Startseite Lebenswissenschaften Susceptibility of Microsporum canis arthrospores to a mixture of chemically defined essential oils: a perspective for environmental decontamination
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Susceptibility of Microsporum canis arthrospores to a mixture of chemically defined essential oils: a perspective for environmental decontamination

  • Simona Nardoni EMAIL logo , Annamaria Tortorano , Linda Mugnaini , Greta Profili , Luisa Pistelli , Silvia Giovanelli , Francesca Pisseri , Roberto Papini und Francesca Mancianti
Veröffentlicht/Copyright: 26. Februar 2015

Abstract

The zoophilic dermatophyte Microsporum canis has cats as natural reservoir, but it is able to infect a wide range of hosts, including humans, where different clinical features of the so-called ringworm dermatophytosis have been described. Human infections are increasingly been reported in Mediterranean countries. A reliable control program against M. canis infection in cats should include an antifungal treatment of both the infected animals and their living environment. In this article, a herbal mixture composed of chemically defined essential oils (EOs) of Litsea cubeba (1%), Illicium verum, Foeniculum vulgare, and Pelargonium graveolens (0.5% each) was formulated and its antifungal activity assessed against M. canis arthrospores which represent the infective environmental stage of M. canis. Single compounds present in higher amounts in the mixture were also separately tested in vitro. Litsea cubeba and P. graveolens EOs were most effective (minimum inhibitory concentration (MIC) 0.5%), followed by EOs of I. verum (MIC 2%) and F. vulgare (MIC 2.5%). Minimum fungicidal concentrations (MFC) values were 0.75% (L. cubeba), 1.5% (P. graveolens), 2.5% (I. verum) and 3% (F. vulgare). MIC and MFC values of the mixture were 0.25% and 0.5%, respectively. The daily spray of the mixture (200 μL) directly onto infected hairs inhibited fungal growth from the fourth day onwards. The compounds present in higher amounts exhibited variable antimycotic activity, with MIC values ranging from >10% (limonene) to 0.1% (geranial and neral). Thus, the mixture showed a good antifungal activity against arthrospores present in infected hairs. These results are promising for a further application of the mixture as an alternative tool or as an adjuvant in the environmental control of feline microsporosis.

1 Introduction

Dermatophytosis due to Microsporum canis represents the most common fungal skin infection in cats [1]. This zoophilic dermatophyte is able to infect a wide range of hosts, including humans, where different clinical features have been reported. The incidence of skin disease due to M. canis has increased in the recent years, in particular in Mediterranean countries, being the most prevalent agent of tinea capitis in children [2]. Tinea faciei and tinea corporis have also been reported recently, mostly as result of contact with pets [3]. Infected cats have been proven to contaminate the environment by shedding arthroconidia (arthrospores) which are asexual spores derived from fragmentation of fungal hyphae that are able to invade hairs and scales [4]. These fungal elements, embedded in hairs and skin debris are highly resistant at room temperature, may be viable up to 18 months and are thus responsible for infection and/or reinfection [5]. For these reasons, a reliable control program should include an antifungal treatment of both animals and their living environment. Aggressive removal of contaminated material followed by thorough application of commercial ready-to-use disinfectants is strongly suggested, and several commercially available sporocidal products have been successfully checked [6]. Users are advised to read labels to avoid toxicity risk for pets and children and to follow the manufacturer’s recommendations regarding target surfaces [7]. Furthermore, these products frequently present a variety of environmental concerns [8]. Hence, there is a growing interest of consumers in ingredients from natural sources; phytochemicals would be considered as alternatives to synthetic disinfectants/antimycotics also because many of them are relatively non-toxic to mammals and the environment. Essential oils (EOs) are gaining increasing interest because of their relatively safe status, their wide acceptance by consumers and their exploitation for potential multipurpose functional use. EOs are complex mixtures comprising many single compounds, chemically mostly of terpenoid origin, and have been used for many thousands of years in food preservation, pharmaceuticals, alternative medicine and natural therapies [9]. Antifungal activity of EOs has been demonstrated both against pathogenic fungi causing mycoses [10–12] and against fungi causing food spoilage and producing mycotoxins [13].

