IMR Press / FBS / Volume 14 / Issue 2 / DOI: 10.31083/j.fbs1402011
Open Access Original Research
Assessment of Antimicrobial Activity of Ethanolic and Aqueous Extracts of Aesculus hippocastanum L. (Horse Chestnut) Bark against Bacteria Isolated from Urine of Patients Diagnosed Positive to Urinary Tract Infections
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1 Department of Microbiology and Virology, Institute of Medicine, RUDN University, 117198 Moscow, Russia
2 Department of Biology and General Genetics, Institute of Medicine, RUDN University, 117198 Moscow, Russia
*Correspondence: (Mbarga M.J. Arsene)
Academic Editor: Jen-Tsung Chen
Front. Biosci. (Schol Ed) 2022 , 14(2), 11;
Submitted: 14 February 2022 | Revised: 14 March 2022 | Accepted: 14 March 2022 | Published: 2 April 2022
(This article belongs to the Special Issue Recent Research on Medicinal Plants)
Copyright: © 2022 The Author(s). Published by IMR Press.
This is an open access article under the CC BY 4.0 license.

The search for new antimicrobials is essential to address the worldwide issue of antibiotic resistance. The present work aimed at assessing the antimicrobial activity of Aesculus hippocastanum L. (horse chestnut) bark against bacteria involved in urinary tract infections (UTIs). Bioactive compounds were extracted from A. hippocastanum bark using water and ethanol as solvents. The extracts were tested against 10 clinical uropathogenic strains including five Gram-positive and five Gram-negative bacteria. Staphylococcus aureus ATCC 6538 and Escherichia coli ATCC 25922 were used as reference bacteria. The susceptibility to antibiotics was assessed using the Kirby Bauer disc diffusion method and the antibacterial activity of the extracts was evaluated using the well diffusion method. The Minimum inhibitory concentration (MIC) and the minimum bactericidal concentrations (MBC) were asseded by the microdilution method. A. hippocastanum bark possessed a dry matter content of 65.73%. The aqueous extract (AE) and ethanolic extract (EE) showed a volume yield of 77.77% and 74.07% (v/v), and a mass yields of 13.4% and 24.3% (w/w) respectively. All the bacteria were susceptible to amoxiclav, imipenem and ceftriaxone but the clinical strains were resistant to at least one antibiotic. Kocuria rizophilia 1542 and Corynebacterium spp 1638 were the most resistant bacteria both with multidrug resistance index of 0.45. Except AE on Proteus Mirabilis 1543 and Enterococcus faecalis 5960 (0 mm), both AE and EE were active against all the microorganisms tested with inhibition diameters (mm) which ranged from 5.5–10.0 for AE and 8.0–14.5 for EE. The MICs of EEs varied from 1–4 mg/mL while those of AEs varied from 4–16 mg/mL. The ethanolic extracts (EE) were overall more active than the aqueous ones. The A. hippocastanum bark extracts had overall weak antibacterial activity (MIC 0.625 mg/mL) and bacteriostatic potential (MBC/MIC 16) on both Gram-positive and Gram-negative bacteria.

Aesculus hippocastanum L.
horse chestnut
urinary tract infections
herbal medicine
1. Introduction

Urinary tract infections (UTIs) are very common infections and occur at least once in a lifetime. These infections are serious public health issues and are responsible for nearly 150 million disease cases every year worldwide [1]. UTIs are defined as any infection, commonly of bacterial origin, which occurs in any part of the urinary system [1]. When UTIs are localized in urethra, they are called urethritis, cystitis (when localized in the bladder), pyelonephritis (infection of the kidneys), and vaginitis (infection of the vagina) [2, 3]. UTIs are more likely to occur in women, because, compared to men, their urethra is shorter and there is relative proximity between the urethra and the anus [4]. In addition, the prevalence of UTIs among sexually active young women has been reported to vary from 0.5 to 0.7 person per year, while this incidence rate among young men was only 0.01 [5]. Otherwise, the so-called uropathogenic bacteria is responsible for 80–90% of UTIs but other germs such as Staphylococcus saprophyticus, Pseudomonas aeruginosa, Staphylococcus aureus, Klebsiella pneumoniae, Proteus mirabilis, Acinetobacter baumannii, Streptococcus, and Enterococcus faecalis are sometimes also involved [6]. The UTIs are easily managed with antibiotics [7] such as trimethoprim-sulfamethoxazole (TMP-SMX), nitrofurantoin, or fosfomycin for 3–5 days [8] and sometimes by cephalosporins (fluoroquinolones; cefixime) and β-lactams (amoxicillin-clavulanate) [9].

However, unfortunately, resistance to antibiotics, which spares no area, has made UTIs more difficult to treat. Several recent studies have reported a considerable increase in antibiotic resistance in uropathogens and an unprecedented number of multidrug-resistant germs worldwide [10, 11]. To respond to this dangerously worrying situation, research teams from all over the world are permanently evaluating the use of potential alternatives to antibiotics such as nanoparticles [12], probiotics [13, 14], phage therapy [15], antimicrobial peptides [16] and medicinal plants [17, 18]. Among these alternatives, medicinal plants seem to offer the most credible evidence [19], considering that plants have been used for millennia in the treatment and prevention of various diseases, including bacterial infections and some of these herbal remedies have proven to be effective in preventing and treating UTIs [19]. In this context, certain plants such as Aesculus hippocastanum which are very widespread (and therefore available) but scarcely utilized deserve to be investigated for their antimicrobial properties.

