In vitro antidermatophytic activity of bioactive compounds from selected medicinal plants

Fungal infections are among the most difficult diseases to manage in humans. Eukaryotic fungal pathogens share many similarities with their host cells, which impairs the development of antifungal compounds. Therefore, it is desirable to harness the pharmaceutical potential of medicinal plants for antifungal drug discovery. In this study, the antifungal activity of sixteen plant extracts was investigated against selected dermatophytic fungi. Of the sixteen plants, the cladode (leaf) of Asparagus racemosus, and seed extract of Cassia occidentalis showed antifungal activity against Microsporum gypseum, Microsporum nanum, Trichophyton mentagrophytes and Trichophyton terrestre. The plant antifungal compounds were located by direct bioassay against Cladosporium herbarum. IR and NMR spectrometry analyses of these compounds identified the presence of saponin (in A. racemosus) and hydroxy anthraquinone (in C. occidentalis) in these antifungal compounds. The antidermatophytic activity of plant anthraquinone and saponins with reports of little or no hemolytic activity, makes these compounds ideal for alternative antifungal therapy and warrants further in-depth investigation in vivo.


Introduction
Fungal infections are among the most difficult diseases to manage in humans. Reports indicate high rates of morbidity and mortality caused by fungal infections (CDC 2020). Despite their irreversible impact on human health, fungal pathogens have been mostly neglected by both the public and public health officials (Rodrigues and Nosanchuk 2020).
Dermatophytoses are characterized by superficial invasion by fungal hyphae in the skin, hair, and nails causing subacute or chronic infections (Burstein et al. 2020). Although dermatophyte infections are restricted to areas of the epidermis, they can be invasive and cause serious widespread infections in immunocompromised patients (Trottier et al. 2020). Major risk factors for the development of invasive fungal infections include, among others, HIV treatment in AIDS patients, cytotoxic chemotherapy in cancer patients, immunosuppressive therapy where innate defenses have been breached and the presence of catheters and other indwelling devices (Casadevall 2019; Li et al. 2020). Currently, mucormycosis also known as black fungus diseases, have been acquired as secondary infections in COVID-19 patients (Mahalaxmi et al. 2021).
As eukaryotic pathogens, fungi share many similarities with their host cells, which impairs the development of antifungal compounds (Rodrigues and Nosanchuk 2020). Cutaneous fungal parasites have survived several generations of therapeutic regimens, and the increasing invasive fungal infections along with the emerging resistance of pathogens and disadvantages with the existing antifungal drugs, demand the development of new antifungal drugs in clinical practice .
The antifungal potential of medicinal plants and their secondary metabolites against different fungal pathogens have been extensively studied (Chahal et al. 2021;Salhi et al. 2017;Mardani et al. 2018;Ezeonu et al. 2019;Simonetti et al. 2020;Alotibi et al. 2020;Kaur et al. 2021;Zagórska-Dziok et al. 2021). However, the limited armamentarium of the current classes of antifungal agents available (pyrimidine analogs, polyenes, azoles, and echinocandins), their toxicity, efficacy and the emergence of resistance are major bottlenecks limiting successful patient outcomes (Juvvadi et al. 2017;Chang et al. 2019). Plants contain a spectrum of secondary metabolites, such as phenols, coumarins, flavonoids, quinones, tannins and their glycosides, alkaloids, and essential oils. According to World Health Organization, medicinal plants would be the best source of a variety of drugs and numerous studies have been conducted on various medicinal plant extracts with the hope of discovering new and more efficient antifungal compounds (Scorzoni et al. 2017).
Plants have been widely used for their medicinal properties since ancient times . Plants produce a lot of antioxidants and represent a source of novel compounds with promising antioxidant activity (Salanţă et al. 2014). Acalypha indica has been used for many therapeutics purposes such as anti-bacterial and other applications (Zahidin et al. 2017). Achyranthus aspera is used in treatment of cough, bronchitis and rheumatism, malarial fever, dysentery, asthma, hypertension and diabetes in traditional Indian medicine (Bhosale et al. 2012). Annona reticulata with anti-inflammatory effects is known to contain phytochemicals like tannins, alkaloids, phenols, glycosides, flavonoids and steroids (Jamkhande and Wattamwar 2015). Annona squamosa leaves have been studied for their biological activities, including anticancer, antidiabetic, antioxidant, and antimicrobial functions (DeFilipps and Krupnick 2018). Asparagus racemosus is a highly valued medicinal plant in Ayurvedic medicine system for the treatment of various ailments such as gastric ulcers, dyspepsia and cardiovascular diseases (Srivastava et al. 2018). Cassia alata is traditionally used in the treatment of ringworms, tinea infections, scabies, blotch, herpes, and eczema (Oladeji et al. 2020).
Research findings indicate the therapeutic use of Cassia fistula as the rich source of antioxidant (Rahmani 2015). The antibacterial activities of leaves and rootbark extracts of Cassia occidentalis have been reported by Ibrahim et al. 2010. Upadhyay et al. 2014 reported the wound healing property of Cleome viscosa. Feronia elephantum fruit is traditionally used in India for the treatment for many liver disorders like jaundice (Sharma et al. 2012a, b). Ficus religiosa is used traditionally as antibacterial in the treatment of gonorrhea and skin diseases (Chandrasekar et al. 2010). Lantana camara is reported to have shown a wide range of antimicrobial activity (Kirimuhuzya et al. 2009). Terminalia catapa is often used in traditional medicine for the treatment of various infectious diseases (Ngouana et al. 2015). The wound healing potential of Wedelia trilobata leaves has been reported by Balekar et al. 2012. Ziziphus jujuba is known all around the world due to their health benefits, as both food and herbal medicine .
Therefore, in this study, the aforementioned sixteen plant specimens were selected and assayed for their antifungal activity against dermatophytic fungi in order to address the need for new antifungal agents with novel mode of action to be included as arsenals against drug resistant fungi.

