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  • Review
  • Open Access

A review on biosynthesis of silver nanoparticles and their biocidal properties

  • 1,
  • 2Email author and
  • 3
Journal of Nanobiotechnology201816:14

https://doi.org/10.1186/s12951-018-0334-5

  • Received: 6 September 2017
  • Accepted: 19 January 2018
  • Published:

Abstract

Use of silver and silver salts is as old as human civilization but the fabrication of silver nanoparticles (Ag NPs) has only recently been recognized. They have been specifically used in agriculture and medicine as antibacterial, antifungal and antioxidants. It has been demonstrated that Ag NPs arrest the growth and multiplication of many bacteria such as Bacillus cereus, Staphylococcus aureus, Citrobacter koseri, Salmonella typhii, Pseudomonas aeruginosa, Escherichia coli, Klebsiella pneumonia, Vibrio parahaemolyticus and fungus Candida albicans by binding Ag/Ag+ with the biomolecules present in the microbial cells. It has been suggested that Ag NPs produce reactive oxygen species and free radicals which cause apoptosis leading to cell death preventing their replication. Since Ag NPs are smaller than the microorganisms, they diffuse into cell and rupture the cell wall which has been shown from SEM and TEM images of the suspension containing nanoparticles and pathogens. It has also been shown that smaller nanoparticles are more toxic than the bigger ones. Ag NPs are also used in packaging to prevent damage of food products by pathogens. The toxicity of Ag NPs is dependent on the size, concentration, pH of the medium and exposure time to pathogens.

Keywords

  • Silver nanoparticles
  • Antimicrobial activity
  • Antioxidant activity
  • Green synthesis
  • Toxicity mechanism

Introduction

Nanoparticles exhibit novel properties which depend on their size, shape and morphology which enable them to interact with plants, animals and microbes [17]. Silver nanoparticles (Ag NPs) have shown excellent bactericidal properties against a wide range of microorganisms [811]. They are prepared from different perspectives, often to study their morphology or physical characteristics. Some authors have used chemical method [12] and mistaken it with green synthesis, although they have done it inadvertently. The Ag NPs and their application in electronics, catalysis, drugs and in controlling microorganism development in biological system have made them eco-friendly [1, 8, 9, 13]. Biogenic synthesis of Ag NPs involves bacteria, fungi, yeast, actinomycetes and plant extracts [1, 10, 11, 1315]. Recently, a number of parts of plants such as flowers, leaves and fruits [1], besides enzymes, have been used for the synthesis of gold and silver nanoparticles. The size, morphology and stability of nanoparticles depend on the method of preparation, nature of solvent, concentration, strength of reducing agent and temperature [1, 6, 10, 11].

Of all the nanoparticles developed and characterized thus far, Ag NPs assume a significant position owing to their inherent characteristic of acting as an antimicrobial agent even in solid state. Although, its significance was recognized much earlier, it was not well exploited except for its use in oriental medicine and in coins. It is estimated that nearly 320 tons of Ag NPs are manufactured every year and used in nanomedical imaging, biosensing and food products [16, 17].

There is a continuous increase in the number of multi-drug resistant bacterial and viral strains due to mutation, pollution and changing environmental conditions. To circumvent this predicament scientists are trying to develop drugs for the treatment of such microbial infections. Many metal salts and metal nanoparticles have been found to be effective in inhibiting the growth of many infectious bacteria. Silver and Ag NPs occupy a prominent place in the series of such metals which are used as antimicrobial agents from time immemorial [18, 19]. Silver salts are used to inhibit the growth of a variety of bacteria in human system. They are used in catheters, cuts, burns and wounds to protect them against infection [20, 21]. Das et al. [22] have reported that small sized Ag NPs are excellent growth inhibitors of certain bacteria. Ag NPs synthesized from silk sericin (SS), a water-soluble protein extracted from silk worms at pH 11, contain hydrophilic proteins with highly polar groups like hydroxyl, carboxyl and amino functional groups. Molecules containing the above functional groups act as reducing agents for AgNO3 to produce elemental silver. Aramwit et al. [23] have suggested that the hydroxyl groups of SS are supposed to form complex with silver ions and prevent their aggregation or precipitation [24, 25]. Ag NPs in elemental state may be segregated due to large molecules present in the solvent but may not be complexed as both of them are neutral. The antibacterial activity of SS-capped Ag NPs against gram positive and gram negative bacteria has been screened. It was found that MIC falls between 0.001 and 0.008 mM for both types of microorganisms namely Staphylococcus aureus, Bacillus subtilis, Pseudomonas aeruginosa, Acinetobacter baumannii and Escherichia coli.