A. hippocastanum, commonly known as horse chestnut and buckeyes, is a rapidly growing ornamental tree belonging to the family Hippocastanaceae [20]. Trees of this plant are grown up to 30 m in height and 1 m thick with short stem having a rounded crown. A. hippocastanum is highly adapted in polluted environment and is commonly used for the treatment and prevention of many diseases [20]. Its composition rich in esculin (over 17%), fraxin (over 7%) and proanthocyanidins (over 6% of epicatechin and over 5% of procyanidin A2) (Fig. 1, Ref. [21]) gives it anti-inflammatory, vasoprotective, antidiabetic, anti-inflammatory, gastroprotective, neuroprotective, anticancer, hepatoprotective and antibacterial properties [20, 21].

Fig. 1.

Structures of the major constituents of the A. hippocastanum bark [21].

Thus, the aim of this work was to assess the antibacterial properties of ethanolic and aqueous A. hippocastanum bark extract against some bacteria involved in urinary tract infections.

2. Materials and Methods
2.1 Vegetal Material

The plant material used in this study was the bark of Aesculus hippocastanum. The plant was collected in June 2021 near the Medical Institute of the Peoples’ Friendship University of Russia (MG23 + 9H Obroutchevski, Moscow, Russia). After harvest, the plant was taken directly to the laboratory where it was dried at 37 C until the weight was constant. The dry matter content was calculated; the plant was grinded and the powders with particle sizes lower than 1 mm were stored in a sterile airtight container until further use.

2.2 Bacterial Strains

The microorganisms used for the screening of antimicrobial activity consisted of five Gram positive bacteria and 5 Gram negative. The five Gram + were Kocuria rhizophila 1542, Enterococcus avium 1669, Staphylococcus simulans 5882, Corynebacterium spp 1638 and Enterococcus faecalis 5960 while the five Gram—were Proteus mirabilis 1543, Morganella morganii 543, Citrobacter freundi 426, Acynetobacter baumannii 5841 and Achromobacter xylosoxidans 4892. Staphylococcus aureus ATCC 6538 and Escherichia coli ATCC 25922 were used as standard Gram + and Gram - respectively. All strains were provided by the Department of Microbiology and Virology of the Peoples’ Friendship University of Russia.

2.3 Chemicals and Media

Dimethyl sulfoxide (DMSO) was purchased from BDH Laboratories, VWR International Ltd., USA. We also used BHIB (Brain Heart Infusion Broth) (HiMedia™ Laboratories Pvt. Ltd., India), Muller Hinton Agar (MHA HiMedia™ Laboratories Pvt. Ltd., India), Sabouraud Dextrose Broth (SDB, HiMedia™ Laboratories Pvt. Ltd., India) and all other reagents and chemicals used were of analytical grade.

2.4 Extraction of Active Compounds

Ethanolic solution (80%, v/v) and distilled water were used as solvents because they have been reported to be efficient solvents for the extraction of bioactive compounds in the medicinal plants used in this study. As we described in our previous investigation [18] thirty grams (30 g) of vegetal material was weighed and added to 270 mL of the solvent in separate conical flasks. The flasks were covered tightly and were shaken at 200 rpm for 24 h and 25 C in a shaker incubator (Heidolph Inkubator 1000 coupled with Heidolph Unimax 1010, Germany). The mixtures were then filtered by vacuum filtration, using Whatman filter paper № 1 then concentrated at 40 C in rotary evaporator (IKA RV8) equipped with a water bath IKA HB10 (IKA Werke, Staufen, Germany) and a vacuum pumping unit IKA MVP10 (IKA Werke, Staufen, Germany). To avoid losses, the extracts were collected when the volumes were small enough and placed in petri dishes previously weighed and then incubated open at 40 C until complete evaporation. The final dried crude extracts were weighed. Extraction volume and mass yield were determined using the following formulas:

(1) Volume yield ( % ) = Volume of the extract after filtration ( ml ) Initial solvent volume ( ml ) × 100

(2) Mass yield ( % ) = Mass of extracted plant residues ( g ) Mass of plant raw sample ( g ) × 100

2.5 Preparation of Antimicrobial Solution

For each plant extract, the crude extract was dissolved in the required volume of DMSO (5%, v/v) to achieve a concentration of 128 mg/mL. The extracts were sterilized by microfiltration (0.22 μm) and the solution obtained was used to prepare the different concentrations used in the analytical process.

2.6 Inoculum Preparation

Bacteria were cultured for 24 h at 37 C in 10 mL of BHI broth. After incubation, the cells were collected by centrifugation (7000 g, 4 C, 10 min), washed twice with sterile saline, resuspended in 5 mL of sterile saline to achieve a concentration equivalent to McFarland 0.5 using DEN‑1 McFarland Densitometer (Grant‑bio).