Essential oils from a number of plants exhibited good anti- M. canis activity both in vitro and in topical treatment of naturally infected cats [11], while no information was available on their environmental use. For these reasons, the aims of this article were to formulate an herbal mixture and to assess its antifungal activity against M. canis arthrospores with special reference to an environmental application.

2 Materials and methods

2.1 Essential oils

Essential oils from star anise (Illicium verum), bergamot (Citrus bergamia), cinnamon (Cinnamomum zeylanicum), fennel (Foeniculum vulgare), geranium (Pelargonium graveolens), litsea sambal (Litsea cubeba), spearmint (Mentha spicata), sandal (Santalum album) and incense (Boswellia sacra) were selected for this study based on their efficiency as antiseptics [14–20], pleasant smell, and safety for both human and animals. The nine selected EOs were examined for both their composition by GC-MS analysis and antimycotic activity by in vitro tests.

2.2 GC-MS analysis

Volatile constituents of each EO were analyzed by GC-MS as previously reported [21]. Briefly, a CP-3800 gas chromatograph equipped with HP-5 capillary column and a Varian Saturn 2000 ion trap mass detector were employed. Analytical conditions were as follows: injector and transfer line temperature, 220 and 240 °C, respectively; oven temperature, programmed from 60 to 240 °C at 3 °C/min; carrier gas, helium at 1 mL/min; injection, 0.2 mL (10% hexane solution); split ratio, 1:30. Identification of the constituents was based on comparison of the retention times with those of authentic samples, comparing their linear retention indices relative to the series of n-hydrocarbons, and on computer matching against commercial and home-made library mass spectra built up from pure substances and components of known oils and MS literature data [22, 23].

2.3 Source of infected hair samples

Shortly before starting the in vitro tests, M. canis ringworm was diagnosed in a symptomatic, male, European short hair, 2-month-old kitten by the hair-brushing technique and colony identification in culture. In some cases of feline ringworm caused by M. canis, a metabolite (pteridine) is produced within infected hairs that lets them fluoresce yellow-green under ultraviolet light. Therefore, the kitten was examined under Wood’s lamp to allow the identification of hairs containing infectious arthrospores. A number of entirely fluorescent, and thus certainly infected hairs, were cut by the use of scissors. After collection, all infected hairs were kept within the same Petri dish and stored in the dark at room temperature (22–25 °C) until tests were performed.

2.4 In vitro susceptibility studies

The antimycotic activity of each EO listed previously was evaluated by a microdilution test on the collected hairs, using the technique described by Mugnaini et al. [11] slightly modified. Briefly, all tests, including EOs or mixtures (see the following), were carried out in triplicate in 24 well plates. Stock solutions at 10% (v/v) of the listed EOs in 95% ethanol were diluted into a semisolid malt extract with 1% agar as culture medium to obtain concentrations ranging from 3% to 0.05%. Such dilutions were arbitrarily chosen considering that a concentration of 3% is the highest for in-home use. In detail, 3%, 2.5%, 2%, 1.5%, 1%, 0.75%, 0.5%, 0.25%, 0.2%, 0.1% and 0.05% dilutions were checked. Each well was seeded with an inoculum of infected hairs (n=5) obtained as mentioned. The viability of inocula was evaluated by seeding control wells containing culture medium with and without ethanol. Plates were incubated at 25 °C for up to 10 days, or until mycotic growth was visually detected in control wells, to determine minimum inhibitory concentration (MIC) values. To further evaluate if lack of growth was due to a fungistatic or fungicidal effect and to assess minimum fungicidal concentration (MFC) values of the EOs, inocula which did not grow were washed with distilled water, subcultured onto malt extract agar and incubated at 25 °C for 4 weeks.