Although, several reviews have been published on the fabrication and characterization of silver nanoparticles, very limited reports are available on their green synthesis, biocidal properties and mechanism of action [8, 9, 13, 16, 23]. Thus, in this review, we have attempted to give a comprehensive detail of the biosynthesis of Ag NPs from herbal extracts, fungi and bacteria. Their potential as antimicrobial agent and the mechanism of their action has also been discussed.

Synthesis and characterization of silver nanoparticles

In general, metallic nanoparticles are produced by two methods, i.e. “bottom-up” (buildup of a material from the bottom: atom by atom, molecule by molecule or cluster by cluster) and “top-down” (slicing or successive cutting of a bulk material to get nano-sized particle) [1]. The “bottom-up” approach is usually a superior choice for the nanoparticles preparation involving a homogeneous system wherein catalysts (for instance, reducing agent and enzymes) synthesize nanostructures that are controlled by the catalyst itself. However, the “top-down” approach generally works with the material in its bulk form, and the size reduction to nanoscale is achieved by specialized ablations, for instance thermal decomposition, mechanical grinding, etching, cutting, and sputtering. The main demerit of the top-down approach is the surface structural defects. Such defects have significant impact on the physical features and surface chemistry of metallic nanoparticles. Several methodologies are available for the synthesis of Ag NPs namely, chemical methods [2629]; physical methods [3032] and biological methods [1, 10, 11]. Chemical method of synthesis can be subdivided into chemical reduction, electrochemical, irradiation-assisted chemical and pyrolysis methods [33]. Ag NPs synthesis in solution requires metal precursor, reducing agents and stabilizing or capping agent. Commonly used reducing agents are ascorbic acid, alcohol, borohydride, sodium citrate and hydrazine compounds. Sotiriou and Pratsinis [28] have shown that the Ag NPs supported on nanostructured SiO2 were obtained by flame aerosol technology, which allows close control of silver content and size. Also, silver/silica nanoparticles with relatively narrow size distribution were obtained by flame spray pyrolysis [29]. However, physical methods do not require lethal and highly reactive chemicals and generally have a fast processing time. These methods include arc-discharge [31], physical vapor condensation [30], energy ball milling method [34] and direct current magnetron sputtering [32]. Physical methods have another advantage over chemical methods in that the Ag NPs have a narrow size distribution [32], while the main demerits are consumption of high energy [32]. Thus, biological synthesis of Ag NPs from herbal extract and/or microorganisms has appeared as an alternative approach as these routes have several advantages over the chemical and physical methods of synthesis. It is also a well-established fact that these routes are simple, cost-effective, eco-friendly and easily scaled up for high yields and or production [13]. Biosynthesis of metal and metal oxide nanoparticles using biological agents such as bacteria, fungi, yeast, plant and algal extracts has gained popularity in the area of nanotechnology [13, 5, 6, 10, 11].

Plants and their parts contain carbohydrates, fats, proteins, nucleic acids, pigments and several types of secondary metabolites which act as reducing agents to produce nanoparticles from metal salts without producing any toxic by-product. The details have been provided in Table 1. Similarly, biomolecules such as enzymes, proteins and bio-surfactants present in microorganisms serve as reducing agents. For instance, in many bacterial strains, bio-surfactants are used as capping and/or stabilizing agents (Table 2).
Table 1

Plant-mediated synthesis of silver nanoparticles

Plant

Plant part

Size and shape

Phytoconstituents responsible for reduction of silver nitrate

Key references

Aloe vera

Leaf gel (removed skin)

5–50 nm; octahedron

Flavanones and terpenoids

Logaranjan et al. [35]

Leaf

70.7–192.02 nm; spherical (size varies through change of times and temperatures)

Lignin, hemicellulose and pectins

Tippayawat et al. [36]