2.7 Evaluation of Susceptibility of the Test Bacteria to Antibiotics

The modified Kirby–Bauer’s disk method described in our previous study [22] was used to study the antibiotic sensitivity of the bacterial strains, and the following eight antibiotics disks were used: amoxicillin, 30 μg/disk; ampicillin, 25 μg/disk; cefazolin, 30 μg/disk; cefazolin/clavulanic acid, 30/10 μg/disk; 30 μg/disk; ceftriaxone, 30 μg/disk; ciprofloxacin, 30 μg/disk; Fosfomycin, 200 μg/disk; imipenem (IMP), 10 μg/disk; nitrofurantoin, 200 μg/disk; tetracyclin (TE), 30 μg/disk and trimethoprim, 30 μg/disk. The inhibition diameters were measured and interpreted then referred to the Clinical & Laboratory Standards Institute [23]. Resistance R, Intermediate I, and Sensitive S interpretations were obtained automatically using algorithms written in Excel software [Microsoft Office 2016 MSO version 16.0.13628.20128 (32 bits), USA] with the parameters described in Table 1 [10].

Table 1.Interpretation criteria for antibiotic sensitivity [10].
Antibiotics/limits of inhibition diameters (mm)
Interpretation R d 15 d 14 d 13 d 13 d 13 d 14 d 13 d 13 d 13 d 14 d 12
I 16–20 15–17 14–17 14–20 14–15 15–18 14–17 14–16 14–15 15–17 13–15
S d 21 d 18 d 18 d 21 d 16 d 19 d 18 d 17 d 16 d 18 d 17
AMC, Amoxycillin; AMP, Ampicillin; CZ, Cefazolin; CAC, Cefazolin/clavulanic acid; CAZ, Ceftazidime; CTR, Ceftriaxone; CIP, Ciprofloxacin; FO, Fosfomycin; IMP, Imipenem; NIT, Nitrofurantoin; TE, Tetracyclin; TR, Trimethoprim.
2.8 Screening of Antibacterial Activity
2.8.1 Assessment of Antimicrobial Activity Using Well Diffusion Method

The well diffusion method previously described [18] was used to assess the antimicrobial activity of the extracts. Briefly, 15 mL of sterile Muller Hinton Agar (for bacteria) was poured into petri dishes and 100 μL of each microorganism were spread. Wells with a capacity of 20 μL were drilled on the culture medium and 20 μL (at 128 mg/mL) of each plant material was added. The sterile DMSO 5% used to prepare the extracts was used as a negative control and all the trials were done in triplicate. After incubation at 37 ℃ for 24 h, the inhibition diameters were measured.

2.8.2 Determination of Minimum Inhibitory Concentrations (MIC)

MIC is the lowest concentration of antibacterial agent that completely inhibits the visible bacterial growth. The MIC of the extracts was determined using the microbroth dilution method as previously described without any modification [24]. Briefly, 100 μL of broth (BHIIB) was added to all the wells of sterile U-bottom 96-well microplates and extract preparations (128 mg/mL) were subjected to serial twofold dilution. Each column represented one type of extract and a single strain. DMSO 5% was used as a negative control. For each test well, 10 μL of the respective inoculum was added (with turbidity equivalent to a 0.5 McFarland scale). Finally, the plates were covered and incubated at 37 ℃ for 24 h and after incubation, MIC was considered the lowest concentration of the tested material that inhibited the visible growth of the bacteria.

2.8.3 Determination of Minimum Bactericidal Concentration (MBC)

MBCs were determined by subculturing the wells without visible growth (with concentrations MIC) on MHA plates. Inoculated agar plates were incubated at 37 ℃ for 48 h and MBC was considered the lowest concentration that did not yield any microbial growth on agar.

2.8.4 Tolerance Level

Tolerance level of tested bacterial strains against aqueous and ethanolic extract was determined using the following formula:

Tolerance = MBC/MIC

The characteristic of the antibacterial activity of extracts was determined by the tolerance level indicating the bactericidal or bacteriostatic action against the tested strains. When the ratio of MBC/MIC is 16, the antibacterial efficacy of the test agent is considered as bacteriostatic, whereas MBC/MIC 4 indicates bactericidal activity [25].

