective antimicrobials. However, the nature of the lipophilic component was determinative in the toxicity of these derivatives on human cells, and in this context, polyamines 5b and 7a also proved promising as alternatives to lead due to their low harmfulness. It would be interesting to advance the research of similar compounds, designed through the rational modification of their structure that could be more selective and effective. Further analyses using computational, biochemical, and microscopy-based methods would also be required to understand their mechanism of action on cells.

Supplementary Materials

The following supporting information can be downloaded at: https://www.mdpi.com/article/10.3390/molecules28227678/s1, Figure S1: 1H NMR spectra of the new compounds; Figure S2: 13C NMR spectra of the new compounds; Figure S3: ATR-IR spectra of all the new compounds; Figure S4: Scheme and X-ray crystallographic structure of 3a·3HCl; Table S1: Crystal data, data collection parameters, and results of the analysis; Figure S5: Molar fraction species distribution diagrams; Figure S6: Determination of the minimal microbicidal concentration; Figure S7: Cytotoxicity determination using FACS.

Author Contributions

Conceptualisation, M.I., E.G.-E. and C.A.; preparation of the compounds to be analysed, M.I. and A.M.S.; development of most experimental work, N.T.H., A.M.S. and G.T.J.; X-ray analyses, S.B.; experimental design, supervision, and review, M.I., C.A. and M.l.d.O.; flow cytometry experiments, B.J. and J.-E.O.; manuscript writing, M.I., C.A. and M.l.d.O.; funding acquisition, E.G.-E. All authors have read and agreed to the published version of the manuscript.

Funding

This work was supported by the Conselleria de Innovación, Universidades, Ciencia y Sociedad Digital, Generalitat Valenciana (PROMETEO Grant CIPROM/2021/030), Spanish MICINN and MEC and FEDER funds (grants PID2019-110751RB-I00, Universitat de València (grants UV-INV-AE19-1199043 and UV-INV-AE-1560151), Red de Excelencia de Química Supramolecular (RED2018-102331-T) and Unidad de Excelencia María de Maeztu (CEX2019-000919). Mario Inclán thanks Generalitat Valenciana and the European Social Fund for the financial support (APOSTD2019).

Informed Consent Statement

Not applicable.

Data Availability Statement

The data presented in this study are available upon request from the corresponding authors.

Acknowledgments

We are grateful to Ayse Banu Demir for sending us the YEPlac195-PDR5 plasmid.

Conflicts of Interest

The authors declare no conflict of interest.