Fungal Isolates
Test dermatophytic fungi Micorsporum gypseum MPS 199,901, M. nanum MPS 199,902, Trichophyton mentagrophytes MPS 199903 and T. terrestre MPS199904. (Ramesh and Hilda 1999;Anbu et al. 2004) were obtained from the Center for Advanced Studies in Botany, University of Madras, Chennai, India. These fungal specimens isolated from the city of Madras Parks and School playgrounds, were preserved in sterile distilled water at room temperature or in a cooling cabinet at 4℃ in the dark as described by Qiangqiang et al. (1998), Deshmukh (2002) and Nakasone et al (2004). The cultures were grown at 30 °C for 7 days on Potato Dextrose Agar and Sabouraud dextrose agar (SDA, HiMedia, India), respectively, prior to the antidermatophytic assay.

Preparation of plant extracts
Fresh plant parts were washed, shade dried and then ground into powder using electric grinder. One hundred gram of powdered samples was extracted with 80% ethanol in a Soxhlet extractor for 72 h (Kalaivanan et al. 2013). The extracts were then passed through two layers of cheese cloth and then centrifuged at 3000 g for 10 min at 4 °C. The clear supernatant was collected and concentrated (to completely remove the solvent) in a rotaevaporator at 40 °C. The crude extracts were stored in a freezer at − 20 °C for further use.

Antifungal activity of plant extracts
The antifungal effect of crude extract of test plants on the growth of dermatophytes was studied using Poisoned Food Technique (Jayshree et al. 2012). The crude extracts were dissolved in 10% aqueous dimethyl sulfoxide (DMSO), sterilized by filtration through a 0.45-μm membrane filter and assayed for their antifungal activity under aseptic condition. One milliliter of the test plant extract (in 10% DMSO) was mixed with 20 ml of sterilized Sabouraud dextrose agar (SDA) medium to yield a final concentration of 1 mg/ml. This mixture was immediately poured into Petri plates and allowed to solidify. The plates were inoculated in the center with 5-mm mycelia discs of 10-day-old test fungal culture. SDA medium was supplemented with reference antibiotic griseofulvin (MIC was 0.6 µg/ml for M. gypseum; 0.8 µg/ ml for M. nanum; 2.5 µg/ml for T. mentagrophytes; and 0.6 µg/ml for T. terrestre) as positive control, while SDA medium with 10% DMSO devoid of plant extract served as negative control. The plates were incubated at 28 ± 2° C for 14 − 21 days. After incubation, the diameter of the fungal growth in control and sample plates was recorded and the percentage of mycelial inhibition (I %) was calculated as I % = [(dc − dt)/dc] X 100 (dc = colony diameter in control, dt = colony diameter in treatment) (Jayshree et al. 2012). All experiments were carried out in triplicates. The plant extracts showing high inhibitory effect were selected for further study.