3. Results and Discussion
3.1 Dry Matter and Extraction Yield

The dry matter, water content, ethanolic (EE) and distilled water extract (AE) yields of Aesculus hippocastanum bark are presented in Table 2. We found that A. hippocastanum bark possessed a dry matter content of 65.73%. Dry matter is an indicator of the amount of constituents (excluding water) in the sample tested. The drying allowed the removal of water from the plant in order to standardize the extraction and to make this work reproducible if authors from other regions project to work with the same plant. Furthermore, we obtained an extraction volume yield of 74.07% with distilled water as the solvent and 77.77% with ethanol. The difference in extraction volume yields can be explained by losses during the extraction process. Indeed, as reported by [18] we noticed that the filtration of ethanolic extracts was faster (less than 5 minutes for 300 mL) compared to the aqueous extract which took much longer (more than 50 minutes on average for 300 mL) and required in average 6 filter changes. Despite the filtration, the EAs still looked cloudy while the EEs were completely clear. This residue cloudiness could therefore explain the higher mass yield in AE (24.3%) compared to EE (13.4%). Several authors [17, 18, 26, 27] reported observations similar to our findings while others [28, 29] found opposite results. Therefore, as Arsene et al. [18] pointed out in their previous work, the extraction performance depends on several factors, including the method used, extraction time, the solvents, and the equipment used. In addition, Mouafo et al. [17] reported that the high yields of phytoconstituent does not necessarily imply better antimicrobial activity and this was further assessed in the present work by evaluating the antimicrobial activity of each of the extracts using the well diffusion method and the determination of minimum inhibitory concentrations (MIC) and minimum bactericidal concentrations (MBC).

Table 2.Dry matter, water content, volume and mass extraction yield of A. hippocastanum bark.
Aqueous extract Ethanolic extract
Volume yield (%) 74.07 77.77
Mass yield (%) 24.3 13.4
Dry matter of the fresh bark of A. hippocastanum = 65.73% (Water content = 34.27%).
3.2 Susceptiility of the Tested Clinical Strains to Antibiotics

The susceptibility of uropathogenic tests to eleven (11) antibiotics was evaluated by the Kirby Bauer disc method, the Multidrug resistance Index (MDR) was calculated, and the results were reported in Table 3. As shown in Table 3, no bacteria were resistant to amoxiclav, imipenem and ceftriaxone while 7/12 were resistant to ampicillin, 6/12 to trimethoprim, 5/12 to tetracycline and ceftazidime/clavulanic acid, 4/12 to ceftazidime, 3/12 to fosfomycin, 2/12 to nitrofurantoin and 1/12 to ciprofloxacin. Interestingly, both standard bacteria (E. coli ATCC 25922 and S. aureus ATCC 6538) were sensitive to all antibiotics while the clinical strains were resistant to at least one antibiotic. Among clinical strains, MDRs ranged from 0.09 to 0.45. K. rizophilia 1542 and Corynebacterium spp 1638 were the most resistant bacteria with MDRs of 0.45 each. The results observed with these clinical strains are similar to those reported in other studies [10, 11]. While the strongest resistance was observed on ampicillin (which is an antibiotic from the β-lactams family, from the group A of the penicillins), no resistance was observed in amoxiclav which is a derivative of amoxicillin (antibiotic of the beta-lactam family, of the aminopenicillin group) of the same family, with the only difference that the latter is combined with clavulanic acid (β-lactamase inhibitor). This shows that antibiotic adjuvants can also play an important role in combating resistant germs [30]. Furthermore, similarly to our findings, other studies have reported low resistance of uropathogens to imipenem and ceftriaxone [11, 31]. In addition, the sensitivity of all strains to amoxiclav, imipenem and ceftriaxone demonstrates that these 3 antibiotics are effective on a wide range of bacteria, including clinical strains with high resistance to other antibiotics. Therefore, these antibiotics which have kept a good activity against various microorganisms should be carefully used and administered only under prescription and after a prior antibiogram.