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Molecules 28 07678 g001
Figure 1. Structures of the compounds studied in this work.
Figure 1. Structures of the compounds studied in this work.
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Molecules 28 07678 sch001
Scheme 1. Synthetic route of compounds 1a–5a.
Scheme 1. Synthetic route of compounds 1a–5a.
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Molecules 28 07678 g002
Figure 2. Analysis of the relationship between the average MIC values of the compounds considered in this work for the E. coli, S. aureus, and S. cerevisiae strains employed and their whole charge.
Figure 2. Analysis of the relationship between the average MIC values of the compounds considered in this work for the E. coli, S. aureus, and S. cerevisiae strains employed and their whole charge.
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Molecules 28 07678 g003
Figure 3. Analysis of the relationship between the average MIC values of the compounds considered in this work for the E. coli, S. aureus, and S. cerevisiae strains employed, and their ClogD values.
Figure 3. Analysis of the relationship between the average MIC values of the compounds considered in this work for the E. coli, S. aureus, and S. cerevisiae strains employed, and their ClogD values.
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Molecules 28 07678 g004
Figure 4. Sinergy between compounds 4a or 5a, and fluconazole or cycloheximide in the strain BY4741/YEplac195. On the left, a scheme of the plate used for these experiments is shown. In each sector, 30 μL of a ten-fold dilution of each one of the tubes prepared as described in the Materials and Methods section was applied. On the right, a representative image of the resulting growth in the plate is shown: (A) fluconazole and compound 4a; (B) cycloheximide and compound 4a; (C) fluconazole and compound 5a; (D) cycloheximide and compound 5a.
Figure 4. Sinergy between compounds 4a or 5a, and fluconazole or cycloheximide in the strain BY4741/YEplac195. On the left, a scheme of the plate used for these experiments is shown. In each sector, 30 μL of a ten-fold dilution of each one of the tubes prepared as described in the Materials and Methods section was applied. On the right, a representative image of the resulting growth in the plate is shown: (A) fluconazole and compound 4a; (B) cycloheximide and compound 4a; (C) fluconazole and compound 5a; (D) cycloheximide and compound 5a.
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Molecules 28 07678 g005
Figure 5. Analysis of the relationship between the average MIC and IC50 values of the compounds considered in this work, and their ClogD. Extended plots for 4a and 5a are also included to better appreciate the differences.
Figure 5. Analysis of the relationship between the average MIC and IC50 values of the compounds considered in this work, and their ClogD. Extended plots for 4a and 5a are also included to better appreciate the differences.
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Molecules 28 07678 g006
Figure 6. Structures of the conjugated polyamines 6a, 7a [44], and 8a, based on macrocyclic scaffold 5b considered in this work.
Figure 6. Structures of the conjugated polyamines 6a, 7a [44], and 8a, based on macrocyclic scaffold 5b considered in this work.
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Molecules 28 07678 g007
Figure 7. Cytotoxicity in the human Jurkat cell line was evaluated for the compounds described in this section using a propidium iodide viability assay via flow cytometry. The MIC values for each compound in the three tested strains are also shown. Data show the average of three independent experiments.
Figure 7. Cytotoxicity in the human Jurkat cell line was evaluated for the compounds described in this section using a propidium iodide viability assay via flow cytometry. The MIC values for each compound in the three tested strains are also shown. Data show the average of three independent experiments.
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Molecules 28 07678 g008
Figure 8. Determination of the ATP intracellular levels of cells treated with the compounds 5a and 6a for 20 h via bioluminescence. Experiments were carried out as described in the Materials and Methods section. Briefly, 50 OD600 units of yeast cultures and 1.5 OD600 units of bacterial ones were used. Experiments were carried out at least in triplicate and the presented data correspond to the normalisation of each average value to that found in untreated cells; the standard deviation was less than 5% in all cases. U—untreated cells, F—fluconazole, A—amphotericin B, D—doxycycline, and AMP—ampicillin.
Figure 8. Determination of the ATP intracellular levels of cells treated with the compounds 5a and 6a for 20 h via bioluminescence. Experiments were carried out as described in the Materials and Methods section. Briefly, 50 OD600 units of yeast cultures and 1.5 OD600 units of bacterial ones were used. Experiments were carried out at least in triplicate and the presented data correspond to the normalisation of each average value to that found in untreated cells; the standard deviation was less than 5% in all cases. U—untreated cells, F—fluconazole, A—amphotericin B, D—doxycycline, and AMP—ampicillin.
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Molecules 28 07678 g009
Figure 9. Average values obtained from three independent experiments to determine the lytic activity of the polyamines studied in this work. Time-kill analyses were carried out as described in the Materials and Methods section. The values shown are relative to those found at time 0 in the untreated samples, for which a value of 100 was assigned. The standard deviation was less than 5% in all cases.
Figure 9. Average values obtained from three independent experiments to determine the lytic activity of the polyamines studied in this work. Time-kill analyses were carried out as described in the Materials and Methods section. The values shown are relative to those found at time 0 in the untreated samples, for which a value of 100 was assigned. The standard deviation was less than 5% in all cases.
Molecules 28 07678 g009
Table 1. Stepwise and cumulative protonation constants of the 1,3-benzodioxole derivatives (a).
Table 1. Stepwise and cumulative protonation constants of the 1,3-benzodioxole derivatives (a).
Reaction (b)1a2a3a4a5a
L + H ⇄ HL10.433 (2)10.81 (3)9.12 (2)10.95 (1)10.48 (1)
LH + H ⇄ H2L8.964 (2)9.481 (8)8.35 (3)9.63 (1)8.78 (1)
H2L + H ⇄ H3L7.699 (2)8.245 (7)6.93 (3)9.12 (1)7.30 (1)
H3L + H ⇄ H4L 7.41 (1) 8.07 (1)
H4L + H ⇄ H5L 7.48 (1)
H5L + H ⇄ H6L 6.35 (2)
log β (c)27.0935.9424.2951.6026.56
n (d)2.73.42.14.52.4
(a) Logarithms of the stepwise (KHjL) and cumulative (β) protonation constants are reported. Values were determined at 298 K in 0.15 mol/dm3 NaCl. Numbers in parentheses are the estimated errors in the last significant figure. (b) Charges are omitted. (c) Calculated as log β = ∑j log KHjL. (d) Average number of positive charges at pH 7.4.