Phytochemical analysis of selected plant extracts
The crude extracts from cladodes of A. racemosus and seed of C. occidentalis were analyzed for the presence of alkaloids, phenolic compounds, tannins, cardiac glycosides, quinones, anthraquinones and saponins using standard methods listed as below (María et al. 2018;Trease and Evans 2002;Harbones 1998).

Test for alkaloids
For alkaloids, 10 mg of each extract was treated with a few drops of Dragendorff 's reagent and Mayer's reagent separately. The presence of alkaloids will be indicated by the formation of red-orange precipitate (Dragendorff ) and yellowish-white precipitate.

Test for phenols
To test the presence of phenolic compounds, 2 ml of alcoholic extract was treated with 5% ferric chloride. The presence of phenols will be indicated by the formation of a blue or black color.

Test for tannins
The test for tannins was carried out with 0.1% FeCl3. Formation of brownish green or a blue-black color shows the presence of tannins.

Test for saponins
The presence of saponins was tested by adding 0.5 g of crude extract to 2 ml of boiling water in a test tube and allowed to cool. The mixture was thoroughly shaken and observed for stable froth and further mixed with 3 drops of olive oil and shaken to observe formation of emulsion.

Test for quinones
Borntrager's test. The crude sample (20 mg) was treated with 3 mL of chloroform and the chloroform layer was separated. Then, 5% potassium hydroxide solution was added to the separated chloroform.

Test for anthraquinones.
Modified Borntrager's test. The crude extract (20 mg) was boiled with 3 ml of 10% hydrochloric acid for 3 min. The hot solution was filtered in a test tube, cooled and extracted gently with 3 ml of benzene. The upper benzene layer was pipetted off and shaken gently in a test tube with half of its volume of 10% ammonium hydroxide solution.

Detection of antifungal compounds by direct bioassay
Plants that showed high antifungal activity in the initial screening were (100 g of powdered samples of the cladodes of A. racemosus and seeds of C. occidentalis) extracted with petroleum ether and ethanol in a Soxhlet extractor for 72 h (Kalaivanan et al. 2013). Then, the extracts were filtered, pooled and solvents were evaporated in rota-evaporator under reduced pressure at 45 °C, and the crude extracts were kept at 4 °C in refrigerator until further use. To detect the antifungal compounds, 100 μl of crude extracts (petroleum ether and ethanol) of A. racemosus and C. occidentalis were applied on a pre-activated (at 100 °C for 30 min) silica gel thin-layer chromatography (TLC) plates (Eastman 6069). The chromatogram was developed in a mixture of benzene and ethyl acetate (7:3) to a distance of 11 cm and dried at room temperature.
Antifungal compounds separated on TLC plates were bio-assayed according to the method described by Tabanca et al. (2005) with slight modification. Conidia from a week old Cladosporium herbarum growing on potato dextrose agar were harvested and washed by centrifugation. A highly concentrated conidial suspension was sprayed on thin chromatograms which were then oversprayed with half strength potato dextrose agar medium (PDA) at 45 °C. The sprayed chromatograms were incubated in moist chamber at room temperature for 48 h. The chromatograms were briefly air dried and sprayed with half strength PDA medium and incubated further in a moist chamber for 24 h at room temperature. At the end of the period, inhibitory area appeared as white zones on a green background of the mycelium. The Rf values of the antifungal zones were measured. Rf = distance traveled by sample/distance traveled by solvent.

Antifungal assay of bioactive compounds
The antifungal compound detected by direct bioassay was eluted in respective solvents and loaded onto 9-mm filter paper discs (100 μg/disc). Petri plates containing Sabouraud dextrose agar medium were seeded with 0.1 ml of standardized spore suspension of test fungi, and the assay discs were aseptically transferred to Petri plates and incubated at room temperature (28 ± 1 °C) for a period of 7 days. The antifungal activity was assessed by measuring the zone of inhibition around the disc and compared with ketoconazole (15 μg/disc) control.