Table 3.Susceptibility to antibiotics of the test uropathogenic bacteria.
Gram + K. rizophilia 1542 10 ± 0 (R) 13 ± 0 (R) 22 ± 0 (S) 22 ± 1 (S) 28 ± 2 (S) 10 ± 0 (R) 23 ± 1 (S) 6 ± 0 (R) 30 ± 1 (S) 13 ± 1 (R) 21 ± 2 (S) 0.45
E. avium 1669 21 ± 1 (S) 6 ± 0 (R) 30 ± 4 (S) 25 ± 3 (S) 31 ± 3 (S) 23 ± 1 (S) 27 ± 4 (S) 24 ± 2 (S) 15 ± 0 (R) 6 ± 0(R) 6 ± 0 (R) 0.36
S. simulans 5882 23 ± 1 (S) 20 ± 2 (S) 19 ± 1 (S) 27 ± 3 (S) 38 ± 4 (S) 11 ± 0 (R) 34 ± 3 (S) 11 ± 0 (R) 26 ± 2 (S) 6 ± 0 (R) 20 ± 2 (S) 0.27
Corynebacterium spp 1638 20 ± 0 (S) 32 ± 4 (S) 32 ± 5 (S) 36 ± 2 (S) 14 ± 1 (R) 6 ± 0 (R) 27 ± 2 (S) 6 ± 0 (R) 26 ± 1 (S) 9 ± 0 (R) 10 ± 0 (R) 0.45
E. faecalis 5960 21 ± 1 (S) 11 ± 0 (R) 22 ± 1 (S) 27 ± 1 (S) 31 ± 3 (S) 17 ± 1 (I) 24 ± 2 (S) 6 ± 0 (R) 32 ± 3 (S) 6 ± 0 (R) 6 ± 0 (R) 0.36
S. aureus ATCC 6538 22 ± 1 (S) 32 ± 3 (S) 30 ± 2 (S) 35 ± 4 (S) 38 ± 2 (S) 25 ± 1 (S) 28 ± 3 (S) 25 ± 2 (S) 32 ± 0 (S) 20 ± 1 (S) 31 ± 2 (S) 0.00
Gram - P. mirabilis 1543 19 ± 1 (S) 6 ± 0 (R) 30 ± 4 (S) 25 ± 2 (S) 31 ± 0 (S) 23 ± 2 (S) 27 ± 1 (S) 24 ± 1 (S) 30 ± 2 (S) 16 ± 1 (I) 6 ± 0 (R) 0.18
M. morganii 1543 15 ± 0 (I) 6 ± 0 (R) 33 ± 2 (S) 17 ± 1 (I) 13 ± 0 (R) 23 ± 1 (S) 22 ± 0 (S) 23 ± 1 (S) 22 ± 2 (S) 10 ± 0 (R) 6 ± 0 (R) 0.36
C. freundi 426 21 ± 1 (S) 30 ± 3 (S) 27 ± 2 (S) 35 ± 1 (S) 40 ± 2 (S) 12 ± 0 (R) 37 ± 1 (S) 10 ± 0 (R) 30 ± 2 (S) 6 ± 0 (R) 22 ± 2 (S) 0.27
A. baumannii 5841 26 ± 2(S) 16 ± 0 (I) 27 ± 3 (S) 35 ± 1 (S) 32 ± 3 (S) 19 ± 2 (S) 34 ± 2 (S) 17 ± 1 (I) 30 ± 1 (S) 21 ± 2 (S) 14 ± 0 (R) 0.09
A. xylosoxidans 4892 6 ± 0 (R) 11 ± 0 (R) 23 ± 2 (S) 36 ± 4 (S) 6 ± 0 (R) 16 ± 0 (I) 32 ± 3 (S) 16 ± 1 (I) 20 ± 2 (I) 20 ± 1 (S) 6 ± 0 (R) 0.36
E. coli ATCC 25922 21 ± 3 (S) 30 ± 2 (S) 24 ± 1 (S) 20 ± 1 (S) 40 ± 4 (S) 18 ± 1 (I) 32 ± 2 (S) 16 ± 1 (I) 24 ± 0 (S) 26 ± 0 (S) 24 ± 0 (S) 0.00
AMC, Amoxycillin; AMP, Ampi5cillin; CZ, Cefazolin; CAC, Cefazolin/clavulanic acid; CAZ, Ceftazidime; CTR, Ceftriaxone; CIP, Ciprofloxacin; FO, Fosfomycin; IMP, Imipenem; NIT, Nitrofurantoin; TE, Tetracycline; TR, Trimethoprim; R, Resistant; I, Intermediate; S, Sensitive.
3.3 Inhibition Zone of the Extracts Against the Tested Bacteria

Fig. 2 presents the inhibition diameters of ethanolic (EE) and aqueous (AE) extract of Aesculus hippocastanum bark on the tested microorganisms. Except AE on Proteus Mirabilis 1543 and Enterococcus faecalis 5960 (0 mm), both AE and EE were active on all microorganisms tested with inhibition diameters (mm) which ranged from 5.5–10.0 for AE and 8.0–14.5 for EE.

Fig. 2.

Inhibition diameter of ethanolic and aqueous Aesculus hippocastanum bark extract on tested uropathogenic bacteria.

The ethanolic extracts (EE) were overall more active than the aqueous ones. Consequently, this means that ethanol extracts more compounds with antimicrobial properties compared to water although we found above that the extraction yields with water was higher than that with ethanol. Several authors have reported that compounds with antimicrobial activity such as flavonoids, polyphenols, tannins and alkaloids are generally insoluble in water but soluble in ethanol [32, 33]. Other authors such as Arsene et al. [18], Mouafo et al. [17] and Evbuomwan et al. [34] also pointed out that ethanol extracts more antimicrobial compounds from plant materials as opposed to water. In addition, we found that extracts of A. hippocastanum bark were both active against Gram + bacteria as against Gram - bacteria. To our knowledge, the antibacterial properties of this plant have not yet been investigated but our findings suggest that A. hippocastanum bark has constituents exhibiting a broad-spectrum antimicrobial.

Most of the research conducted on A. hippocastanum focused on its properties to regulate circulatory system imbalances and relieve attacks of hemorrhoids [19]. In a study conducted by Owczarek et al. [19] on the composition of A. hippocastanum bark, it has been reported that this plant presents mainly two groups of compounds: coumarins and proanthocyanidins. Among the coumarins there was mainly esculin (over 17%) and fraxin (over 7%) while among the proanthocyanidins, the authors found epicatechin (over 6%) and procyanidin A2 (over 5%) (Fig. 1) [19]. Owczarek et al. [19] finally concluded that, in total, about 40% of the A. hippocastanum bark extract could be attributed to simple phenolics compounds detectable by LC-PDA. Unfortunately, due to limited ressources we were unable to assess the composition of our extracts in order to compare with the data in the literature. However, we can hypothesize that the antimicrobial properties of A. hippocastanum bark can be attributed to all its components or specifically to esculin [35], to fraxin [36] or proanthocyanidins [37] because these compounds (from other plants) have been reported to have antimicrobial properties. Notwithstanding our findings, further investigations are required to confirm or refute our hypothesis.