After preliminary results on the effectiveness of each single EO, the most effective were selected to compose a mixture for a further trial. Therefore, inocula, obtained as described, were also tested against a mixture composed of 1% L. cubeba, 0.5% I. verum, 0.5% F. vulgare and 0.5% P. graveolens, in 95% ethanol. The mixture was formulated on the basis of the antimycotic efficiency of each ingredient when tested alone, as well as of pleasant smell, considering that, when infected subjects are present, the whole environment where the animals are allowed to roam should be treated. In order to reproduce conditions similar to environmental usage, the mixture was checked at dilutions of 50%, 25%, 10%, 5%, 1%, 0.5%, 0.25% and 0.1%. Minimum inhibitory concentration and MFC values were assessed.

Single components present in amounts of >10% in EOs selected to formulate the mixture and/or known for their antifungal activity were separately tested in vitro as well. So anethole, citronellol, geranial, neral, geraniol, fenchone and limonene were assayed against M. canis obtained as described. All tests were carried out in triplicate. The viability of the inocula was evaluated as described.

In addition, the mixture was assayed by direct spraying of 200 μL onto 50 infected hairs, once a day for 1 week. After each spraying, hairs were left to air dry and five of them subcultured onto Sabouraud medium supplemented with chloramphenicol (0.05 g/L) and cycloheximide (0.4 g/L).

3 Results

3.1 GC-MS analysis

The chemical composition of the tested oils is reported in Tables 1 and 2.

Table 1:

Major classes of constituents of the tested essential oils (area percentage, %) determined by GC-MS.

Class of constituents compoundsBoswellia sacraLitsea cubebaMentha spicataSanthalum albumPelargonium graveolensIllicium verumCinnamonum zeylanicumFoeniculum vulgareCitrus bergamia
Monoterpene hydrocarbons84.294.427.080.000.003.030.008.2338.80
Oxygenated monoterpenes6.7650.3776.690.0086.160.0018.6819.3757.74
Sesquiterpenes hydrocarbons3.7439.5710.525.637.770.000.000.001.62
Oxygenated sesquiterpenes0.000.331.5288.794.140.000.380.000.46
Phenylpropanoids0.250.000.000.000.0094.2080.1467.900.00
Others0.001.380.180.001.190.000.001.920.12
Total95.0496.0795.9994.4299.2697.2399.2097.4298.74
Table 2:

Constituents of the tested essential oils (area percentage,%) determined by GC-MS.