Minimum inhibitory concentration assay
The minimum inhibitory concentrations (MICs) of antifungal compounds against dermatophytes were determined using the standard broth microdilution assay according to the guidelines of Clinical and Laboratory Standards Institute M38 (CLSI 2017). The test fungi were grown in Sabouraud Dextrose Agar (SDA) at 30 °C for 48 h and adjusted to a final density of 1 × 10 8 CFU/mL by suspending in sterilized normal saline solution. The MIC values of test samples were determined as described by Kalaivanan et al. (2013) and Chellappandian et al. (2018). Twenty microliters of plant extract (50 mg/mL) in 10% DMSO was added to 980 µL of RPMI-1640 to yield the concentration 1000 µL (1 mg/mL). This solution was used for twofold serial dilutions to attain concentrations ranging from 3.9 to 1000 µg/mL. Two hundred microliters of the solution was placed into the first well of a 96-well microtiter plate, and then, 100 µl from the first well was transferred to the next well containing 100 µl of RPMI-1640. The same procedure was performed for all wells. A volume of 100 µL of standardized inoculum suspensions was transferred on to each well. Ketoconazole was used as positive antifungal control, and 10% DMSO was used as negative control. Each experiment was performed in triplicate and repeated twice. The MIC was interpreted as the lowest concentration of the test samples showing no visible growth.

Spectrometric analysis of antifungal compounds
IR and NMR spectrum of the purified antifungal compounds from A. racemosus (cladodes) and C. occidentalis (seed) was analyzed using IR-P-983 spectrometer and EM-390 (90 MHz) NMR spectrometer as described by Ganesan andMathuram (2020), andAkhtar et al. (2017). Deuterochloroform (CDCl 3 ) was used as an internal reference for NMR studies.

Statistical analysis
The results were expressed as the mean ± standard deviation. All statistical analyses were performed using SPSS version 27.0 statistical software, and comparison of treatments was carried out using one-way analysis of variance (ANOVA) and Turkey HSD test. P value < 0.05 was considered statistically significant.

Antifungal activity of plant extracts against dermatophytes
Of the sixteen plant species tested, crude ethanol extracts from cladodes (leaves) of A. racemosus and seed extract of C. occidentalis completely inhibited the mycelial growth of all four species of dermatophytes tested (Fig. 1). Compared to griseofulvin 0.6 µg/ml for M. gypseum; 0.8 µg/ml for M. nanum; 2.5 µg/ml for T. mentagrophytes; and 0.6 µg/ml for T. terrestre (positive controls), the leaf extracts of A. indica, A. aspera, A. reticulata, A. squamosa, C. alata, F. religiosa and L. camera exhibited about 60% inhibition, while the remaining plants showed low inhibitory effect against the test dermatophytes. The negative control (10% DMSO) showed no antifungal activity. Therefore, A. racemosus and C. occidentalis were selected for further study.

Phytochemical analysis of plant extracts
Phytochemical screening of ethanolic extracts from the seed of C. occidentalis and the cladode of A. racemosus was carried out using various chemical assays in order to identify either the presence or absence of secondary metabolites that are useful in treating various ailments. Table 1 summarizes the phytochemicals present in assayed alcoholic extracts. Both extracts tested positive to Dragendorff (observing an orange precipitate) and Mayer's test (formation of yellowish-white precipitate) indicating the presence of alkaloids. The seed extract of C. occidentalis also showed positive results for phenols, Page 5 of 13 Savarirajan et al. J Anal Sci Technol (2021) 12:53 tannins, quinones and anthraquinones but was negative for saponins. The cladode of extract of A. racemosus tested positive for the presence of saponins, phenols and steroids but showed negative results for tannins, quinones and anthraquinones.

Detection of antifungal compounds by direct bioassay
The Rf values of the antifungal zones on the TLC plates were measured (Fig. 2   Page 6 of 13 Savarirajan et al. J Anal Sci Technol (2021) 12:53 any of the test dermatophytes, whereas the antifungal compounds from ethanol extract detected at the Rf value of 0.3 were inhibitory to all the test fungi. The antifungal compounds detected at the Rf value of 0.92 from petroleum ether extract of C. occidentalis showed inhibitory effect against all the dermatophytes tested, whereas compounds at Rf 0.46 showed no inhibitory effect against any of the test dermatophytes ( Table 2). The antifungal compounds from ethanol extract also showed no inhibitory effect against any the test dermatophytes. Therefore, the antifungal compounds showing inhibitory effect from C. occidentalis (Rf 0.92) and A. racemosus (Rf 0.3) were chosen for further characterization.

Minimum inhibitory concentration assay
Evaluation of MIC of TLC detected antifungal compounds C. occidentalis and A. racemosus indicated variable inhibitory effects (Table 3). The MICs of the two bioactive compounds were ranging from 15.62 to 62.5 μg/mL. Among all the tested fungi, M. gypseum was highly sensitive to both compounds, followed by M. canis and T. terestre.