3.4 Minimum Inhibitory Concentrations (MIC) and Minimum Bactericidal Concentrations

After evaluating the antibacterial properties of aqueous (AE) and ethanolic (EE) extracts of Aesculus hippocastanum bark against the uropathogens tested using the well diffusion, we investigated the minimal inhibitory concentrations (MIC) and minimal bactericidal concentrations (MBC) of the two extracts. MIC and MBC are two very important elements in the search for new antimicrobials and respectively provide the minimum concentrations required to inhibit or kill the microorganism tested. Table 4 presents the MIC, the MBC, and the MBC/MIC ratio of our 2 extracts on the uropathogens investigated. Similarly to the inhibition diameters, ethanolic extracts (EE) showed the best antimicrobial activity with the lowest MIC and MBC. The MICs of EEs varied from 1–4 mg/mL while those of EAs varied from 4–6 mg/mL. Almost all the MBCs of AEs were indeterminate (>64 mg/mL) while those of EE were successfully determined.

Table 4.Minimum inhibitory concentrations (MIC) and minimum bactericidal concentrations (MBC) of ethanolic and aqueous Aesculus hippocastanum bark extract on tested uropathogenic bacteria.
Aqueous extract Ethanolic extract
(mg/mL) (mg/mL) (mg/mL) (mg/mL)
Gram + K. rizophilia 1542 16 >64 - 4 >64 -
E. avium 1669 4 >64 - 2 64 32
S. simulans 5882 16 >64 - 2 16 8
Corynebacterium spp 1638 64 64 1 4 32 8
E. faecalis 5960 4 64 16 2 64 32
S. aureus ATCC 6538 16 64 4 2 16 8
Gram - P. mirabilis 1543 8 >64 - 2 64 32
M. morganii 1543 2 >64 - 1 64 64
C. freundi 426 16 64 4 2 32 16
A. baumannii 5841 4 >64 - 2 64 32
A. xylosoxidans 4892 4 >64 - 2 64 32
E. coli ATCC 25922 16 >64 - 2 16 8

With water as a solvent, the highest antimicrobial activity was observed against E. faecalis 5960, S. aureus ATCC 6538 and C. freundi 426. Although the MIC and MBC of AE were high against these bacteria, AE was found to be bactericidal against S. aureus ATCC 6538 and C. freundi 426 since the MBC/MIC ratio was 4 for both bacteria. Indeed, Mondal et al. [25] reported that when the ratio MBC/ MIC is 16, the antibacterial efficacy of the test agent is considered as bacteriostatic, whereas MBC/MIC 4 indicates bactericidal activity. Similarly, although the MICs of EEs were relatively low, the MBCs of this extract were quite high, and we concluded that the antibacterial activity was overall bacteriostatic (MBC/ MIC 16) against most bacteria except against some Gram-positive bacteria such as S. simulans 5882, Corynebacterium spp 1638 and S. aureus ATCC 6538. This difference in the activity (although not significant) of EE between Gram positive and Gram negative can be ascribed to the cell wall structure of Gram - bacteria, which differs from the structure of Gram + bacteria with a thin layer of peptidoglycan, the presence of a periplasm, and ease of exchange on the plasma membrane [18]. Furthermore, according to the classification of Kuete [38], the different extracts could be considered as deserving a weak antimicrobial activity independently of the extraction solvent and the tested strain as they scored a MIC value higher than 0.625 mg/mL. Therefore, further studies are needed to evaluate the antibacterial activity of A. hippocastanum bark extracts with other solvents and to assess their synergy with other antibiotics, as the weak antimicrobial activity observed here does not allow us to recommend our plant extracts as such for a possible use in the fight against antibiotic resistance and the management of urinary tract infections.

4. Conclusions

The search for new antimicrobials is essential for overcoming antibiotic resistance in the management of bacterial diseases including urinary tract infections (UTIs). In this study we evaluated the antibacterial properties of aqueous and ethanolic extracts of Aesculus hippocastanum bark against ten (10) clinical uropathogenic bacteria and two (2) standard bacteria. The results showed that, except against few bacteria, the extracts had overall weak antibacterial activity (MIC 0.625 mg/mL) and bacteriostatic potential (MBC/MIC 16) on both Gram positive and Gram-negative bacteria. Therefore, studies with other solvents (such as methanol, aceton or chloroform), other extraction techniques, and synergy tests with conventional antibiotics are needed to conclude on a potential better antimicrobial activity of this plant.


UTI, Urinary tract infection; MIC, Minimum Inhibitory Concentration; MBC, Minimum Bactericidal Concentration; EE, Ethanolic extract; AE, Aqueous Extract; MDR, Multidrug Resistance.

Author Contributions

MMJA & PIV designed the research study. KYK & MMJA performed the research. MMJA analyzed the data. KYK, MMJA, VGE, MVA, MMA, AAA and PIV wrote the manuscript. All authors contributed to editorial changes in the manuscript. All authors read and approved the final manuscript.