CompoundLRI§Boswellia sacraLitsea cubebaMentha spicataSanthalum albumPelargonium graveolensIllicium verumCinnamonum zeylanicumFoeniculum vulgareCitrus bergamia
α-Thujene93254.19
Tricyclene9380.21
α-Pinene9406.211.120.630.4002.2400.43
Camphene9550.800.33
Thuja-2,4(10)-diene9597.26
Sabinene9780.370.950.4500.1100.54
β-Pinene9811.100.921.0000.482.81
6-Methyl-5-hepten-2-one9901.38
Myrcene9930.451.090.1000.500.62
3-Octanol9980.18
α-Phellandrene10063.6901.29
iso-Sylvestrene10090.24
α-Terpinene10195.14
o-Cymene10263.300.61
p-Cymene10281.673.75
Limonene10320.3610.841.652.901.7627.06
1,8-Cineole10360.645.210.14
(Z)-β-Ocimene10420.46
(E)-β-Ocimene10530.14
γ-Terpinene10620.110.183.45
cis-Sabinene hydrate10720.270.95
trans-Linalool oxide (furanoid)10790.85
Terpinolene10900.400.10
Fenchone109017.4018.39
cis-Linalool oxide (furanoid)10940.98
Linalool11020.161.660.73.9000.1016.83
cis-Thujone11081.05
cis-Rose oxide11110.99
trans-Thujone11200.32
trans-Rose oxide11310.42
cis-Limonene oxide113700.32
trans-Sabinol11400.09
trans-Pinocarveol11420.10
trans-Limonene oxide11420.22
Sabinol11431.52
trans-Verbenol11450.39
neo-Isopulegol11460.14
Camphor11480.60
cis-Verbenol11490.08
Menthone115416.461.07
neo-3-Thujanol11540.20
Citronellal11551.70
Isomenthone11643.48
neo-Menthol116611.18
Menthol117839.03
4-Terpineol11800.300.830.15
Isomenthol11830.77
neo-iso-Menthol11870.21
α-Terpineol11920.750.310.250.290.28
Myrtenol11950.11
Methyl chavicol (= estragol)11982.89
Safranal120000.16
trans-para-Menthan-2-one120500.11
γ-Terpineol12070.11
Octanol acetate12140.12
trans-Carveol12210.15
Nerol12280.86
cis-Carveol12290.18
Citronellol123144.46
cis-para-Mentha-1(7),8-dien-2-ol12310.15
Pulegone12373.29
(E)-β-Ocimenone12380.13
Isobornyl formate12392.54
Neral124231.970.180.15
Cuminaldehyde12440.79
Carvone12480.23
(Z)-Anethole12530.06
trans-Sabinene hydrate acetate12560.15
Piperitone12580.59
para-Anisaldehyde12581.92
Geraniol12591.4813.73
Linalool acetate126034.47
neo-Menthyl acetate12740.36
Geranial127636.890.700.26
Citronellyl formate12800.487.26
(E)-Anethole128394.2065.01
Safrole12911.36
Menthyl acetate12946.94
Geranyl formate12981.920.48
α-Cubebene13510.25
α-Terpinyl acetate13520.28
Citronellyl acetate13530.44
neo-iso-Dihydro carveol acetate13590.65
Eugenol136164.77
Neryl acetate1368
α-Ylangene13720.31
α-Copaene13761.52 0.26
β-Bourbonene13830.390.50.73
Geranyl acetate13840.68
β-Elemene13920.230.13
Methyl eugenol14070.19
β-Cedrene14180.17
α-Santalene14180.58
β-Caryophyllene14182.212.090.680.23
β-Copaene14290.12
β-Gurjunene1432
trans-α-Bergamotene14370.120.53
α-Guaiene14400.28
Aromadendrene14450.102.86
epi-β-Santalene14490.58
Isoeugenol144914.01
Citronellyl propanoate14500.72
α-Humulene14560.220.090.21
allo-Aromadendrene14610.22
β-Santalene14611.42
9-epi-(E)-Caryophyllene14670.230.11
β-Chamigrene14750.16
γ-Muurolene14770.13
Geranyl propanoate14780.68
γ-Curcumene14810.25
Germacrene D14810.880.670.20
ar-Curcumene1484
β-Selinene14850.34
Valencene14930.25
Bicyclogermacrene14950.15
Viridiflorene14950.63
α-Muurolene14990.25
β-Dihydro agarofuran15000.86
cis-Dihydro agarofuran15030.33
β-Bisabolene15090.330.76
α-Alaskene15110.28
trans-γ-Cadinene15130.19
(Z)-γ-Bisabolene15150.20
7-epi-α-Selinene15190.40
δ-Cadinene15230.72
β-Sesquiphellandrene15240.38
Kessane1528
Citronellyl butyrate15321.19
Furopelargone A15400.18
Selina-3,7(11)-diene15421.00
α-Agarofuran15480.63
Elemol15534.69
Geranyl butyrate15641.11
(E)-Nerolidol15660.28
Spathulenol15770.270.25
Caryophyllene oxide15820.330.690.85
(E)-2-Phenyl ethyl tiglate15851.19
Viridiflor15910.56
Caryophyllene oxide15920.1700.46
Guaiol15970.620.26
Geranyl-2-methyl butyrate16070.22
Humulene epoxide II16070.2200.21
1,10-di-epi-Cubenol16140.33
Citronellyl pentanoate16250.20
epi-10-γ-Eudesmol16274.870.92
1-epi-Cubenol16300.21
Eremoligenol16320.41
γ-Eudesmol16345.16
Hinesol16380.49
Cubenol16410.33
β-Eudesmol16495.52
4-α-hydroxy-dihydro agarofuran16530.22
α-Cadinol16550.37
(Z)-Citronellyl tiglate16581.15
Valerianol165814.35
7-epi-α-Eudesmol16645.92
(E)-Citronellyl tiglate16680.22
(Z)-α-Santalol167227.09
(Z)-trans-α-Bergamotol16912.00
Geranyl tiglate16961.19
(Z)-β-cis-Santalol17052.13
(Z)-β-trans-Santalol171010.75
(E)-β-Santalol17400.59
6S,7R-Bisabolone17500.50
Drimenol17590.44
(Z)-Lanceol17681.16