Table 2. MIC values obtained for the control and test compounds in the E. coli, S. aureus, and S. cerevisiae strains considered in this work.
Table 2. MIC values obtained for the control and test compounds in the E. coli, S. aureus, and S. cerevisiae strains considered in this work.
CompoundMIC (µg/mL), Bacteria aMIC (µg/mL), Yeast aClogD b
(pH 7.4)
E. coli JM101S. aureus BHIBY4741/
YEplac195		BY4741/
PDR5
1a50150>400>400−2.53
1b400>400>400>400−7.33
2a1050250250−3.92
2b100400>400>400−8.74
3a2515>400>400−1.15
3b250400>400>400−8.02
4a54150150−4.85
4b400250>400>400−12.72
5a5356060−3.04
5b10200110110−5.36
1,3-Benzodioxole>500>500>500>500+1.6
Fluconazole--1060
Cycloheximide--0.50.5
Amphotericin B--11
Doxycycline10.25--
Ampicillin20.14--
Gentamicin0.020.04--
Ciprofloxacin0.040.1--
a Average values from at least three independent experiments are shown. Standard deviation was lower than 5% of the average value. b Calculator plugins were used for logD calculation, Marvin 22.15.0, 2022, ChemAxon, https//plugins.calculators.cxn.io/logd (accessed on 14 May 2023).
Table 3. Minimal bactericidal or fungicidal concentration (MBC and MFC) of the compounds described in this work.
Table 3. Minimal bactericidal or fungicidal concentration (MBC and MFC) of the compounds described in this work.
CompoundE. coli JM101S. aureus BHIS. cerevisiae Strains
1a100 an.d. bn.d. b
2a20 a100 an.d. b
3a50 a30 an.d. b
4a10 a8 aFungistatic
5a10 a70 aFungistatic
5b20 an.d. bFungistatic
a Values (in µg/mL) correspond to the MBC. These values were confirmed with three independent experiments. b Not determined due to the high MIC values previously described.
Table 4. Synergies between the most active compounds considered in this work and antifungal drugs already described.
Table 4. Synergies between the most active compounds considered in this work and antifungal drugs already described.
BY4741/YEplac1954a5a5b
Fluconazole+++
Cycloheximide+++
Amphotericin B++-
BY4741/PDR5
Fluconazolen.d. an.d. an.d. a
Cycloheximide+++
Amphotericin B++-
a Not determined due to the high MIC values previously described. These results were confirmed with three independent experiments.
Table 5. Cytotoxicity on the human Jurkat cell line of the compounds described in this work, as determined with flow cytometry viability assay with propidium iodide. MIC values for each compound in the strains considered are also shown.
Table 5. Cytotoxicity on the human Jurkat cell line of the compounds described in this work, as determined with flow cytometry viability assay with propidium iodide. MIC values for each compound in the strains considered are also shown.
Compound/ClogDIC50
(μg/mL) a		MIC E. coli
(μg/mL)		MIC S. aureus
(μg/mL)		MIC Yeast
(μg/mL)
1a/−2.5311.4150150>400
2a/−3.928.801050250
3a/−1.151.862515>400
4a/−4.8576.8654150
5a/−3.0437.8453560
5b/−5.36125210200110
a The presented data correspond to the average of three independent experiments, with a standard deviation lower than 5% in all cases.
Table 6. Stepwise and cumulative protonation constants of polyamines 6a, 7a [44] and 8a (a).
Table 6. Stepwise and cumulative protonation constants of polyamines 6a, 7a [44] and 8a (a).
Reaction (b)6a7a8a
L + H ⇄ HL9.93 (1)10.153 (9)9.943 (3)
LH + H ⇄ H2L9.11 (1)9.473 (9)8.736 (3)
H2L + H ⇄ H3L7.92 (1)8.516 (8)7.296 (4)
H3L + H ⇄ H4L6.67 (2)7.341 (9)
log β (c)33.7235.4826.17
n (d)1.912.42.4
(a) Logarithms of the stepwise (KHjL) and cumulative (β) protonation constants are reported. Values were determined at 298 K in 0.15 mol/dm NaCl. Numbers in parentheses are the estimated errors in the last significant figure. (b) Charges are omitted. (c) Calculated as log β = ∑j log KHjL. (d) Average number of positive charges at pH 7.4.
Table 7. MIC values obtained for polyamines derived from 5b in the E. coli, S. aureus, and S. cerevisiae strains considered in this work.
Table 7. MIC values obtained for polyamines derived from 5b in the E. coli, S. aureus, and S. cerevisiae strains considered in this work.
CompoundMIC (µg/mL), Bacteria aMIC (µg/mL), Yeast aClogD b
(pH 7.4)
E. coli JM101S. aureus BHIBY4741/
YEplac195		BY4741/
PDR5
5a5356060−3.04
5b10200110110−5.36
6a2.5404545−3.36
7a13135295295−3.12
8a15100400400−3.01
a Average values from at least three independent experiments are shown. Standard deviation was lower than 5% of the average value. b Calculator Plugins were used for logD calculation, Marvin 22.15.0, 2022, ChemAxon, https//plugins.calculators.cxn.io/logd (accessed on 14 May 2023).
Table 8. Minimal bactericidal or fungicidal concentration (MBC and MFC) of 6a, 7a, and 8a.
Table 8. Minimal bactericidal or fungicidal concentration (MBC and MFC) of 6a, 7a, and 8a.
CompoundE. coli JM101S. aureus BHIS. cerevisiae Strains
6a10 a160 aFungistatic
7aBacteriostatic n.d. bn.d. b
8a60 a400 an.d. b
a Values (in µg/mL) correspond to the MBC. These values were confirmed with three independent experiments. b Not determined due to the high MIC values previously described.
Table 9. Synergies between polyamines based in the macrocyclic scaffold and commercial antimicrobials.
Table 9. Synergies between polyamines based in the macrocyclic scaffold and commercial antimicrobials.
6a7a8a
E. coli
Ampicillin--+
Ciprofloxacin---
Doxycycline--+
Gentamicin-++
S. aureus
Ampicillin-n.d. an.d. a
Ciprofloxacin-n.d. an.d. a
Doxycycline-n.d. an.d. a
Gentamicin-n.d. an.d. a
BY4741/YEplac195
Fluconazole-n.d. an.d. a
Cycloheximide+n.d. an.d. a
Amphotericin+n.d. an.d. a
BY4741/PDR5
Fluconazolen.d. an.d. an.d. a
Cycloheximide+n.d. an.d. a
Amphotericin+n.d. an.d. a
(+) Positive result, (-) Negative result. a Not determined due to the high MIC values previously described. These results were confirmed with three independent experiments.
Table 10. Cytotoxicity on the human Jurkat cell line of the compounds described in this section, as determined via flow cytometry viability assay with propidium iodide. MIC values for each compound in the strains considered are also shown.
Table 10. Cytotoxicity on the human Jurkat cell line of the compounds described in this section, as determined via flow cytometry viability assay with propidium iodide. MIC values for each compound in the strains considered are also shown.
Compound/ClogDIC50
(μg/mL) a		MIC E. coli
(μg/mL)		MIC S. aureus
(μg/mL)		MIC Yeast
(μg/mL)
5a/−3.0437.8453560
5b/−5.36125210200110
6a/−3.3697.952.54045
7a/−3.12950.6113135295
8a/−3.01127.9515100400
a The presented data correspond to the average of three independent experiments, with a standard deviation lower than 5% in all cases.
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Inclán, M.; Torres Hernández, N.; Martínez Serra, A.; Torrijos Jabón, G.; Blasco, S.; Andreu, C.; del Olmo, M.l.; Jávega, B.; O’Connor, J.-E.; García-España, E. Antimicrobial Properties of New Polyamines Conjugated with Oxygen-Containing Aromatic Functional Groups. Molecules 2023, 28, 7678. https://doi.org/10.3390/molecules28227678