Ethics Approval and Consent to Participate

Not applicable.


This study has been supported by the RUDN University strategic Academic Leadership Program.


This research received no external funding.

Conflict of Interest

The authors declare no conflict of interest.

Motse DFK, Ngaba GP, Foko LPK, Ebongue CO, Adiogo DD. Etiologic profile and sensitivity pattern of germs responsible for urinary tract infection among under-five children in Douala, Cameroon: a HospitalBased Study. Avicenna Journal of Clinical Microbiology and Infection. 2019; 6: 49–56.
Ebob Agbortabot Bissong M. Spectrum of Uropathogens and Antimicrobial Susceptibility in Clinically Diagnosed Cases of Urinary Tract Infection in the Bamenda Regional Hospital, Cameroon. American Journal of Health Research. 2017; 5: 19.
Fosso JAM, Njouendou AJ, Ekom SE, Kengne IC. Antibacterial activity of three Cameroonian medicinal plants traditionally used for the treatment of urinary tract infections and their synergistic effects with amoxicillin and serum. Journal of Advances in Medical and Pharmaceutical Sciences. 2017; 15: 1–14.
Walsh C, Collyns T. Pathophysiology of urinary tract infections. Surgery. 2020; 38: 191–196.
Rowe TA, Juthani-Mehta M. Urinary tract infection in older adults. Aging Health. 2013; 9: 519–528.
Arsene MMJ, Viktorovna PI, Davares AKL, Esther N, Nikolaevich SA. Urinary tract infections: Virulence factors, resistance to antibiotics, and management of uropathogenic bacteria with medicinal plants—A review. Journal of Applied Pharmaceutical Science. 2021; 11: 001–012.
Abou Heidar NF, Degheili JA, Yacoubian AA, Khauli RB. Management of urinary tract infection in women: a practical approach for everyday practice. Urology Annals. 2020; 11: 339–346.
Gupta K, Hooton TM, Naber KG, Wullt B, Colgan R, Miller LG, et al. International Clinical Practice Guidelines for the Treatment of Acute Uncomplicated Cystitis and Pyelonephritis in Women: a 2010 Update by the Infectious Diseases Society of America and the European Society for Microbiology and Infectious Diseases. Clinical Infectious Diseases. 2011; 52: e103–e120.
Bader MS, Loeb M, Leto D, Brooks AA. Treatment of urinary tract infections in the era of antimicrobial resistance and new antimicrobial agents. Postgraduate Medicine. 2020; 132: 234–250.
Mbarga MMJ, Andreevna SL, Viktorovna PI. Evaluation of apparent microflora and study of antibiotic resistance of coliforms isolated from the shells of poultry eggs in Moscow-Russia. Journal of Advances in Microbiology. 2020; 20: 70–77.
Suadkia S, Podoprigora IV, Yashina NV, Sarukhanova LE, et Kravtsov EG. Antibiotic-resistant uropathogenic Escherichia coli isolated from children with birth defects of the urinary system. Antibiotics and chemotherapy, 2020; 65: 23–26.
Amer MW, Awwad AM. Green synthesis of copper nanoparticles by Citrus limon fruits extract, characterization and antibacterial activity. Chemistry International. 2021; 7: 1–8.
Joseph AMM, Davares AK, Andreevna SL, Vladimirovich EA, Carime BZ, Marouf R, et al. The use of probiotics in animal feeding for safe production and as potential alternatives to antibiotics. Veterinary World. 2021; 14: 319–328.
Mbarga MJA, Desobgo SCZ, Tatsadjieu LN, Kavhiza N, Kalisa L. Antagonistic effects of raffia sap with probiotics against pathogenic microorganisms. Foods and Raw Materials. 2021; 9: 24–31.
Mireille A, Pascale B, Charlotte B, Laurent D, Nicolas D, Rémy F, et al. Les applications antibactériennes des bactériophages. Virologie. 2020 ; 24: 23–36.
Andersson DI, Hughes D, Kubicek-Sutherland JZ. Mechanisms and consequences of bacterial resistance to antimicrobial peptides. Drug Resistance Updates : Reviews and Commentaries in Antimicrobial and Anticancer Chemotherapy. 2018; 26: 43–57.
Mouafo HT, Tchuenchieu ADK, Nguedjo MW, Edoun FLE, Tchuente BRT, Medoua GN. In vitro antimicrobial activity of Millettia laurentii De Wild and Lophira alata Banks ex C. F. Gaertn on selected foodborne pathogens associated to gastroenteritis. Heliyon. 2021; 7: e06830.
Arsene MMJ, Podoprigora IV, Davares AKL, Razan M, Das MS, Senyagin AN. Antibacterial activity of grapefruit peel extracts and green-synthesized silver nanoparticles. Veterinary World. 2021; 14: 1330–1341.
Wojnicz D, Kucharska AZ, Sokół-Łętowska A, Kicia M, Tichaczek-Goska D. Medicinal plants extracts affect virulence factors expression and biofilm formation by the uropathogenic Escherichia coli. Urological Research. 2013; 40: 683–697.