Leaf

Size varies in accordance to different parameters; spherical

Flavonoids, terpenoids and phenols

Moosa et al. [37]

Mangifera indica

Seed

14 nm; spherical and hexagonal

Phenolic compounds, gallotannins and tannin

Sreekanth et al. [38]

Erigeron bonariensis

Leaf

13 nm; spherical

Flavonoids, steroids, glycosides, triterpenes, sugars and caffeoyl derivatives

Kumar et al. [39]

Myristica fragrans

Bark and seeds

Spherical, polydispersed

Secondary metabolites

Jelin et al. [40]

Momordica charantia

Leaf

11 nm; spherical

Momorcharins, momordenol, momordicius, momordin, momordolo, charantin, charine, cucuritanes, cucurbitns, goyaglycosides and goyasaponins

Ajitha et al. [41]

Carambola

Fruit

16, 13, 12 nm at pH 4, 7, 10 respectively

Polysaccharides, polyols and ascorbic acid

Chowdhury et al. [42]

Rubus glaucus

Fruit

12–50 nm; spherical

Phenolic groups and flavonoids

Kumar et al. [43]

Prunus serotina

Fruit

20–80 nm (blue LED) 40–100 nm (white solar); spherical

Chlorogenic acid, catechin, proanthocyanidin, and flavonol glycosides

Kumar et al. [44]

Piper nigrum

Seeds

10–60 nm; rod shaped

Polysaccharides, amino acids, alkaloids, proteins and vitamins

Mohapatra et al. [45]

Nigella sativa

Leaf

15 nm; spherical

Alkaloids, ascorbic acid, saponins, glycosides, amino acids, flavonoids like catechin, apigenin, gallic acid and benzoates especially vanillic acid

Amooaghaie et al. [46]

Calotropis gigantean

Flower

10–50 nm; spherical

Pavani et al. [47]

Acmella oleracea

Flower

2–20 nm; spherical

Raj et al. [48]

Piper betle

Leaf

48–83 nm; spherical

Allylic benzenes, phenolic, amino acids, proteins, alcoholic compounds, terpenes and terpenoids

Kamachandran et al. [49]

Morinda tinctoria

Leaf

80–100 nm; spherical and rod

Ascorbic acid, niacin, copper and iron

Vennila and Prabha [50]

Trigonella foenum-graecum

Seeds

20–50 nm; spherical

Saponins and alkaloids

Meena and Chouhan [51]

Picrasma quassioides

Bark

17.5–66.5 nm; spherical

Sreekanth et al. [52]

Rosa ‘Andeli’

Petals

0.5–1.4 nm; spherical

Polyphenols and flavonoids

Suarez-Cerda et al. [53]

Salvadora persica

Stem

1–6 nm; spherical

Phenolic compounds

Tahir et al. [54]

Artemisia absinthium

 

5–20 nm; round shaped

Phenolic compounds and flavonoids

Ali et al. [55]

Chelidonium majus

Aerial parts

DLS-253.3 nm; spherical, quasi-spherical

Flavonoids and alkaloids

Barbinta-Patrascu et al. [56]

Calotropis procera

Flower

35 nm; face centered cubic

Tannins, triterpenes, flavonoids, steroids, alkaloids and cardiac glycosides

Babu and Prabu [57]

Sterculia acuminata

Fruit

~ 10 nm; spherical

Ascorbic acid, gallic acid, phenolic compounds, pyrogallol, methyl gallate and polyphenolic compounds

Bogireddy et al. [58]

Terminalia cuneata

Bark

25–50 nm; spherical

Tannins, saponins, triterpenoids, flavonoids, gallic acid, ellagic acid and phytosterols

Edison et al. [59]

Cirsium japonicum

Plant

4–8 nm; spherical

Saponins, proteins and flavonoids

Khan et al. [60]

Isatis tinctoria

Plant

10–15 nm; spherical

Saponins and flavonoids

Ahmad et al. [61]

Aegle marmelos

Fruit

22.5 nm; spherical, hexagonal, roughly circular

Phytosterols, flavonoids, alkaloids, triterpenoids and amino acids

Velmurugan et al. [62]

Trachyspermum ammi

Seeds

36 nm; cubic

Fatty acids, proteins, flavonoids and alkaloids

Chouhanand Meena [63]