§LRI, Linear Retention Index calculated on the basis of the retention times of a mixture of n-alkanes (C8–C30).

3.2 In vitro susceptibility studies

Essential oils showing antimycotic activity at dilutions ≤3% were L. cubeba and P. graveolens (MIC 0.5% each), followed by I. verum (MIC 2%) and F. vulgare (MIC 2.5%). Their MFC values were 0.75% (L. cubeba), 1.5% (P. graveolens), 2.5% (I. verum) and 3% (F. vulgare).

The whole mixture composed of 1% L. cubeba, 0.5% I. verum, 0.5% F. vulgare and 0.5% P.graveolens, in 95% ethanol was effective with MIC and MFC values of 0.25% and 0.5%, respectively.

The main constituents present in each EO selected to formulate the mixture showed variable antimycotic activity, ranging from MIC >10% (limonene) to 0.1% (geranial and neral). MFC was equal to MIC for citronellol and geraniol, while all other tested compounds, including the mixture, were fungicidal at concentrations higher than the MIC. More detailed results are reported in Table 3. The mixture sprayed on infected hairs inhibited fungal growth from the fourth day of spraying onwards.

Table 3:

Minimal inhibitory (MIC) and fungicidal (MFC) concentrations, respectively, of the mixture of EOs and their major constituents.

CompoundMIC, %MFC, %
Mixture0.250.5
Foeniculum vulgare2.53
Illicium verum22.5
Litsea cubeba0.50.75
Pelargonium graveolens0.51.5
Anethole15
Citronellol0.250.25
Geranial0.10.25
Geraniol0.250.25
Limonene>10>10
Neral0.10.25
Fenchone0.250.5

4 Discussion

In this article, the antifungal activity of a mixture composed of 1% L.cubeba, 0.5% I. verum, 0.5% F. vulgare and 0.5% P. graveolens, in 95% ethanol against the parasitic form of M. canis (arthrospores) in infected cat hairs was investigated.

Considering that arthrospores, the infective element, are present on the broken hairs, and contamination of the environment from these sources is common, this work represents the first attempt to assess the antifungal role of EOs in environmental decontamination from M. canis. Our results can be only partially compared with those of Mugnaini et al. [11], who topically administered a mixture composed by 5% O. vulgare, 5% R. officinalis and 2% T. serpillum essential oil, respectively, in sweet almond oil to seven M. canis infected cats with satisfactory results. In fact, in this article EOs were dissolved in 95% ethanol, which is a solvent appropriate for environmental usage and not suitable for in vivo administration.

Litsea cubeba showed the lowest MIC and MFC values, probably due to its high content of geranial (36.8%) and neral (31.9%) which exhibited a strong antifungal activity as single compounds. P. graveolens also gave good results, probably due to the presence of geraniol and citronellol accounting for 13.7% and 44.4% of the total oils. The MIC and MFC shown by I. verum were 2% and 2.5%, respectively. These values were slightly higher in F. vulgare. The difference could be due to the lower amount of anethole present in the fennel EO.

Essential oils selected for the mixture are known to have antiseptic properties. All EOs showed antifungal effects and have previously been tested mostly against plant pathogens and postharvest pathogenic fungi, except for P. graveolens [24] and I. verum [11] that were assayed also against several Trichophyton species and M. canis, respectively, with antifungal activities agreeing to those found in the present study. L. cubeba was effective against Aspergillus niger, Alternaria alternata, Fusarium moniliforme and Fusarium solani [25], while F. vulgare inhibited several fungi responsible for food spoilage [26]. Furthermore P. graveolens and I. verum were active against plant pathogens [17, 27].