AMA Style

Inclán M, Torres Hernández N, Martínez Serra A, Torrijos Jabón G, Blasco S, Andreu C, del Olmo Ml, Jávega B, O’Connor J-E, García-España E. Antimicrobial Properties of New Polyamines Conjugated with Oxygen-Containing Aromatic Functional Groups. Molecules. 2023; 28(22):7678. https://doi.org/10.3390/molecules28227678

Chicago/Turabian Style

Inclán, Mario, Neus Torres Hernández, Alejandro Martínez Serra, Gonzalo Torrijos Jabón, Salvador Blasco, Cecilia Andreu, Marcel lí del Olmo, Beatriz Jávega, José-Enrique O’Connor, and Enrique García-España. 2023. "Antimicrobial Properties of New Polyamines Conjugated with Oxygen-Containing Aromatic Functional Groups" Molecules 28, no. 22: 7678. https://doi.org/10.3390/molecules28227678

APA Style

Inclán, M., Torres Hernández, N., Martínez Serra, A., Torrijos Jabón, G., Blasco, S., Andreu, C., del Olmo, M. l., Jávega, B., O’Connor, J. -E., & García-España, E. (2023). Antimicrobial Properties of New Polyamines Conjugated with Oxygen-Containing Aromatic Functional Groups. Molecules, 28(22), 7678. https://doi.org/10.3390/molecules28227678

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