IR spectrum of antifungal compounds from cladode extract of A. racemosus and seed extract C. occidentalis
The TLC detected antifungal compounds were partially characterized using IR and NMR spectral studies. The IR spectrum of antifungal compound from A. racemosus showed a broad peak at 3550-3450 cm −1 indicating the presence of OH group (Fig. 3). Formation of peaks around 920, 890 and 840 showed the presence of typical spirochetal side chain suggesting that it is spirostanol glycosides.
The IR spectrum of antifungal compound from C. occidentalis showed 2 broad peaks at 3480 cm −1 and 3580 cm −1 indicating the presence of phenolic OH (Fig. 4). Peaks at 2990 cm −1 showed the presence of C-H stretching frequency. The presence of aromatic skeleton was shown by the formation peaks at 3000, 1500, 820 and 740 cm −1 . The absorption peak at 1640 cm −1 showed the presence of (carboxyl group) carbonyl band.

Discussion
Fungal members belonging to various taxonomical groups detected in the soil of areas of various human activities are potentially pathogenic to human and animals (Wójcik 2016). Some of them are considered as emerging pathogens (Wójcik 2016;Friedman and Schwartz 2019;Morio 2020). Reports indicate health concerns due to public parks and school playgrounds as ideal environment for the growth of pathogenic fungal   Khodadadi et al. 2021). Besides the evolutionary pressure from the antifungal drugs, it is now identified that environmental pressures including the climate change are affecting the fungal evolution to confer novel traits including virulence and antifungal resistance (Nnadi and Carter 2021). Human-dominated environments like parks or playground are natural niches of dermatophytic fungi and pose a public health problem. Hence, in the search for alternative therapies for the emerging resistant fungal strains, we investigated the potential antifungal effect of several plant extracts on dermatophytes isolated from public parks and school playgrounds. The different parts of C. occidentalis and A. racemosus such as root, leaves, seeds and pods have been used in traditional medicines for the treatment of various infectious and non-infectious diseases (Fidèle et al. 2017;Karuna et al. 2017;Srivastava et al. 2018;Okonkwo et al. 2019). In this present study, the extracts of C. occidentalis (seed) and A. racemosus (cladode) inhibited the growth of all the tested dermatophytic fungi (Table 1).