Most of the represented components, except for limonene, provided good antimycotic activity in agreement with literature data [28–30], in particular the isomers of citral (neral and geranial) are the main components of L. cubeba EO. Citral has a strong influence on fungi [31], being able to injure the wall and the membrane of Aspergillus flavus spores. This action results in a decrease of elasticity, and in a changed aggregation of protein-like macromolecules.

Tests of the sensitivity of dermatophytes to EOs described in the literature have been performed with fungal mycelia cultured from clinical isolates, which is not the form of spreading in the environment as represented by arthrospores [7]. In the present work, M. canis arthrospores embedded in infected hairs were employed to reproduce an in-field situation to set up an effective mixture for environmental usage.

The EO mixture showed MIC and MFC values lower than that obtained for L. cubeba, the most effective ingredient. These findings could be ascribed to synergism of the different active components.

Conventional treatment of infected environments has been exhaustively investigated by Moriello et al. [7], who reported complete inhibition of M. canis by commercial disinfectants at concentrations ranging from 3.2% for disinfectants containing lactic acid, to 0.22% for disinfectants based on quaternary ammonium derivatives. Thus, the mixture prepared by us, being effective at a concentration of 0.25%, showed antimycotic activity comparable to that of the most effective commercial product.

The direct application of the mixture on infected hairs inhibited fungal growth at day 4, with a total amount of 800 μL sprayed on the specimens. This volume was lower than that required to obtain the same results with some commercial disinfectants [7]. The mixture sprayed on soft furnishing did not stain (data not shown), unlike some conventional disinfectants such as sodium hypochlorite and lime sulphur. Furthermore this last product is not available worldwide.

P. graveolens and L. cubeba at concentrations used in the present work do not act as potential contact allergens [32] and the other selected oils are not reported to induce cutaneous adverse reactions in contrast with common household cleaning products [33]. These preliminary results seem to be promising for a further application of the EO’s mixture as a suitable tool to inactivate the environmental form of M. canis.

Conflict of interest statement: None declared.


Corresponding author: Simona Nardoni, Dipartimento di Scienze Veterinarie, Università di Pisa, Viale delle Piagge, 2 56100 Pisa, Italy, Fax: +39 050 2210655, E-mail:

References

1. Chermette R, Ferreiro L, Guillot J. Dermatophytoses in animals. Mycopathologia 2008;166:385–405.10.1007/s11046-008-9102-7Suche in Google Scholar PubMed

2. Seebacher C, Bouchara JP, Mignon B. Updates on the epidemiology of dermatophyte infections. Mycopathologia 2008;166:335–2.10.1007/s11046-008-9100-9Suche in Google Scholar PubMed

3. Atzori L, Aste N, Aste N, Pau M. Tinea faciei due to Microsporum canis in children: a survey of 46 cases in the District of Cagliari (Italy). Pediatr Dermatol 2012;29:409–13.10.1111/j.1525-1470.2011.01595.xSuche in Google Scholar PubMed

4. Mancianti F, Nardoni S, Corazza M, D’Achille P, Ponticelli C. Environmental detection of Microsporum canis arthrospores in the households of infected cats and dogs. J Feline Med Surg 2003;11:91–5.10.1016/j.jfms.2008.05.006Suche in Google Scholar PubMed

5. Sparkes AH, Werrett G, Stokes C, Gruffydd-Jones TJ. Microsporum canis: inapparent carriage by cats and the viability of arthrospores. J Small Anim Pract 1994;35:397–401.10.1111/j.1748-5827.1994.tb03861.xSuche in Google Scholar

6. Moriello KA, Hondzo H. Efficacy of disinfectants containing accelerated hydrogen peroxide against conidial arthrospores and isolated infective spores of Microsporum canis and Trichophyton sp. Vet Dermatol 2014;25:191–4.10.1111/vde.12122Suche in Google Scholar PubMed