Idris S, Mishra A, Khushtar M. Phytochemical, ethanomedicinal and pharmacological applications of escin from Aesculus hippocastanum L. towards future medicine. Journal of Basic and Clinical Physiology and Pharmacology. 2020; 31.
Evbuomwan L, Chukwuka EP, Obazenu EI, Ilevbare L. Antibacterial Activity of Vernonia amygdalina Leaf Extracts against Multidrug Resistant Bacterial Isolates. Journal of Applied Sciences and Environmental Management. 2018; 22: 17–21.
Manga MJA, Viktorovna PI, Grigorievna VE, Davares AK, Sergeevna DM, et al. Prolonged exposure to antimicrobials induces changes in susceptibility to antibiotics, biofilm formation and pathogenicity in staphylococcus aureus. Journal of Pharmaceutical Research International. 2021; 33: 140–151.
CLSI: Clinical & Laboratory Standards Institute. Control methods. Biological and micro-biological factors: Determination of the sensitivity of microorganisms to antibacterial drugs. Federal Center for Sanitary and Epidemiological Surveillance of Ministry of Health of Russia. 2019.
Manga MJA, Podoprigora IV, Volina EG, Ermolaev AV, Smolyakova LA. Evaluation of changes induced in the probiotic Escherichia coli M17 following recurrent exposure to antimicrobials. Journal of Pharmaceutical Research International. 2021; 33: 158-167.
Mondal AH, Yadav D, Mitra S, Mukhopadhyay K. Biosynthesis of silver nanoparticles using culture supernatant of shewanella sp. Ary1 and their antibacterial activity. International Journal of Nanomedicine. 2020; 15: 8295.
Ezemokwe GC, Aguiyi JC, Chollom FP. The antibacterial activity of aqueous and ethanolic leaf extracts of Balanites aegyptiaca (L.) Del plant on some selected clinical human pathogens. Journal of Advances in Microbiology. 2020; 20: 51–66.
Ibrahim M, Emlee A. Anti-fungal study on aqueous and ethanolic leaves extracts of Piper sarmentosum. Matrix Science Pharma. 2020; 4: 13.
Noshad M. Evaluation of the effect of aqueous and ethanolic extraction methods on extraction yield, phenolic compounds, and antioxidant and antimicrobial activity of Stachys schtschegleevii extract. Journal of food science and technology. 2020; 17: 117–125.
Gonfa T, Teketle S, Kiros T. Effect of extraction solvent on qualitative and quantitative analysis of major phyto-constituents and in-vitro antioxidant activity evaluation of Cadaba rotundifolia Forssk leaf extracts. Cogent Food & Agriculture. 2020; 6: 1853867.
Melander RJ, Melander C. The Challenge of Overcoming Antibiotic Resistance: an Adjuvant Approach? ACS Infectious Diseases. 2017; 3: 559–563.
Upendra Thapa Shrestha, Sabnum Shrestha, Nabaraj Adhikari, Komal Raj Rijal, Basudha Shrestha, Bipin Adhikari, et al. Plasmid profiling and occurrence of β-lactamase enzymes in multidrug-resistant uropathogenic Escherichia coli in Kathmandu, Nepal. Infection and Drug resistance. 2020; 13: 1905.
Onivogui G, Letsididi R, Diaby M, Wang L, Song Y. Influence of extraction solvents on antioxidant and antimicrobial activities of the pulp and seed of Anisophyllea laurina R. Br. ex Sabine fruits. Asian Pacific Journal of Tropical Biomedicine. 2016; 6: 20–25.
Al Farraj DA, Ragab Abdel Gawwad M, Mehmood A, Alsalme A, Darwish NM, Al-Zaqri N, et al. In-vitro antimicrobial activities of organic solvent extracts obtained from Dipcadi viride (L.) Moench. Journal of King Saud University - Science. 2020; 32: 1965–1968.
Aleksandra Owczarek, Joanna Kolodziejczyk-Czepas, Joanna Woźniak-Serwata, Anna Magiera, Natalia Kobiela, Katarzyna Wąsowicz, et al. Potential activity mechanisms of aesculus hippocastanum bark: Antioxidant effects in chemical and biological in vitro models. Antioxidants. 2021, 10: 995.
Mokdad-Bzeouich I, Mustapha N, Chaabane F, Ghedira Z, Ghedira K, Ghoul M, et al. Oligomerization of esculin improves its antibacterial activity and modulates antibiotic resistance. The Journal of Antibiotics. 2015; 68: 148–152.
Venugopala KN, Rashmi V, Odhav B. Review on Natural Coumarin Lead Compounds for their Pharmacological Activity. BioMed Research International. 2013; 2013: 1–14.
Izabela Nawrot-Hadzik, Adam Matkowski, Jakub Hadzik, Barbara Dobrowolska-Czopor, Cyprian Olchowy, Marzena Dominiak, et al. Proanthocyanidins and Flavan-3-ols in the Prevention and Treatment of Periodontitis—Antibacterial Effects. Nutrients. 2021; 13: 165.
Kuete V. Potential of Cameroonian Plants and Derived Products against Microbial Infections: a Review. Planta Medica. 2010; 76: 1479–1491.
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