M. gypseum
Similarly, the antifungal activity against fluconazole resistant Candida isolates was reported in Cassia fistula (Sony et al. 2018). Cassia fistula seed extract reportedly disrupts the cell membrane in C. albicans, resulting in damage to yeast cells (Sitarek et al. 2020a, b). Onlom et al. (2014) reported the in vitro antifungal   Savarirajan et al. J Anal Sci Technol (2021) 12:53 activity of A. racemosus roots extracts against Malassezia spp. and its potential use as an active ingredient in an anti-dandruff formulation.
Medicinal plants produce a diverse range of bioactive molecules that provide reliable therapy in the treatment of various diseases and skin infections in humans (Sitarek et al. 2020a, b). The phytochemical analysis of the ethanolic extract of C. occidentalis indicated the presence of phenols, tannins, quinones and anthraquinones but was negative for saponins. The cladode extract of A. racemosus, tested positive for the presence of saponins but did not contain phenols, tannins, quinones and anthraquinones. Previous studies reported that the presence of saponins and flavonoids in these plants plays a role in therapeutic applications (Onlom et al. 2017;Srivastava et al. 2018;Issa et al. 2020).
The plant kingdom has an immense potential for the safe use of natural products in treatment of invasive and systemic fungal infections (D'agostino et al. 2019). Evaluation of MIC of the TLC detected bioactive compounds, C. occidentalis and A. racemosus, indicated variable inhibitory effects against fungal pathogens (Table 3). Among all the tested fungal specimens, M. gypseum was highly sensitive to both compounds from C. occidentalis and A. racemosus, followed by M. nanum and T. terestre. When compared to the antifungal activity of antibiotics reported by Banfalvi (2020), M. gypseum was more susceptible to gentamicin B1 (MIC 3.1 µg/mL). However, evidence shows antifungal topicals are more expensive when used in combination with corticosteroid and less effective as single-agent antifungals (Wheat et al. 2017). Therefore, the synergistic potential of the test plant extracts with topical antifungals that are already in medical use, makes it a promising alternative for antifungal therapy. This approach could help curb the rise in chronic and recalcitrant dermatophytosis cases (Tuknayat et al. 2020).
In the present study, fractions from C. occidentalis and A. racemosus that were inhibitory to the test dermatophytes were partially characterized by IR, NMR and identified as dihydroxy anthraquinone and spirostanol saponin, respectively. The compound from the cladodes of A. racemosus was identical in spectral properties (IR and NMR) with those reported for spirostanol saponin (Sharma et al. 2012a, b;Sharma et al. 2009). Therefore, it is concluded that the compound isolated from the ethanol extract of A. racemosus (cladode) may be spirostanol saponin. Saponins perforate lipid bilayers and increase the permeability of the cell membrane allowing transport of molecules that would otherwise be excluded Efimova and Ostroumova 2021). The antidermatophytic activity of spirostanol saponin isolated from A. racemosus cladode in our study is similar to other findings. Antimycotic activity of spirostanol saponins has been reported in Solanum hispidum leaves (Manases González et al. 2004;Diretto et al. 2017;El Sayed et al. 2020;Dąbrowska-Balcerzak et al. 2021). Therefore, this plant saponin has great potential to bolster the antifungal armamentarium for treatment of fungal infections that does not respond to conventional therapy.
The IR and NMR spectrum data for the antifungal compound from the seeds of C. occidentalis, inferred that the compound has anthraquinone skeleton which was identical in spectral properties to those reported for dihydroxy methyl anthraquinone derivative (Tiwari and Singh 1979;Mehta 2012). According to Brilhante, (2020), the antifungal mechanism of anthraquinones may be related to the inhibition of (1,3)-β-D-glucan synthase activity, leading to disruption of (1,3)-β-Dglucans in the fungal cell wall. High antifungal activity of anthraquinone aglycones was reported against clinical strains of dermatophytes in Senna alata leaves, and C. fistula pod pulp (Wuthi-udomlert et al. 2010;Chewchinda et al. 2013;Friedman et al. 2020) reported the inhibitory potency of plant derived anthraquinones against pathogenic fungi.
The antidermatophytic activity of anthraquinone and saponins has been confirmed by several studies (Njateng et al. 2013;Yang et al. 2019). Phytochemical screening of Polyscias fulva indicated antidermatophytic activity of saponins, tannins, alkaloids, and anthraquinones (Njateng et al. 2013). Reports on Cassia occidentalis poisoning are rare (Chappola et al. 2018). Moreover, to avoid unwanted side effects, natural anthraquinones are preferred as an alternative antifungal. Hence, Cassia occidentalis, a traditional Ayurvedic edible shrub with anthraquinones as the principle active constituent, warrants further investigation for development of novel antifungals for treatment of filamentous fungal dermatophytes.
Climate changes can affect epidemiology of fungal disease, leading to the emergence of new virulent strains (van Rhijn and Bromley 2021). Conventional antifungal drugs like griseofulvin gets quickly eliminated from the body and must be taken over an extended period to have efficacy and therefore have adverse side effects (Gupta et al. 2018). Therefore, the quest for alternative therapies with new antimicrobial mechanisms has become an urgent priority to overcome the developing resistance of fungal pathogens (Shaban et al. 2020). Plants are an indispensable source of novel compounds that can be used for the treatment of multidrug-resistant (MDR) fungal infections (Marquez and Quave 2020). Needless to say, novel antifungal agents in the drug development pipeline hold a promising future for antifungal therapeutics (Wall and Lopez-Ribot 2020).

Conclusions
In conclusion, the results demonstrated that extracts from A. racemosus cladodes and seed of C. occidentalis have strong antifungal activity against dermatophytic fungal species, M. gypseum, M. nanum, T. mentagrophytes and T. terrestre. Partial characterization of the antifungal compounds from these two plant species using IR and NMR inferred the two compounds from C. occidentalis as hydroxy anthraquinone and from A. racemosus, as saponin. Conventional antifungal agents have limited effectiveness due to their common side effects. The antidermatophytic activity of plant anthraquinone and saponins with reports of little or no hemolytic activity, makes these compounds ideally suited for alternative antifungal therapy. The precise determination of selective antifungal activity of hydroxy anthraquinone and saponin warrants future in-depth investigation in vivo. The results of the present investigation support the traditional use of the selected medicinal plants in the treatment of various infections. They also provide an important basis for further studies to test the clinical safety and efficacy of the phytotherapeutic bioactive compounds. Comparison of the antifungal effect on multiple fungal strains along with a standard fungal strain would be necessary to provide additional valid information for the future therapeutic applications against other fungal pathogens.