7. Moriello KA, Kunder D, Hondzo H. Efficacy of eight commercial disinfectants against Microsporum canis and Trichophyton spp. infective spores on an experimentally contaminated textile surface. Vet Dermatol 2013;24:621–3.10.1111/vde.12074Suche in Google Scholar PubMed

8. Deblonde T, Hartemann P. Environmental impact of medical prescriptions: assessing the risks and hazards of persistence, bioaccumulation and toxicity of pharmaceuticals. Public Health 2013;127:312–27.10.1016/j.puhe.2013.01.026Suche in Google Scholar PubMed

9. Vigan M. Essential oils: renewal of interest and toxicity. Eur J Dermatol 2010;20:685–92.Suche in Google Scholar

10. Zuzarte M, Gonçalves MJ, Cavaleiro C, Canhoto J, Vale-Silva L, Silva MJ, et al. Chemical composition and antifungal activity of the essential oils of Lavandula viridis L’Her. J Med Microbiol 2011;60:612–8.10.1099/jmm.0.027748-0Suche in Google Scholar PubMed

11. Mugnaini L, Nardoni S, Pinto L, Pistelli L, Leonardi M, Pisseri F, et al. In vitro and in vivo antifungal activity of some essential oils against feline isolates of Microsporum canis. J Mycol Méd 2012;22:179–84.10.1016/j.mycmed.2012.04.003Suche in Google Scholar PubMed

12. Nardoni S, Mugnaini L, Pistelli L, Leonardi M, Sanna V, Perrucci S, et al. Clinical and mycological evaluation of an herbal antifungal formulation in canine Malassezia dermatitis. J Myc Méd 2014;24:234–40.10.1016/j.mycmed.2014.02.005Suche in Google Scholar PubMed

13. Nguefack J, Letha V, Amvam Zollob PH, Mathur SB. Evaluation of five essential oils from aromatic plants of Cameroon for controlling food spoilage and mycotoxin producing fungi. Int J Food Microbiol 2004;94:329–34.10.1016/j.ijfoodmicro.2004.02.017Suche in Google Scholar PubMed

14. Burt S. Essential oils: their antibacterial properties and potential applications in foods – a review. Int J Food Microbiol 2004;1:223–53.10.1016/j.ijfoodmicro.2004.03.022Suche in Google Scholar PubMed

15. Fisher K, Phillips CA. The effect of lemon, orange and bergamot essential oils and their components on the survival of Campylobacter jejuni, Escherichia coli O157, Listeria monocytogenes, Bacillus cereus and Staphylococcus aureus in vitro and in food systems. J Appl Microbiol 2006;101:1232–40.10.1111/j.1365-2672.2006.03035.xSuche in Google Scholar PubMed

16. Moussaieff A, Mechoulam R. Boswellia resin: from religious ceremonies to medical uses; a review of in-vitro, in-vivo and clinical trials. J Pharm Pharmacol 2009;61:1281–93.10.1211/jpp/61.10.0003Suche in Google Scholar PubMed

17. Huang Y, Zhao J, Zhou L, Wang J, Gong Y, Chen X, et al. Antifungal activity of the essential oil of Illicium verum fruit and its main component trans-anethole. Molecules 2010;15:7558–69.10.3390/molecules15117558Suche in Google Scholar PubMed PubMed Central

18. Wang H, Liu Y. Chemical composition and antibacterial activity of essential oils from different parts of Litsea cubeba. Chem Biodivers 2010;7:229–35.10.1002/cbdv.200800349Suche in Google Scholar PubMed

19. Wang GW, Hu WT, Huang BK, Qin LP. Illicium verum: a review on its botany, traditional use, chemistry and pharmacology. J Ethnopharmacol 2011;136:10–20.10.1016/j.jep.2011.04.051Suche in Google Scholar PubMed

20. Khan UA, Rahman H, Niaz Z, Qasim M, Khan J, Tayyaba RB, et al. Antibacterial activity of some medicinal plants against selected human pathogenic bacteria. Eur J Microbiol Immunol 2013;3:272–4.10.1556/EuJMI.3.2013.4.6Suche in Google Scholar PubMed PubMed Central

21. Pistelli L, Mancianti F, Bertoli A, Cioni PL, Leonardi M, Pisseri F, et al. Antimycotic activity of some aromatic plants essential oils against canine isolates of Malassezia pachydermatis: an in vitro assay. Open Mycol J 2012;6:17–21.10.2174/1874437001206010017Suche in Google Scholar

22. National Institute of Standards and Technology. NIST/EPA/NIH Mass Spectral Library, Version 1.7. Norwalk: Perkin Elmer, 1999.Suche in Google Scholar

23. Adams RP. Identification of essential oils by capillary gas chromatography/mass spectroscopy. Carol Stream, IL, USA: Allured Publishing, 2013.Suche in Google Scholar

24. Shin S, Lim S. Antifungal effects of herbal essential oils alone and in combination with ketoconazole against Trichophyton spp. J Appl Microbiol 2004;97:1289–96.10.1111/j.1365-2672.2004.02417.xSuche in Google Scholar PubMed

25. Gogoi P, Baruah P, Nath SC. Antifungal activity of the essential oil of Litsea cubeba. Pers J Ess Oil Res 1997;9:213–15.10.1080/10412905.1997.9699462Suche in Google Scholar

26. Aminifad M, Mohammadi S. Essential oils to control Botrytis cinerea in vitro and in vivo on plum fruits. J Sci Food Agric 2013;93:348–53.10.1002/jsfa.5765Suche in Google Scholar PubMed

27. Bouzenna H, Krichen L. Pelargonium graveolens L’Her. and Artemisia arborescens L. essential oils: chemical composition, antifungal activity against Rhizoctonia solani and insecticidal activity against Rhysopertha dominica. Nat Prod Res 2013;27:841–6.10.1080/14786419.2012.711325Suche in Google Scholar PubMed

28. De M, De AK, Sen P, Banerjee AB. Antimicrobial properties of star anise (Illicium verum Hook f). Phytother Res 2002;16:94–5.10.1002/ptr.989Suche in Google Scholar PubMed

29. Angioni A, Barra A, Coroneo V, Dessi S, Cabras P. Chemical composition, seasonal variability, and antifungal activity of Lavandula stoechas L. ssp. stoechas essential oils from stem/leaves and flowers. J Agric Food Chem 2006;54:4364–70.10.1021/jf0603329Suche in Google Scholar PubMed

30. Zore GB, Thakre AD, Rathod V, Karuppayil SM. Evaluation of anti-Candida potential of geranium oil constituents against clinical isolates of Candida albicans differentially sensitive to fluconazole: inhibition of growth, dimorphism and sensitization. Mycoses 2011;54:e99–109.10.1111/j.1439-0507.2009.01852.xSuche in Google Scholar PubMed

31. Luo M, Jiang LK, Huang YX, Xiao M, Li B, Zou GL, et al. Effects of citral on Aspergillus flavus spores by quasi-elastic light scattering and multiplex microanalysis techniques. Acta Biochim Biophys Sin (Shanghai) 2004;36:277–83.10.1093/abbs/36.4.277Suche in Google Scholar PubMed

32. Lalko J, Api AM. Investigation of the dermal sensitization potential of various essential oils in the local lymph node assay. Food Chem Toxicol 2006;44:739–46.10.1016/j.fct.2005.10.006Suche in Google Scholar PubMed

33. Magnano M, Salvani S, Vincenzi C, Nino M, Tosti A. Contact allergens and irritants in household washing and cleaning products. Contact Dermatitis 2009;61:337–41.10.1111/j.1600-0536.2009.01647.xSuche in Google Scholar PubMed

Received: 2014-6-6
Revised: 2015-1-22
Accepted: 2015-1-30
Published Online: 2015-2-26
Published in Print: 2015-1-1

©2015 by De Gruyter

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