Eucalyptus globulus

Leaf

1.9–4.3 and 5–25 nm with and without microwave treatment respectively

Alkaloids and flavonoids

Ali et al. [64]

Cydonia oblonga

Seeds

38 nm; face-centered cubic

Flavonones, terpenoids, proteins and amino acids

Zia et al. [65]

Hydrocotyle asiatica

Leaf

21 nm; spherical

Flavonoids and glycosides

Devi et al. [66]

Lantana camara

Leaf

33.8 nm; spherical

Flavonoids, proteins, saccharides secondary metabolites like alkaloids, tannins, saponins, carbohydrates, steroids and triterpenoids

Manjamadha and Muthukumar [67]

Nyctanthes arbor-tristis

Seeds

50–80 nm; spherical

Carbohydrates and phenolic compounds

Basu et al. [68]

Pennyroyal sp.

Leaf

19.14 ± 9.791 nm; spherical

Sedaghat et al. [69]

Saraca indica

Leaf

23 ± 2 nm; spherical

Flavonoids and steroids

Perugu et al. [70]

Terminalia chebula

Fruit

30 nm; distorted spherical

Edison et al. [71]

Euphorbia amygdaloides

Plant

7–20 nm; spherical

Cicek et al. [72]

Pedalium murex

Leaf

50 nm; spherical

Flavonoids, alkaloids, steroids, rosins, saponins and proteins

Anandalakshmi et al. [73]

Chelidonium majus

Root

15.42 nm; spherical

Alishah et al. [74]

Salacia chinensis

Powdered plant

20–80 nm; spherical, rods, triangular, hexagonal

Flavonoids, saponins, proteins, carbohydrates and phenolics

Jadhav et al. [75]

Tamarindus indica

Seed coat

~ 12.73 nm

Flavonoids, tannin and saponins,

Ramamurthi et al. [76]

Parkia roxburghii

Leaf

5–25 nm; poly dispersped, quasi-spherical

Proteins

Paul et al. [77]

Aristolochia indica

Leaf

32–55 nm; spherical

Shanmugam et al. [78]

Cerasus serrulata

Leaf

10–50 nm; spherical

Alcohol and phenolic compounds and proteins

Karthik et al. [79]

Matricaria camomilia

Flower

8–35 nm; spherical

Terpenoids, flavones and polysaccharides

Parlinska-Wojtan et al. [80]

Flower

~ 5.5 nm; spherical

Phenolics, carbonyl and amines or alcohol groups

Ocsoy et al. [81]

Fruits

~ 15.4 nm; spherical

Phenolics, flavonoids, terpenoids and vitamins

Swamy et al. [82]

Alpinia calcarata

Root

5–15 nm; quasi-spherical

Proteins, flavonoids and polyphenols

Pugazhendhi et al. [83]

Salvinia molesta

Leaf

12.46 nm; spherical

Alkaloids, flavonoids, tannins, phenols, sugars and proteins

Verma et al. [84]

Helicteres isora

Root

16–95 nm; spherical

Steroids, terpenoids, alkaloids, carbohydrates and phenolic compounds

Bhakya et al. [85]

Mukia maderaspatana

Leaf

158 nm; spherical

Phenolic compounds

Harshiny et al. [86]

Ficus benghalensis and Azadirachta indica

Bark

60 nm; spherical

Flavonoids, terpenoids and phenols

Nayak et al. [87]

Azadirachta indica

Leaf

34 nm; spherical and irregular shape

Flavanoids and terpenoids

Ahmed et al. [88]

Adathoda vasica

Leaf

10–50 nm; spherical

Alkaloids compounds

Latha et al. [89]

Amaranthus gangeticus

Leaf

11–15 nm; globular and polycrystalline

Amino acids

Kolya et al. [90]

Phlomis

Leaf

25 nm; spherical

Glycosides such as flavonoids, iridoids, diterpenoids, triterpenoids and other phenolic compounds

Allafchian et al. [91]

Syzygium alternifolium

Fruit

4–48 nm; spherical

Phenols and primary amines of proteins

Yugandhar et al. [92]

Afzelia quanzensis

Bark

10–80 nm; spherical

Proteins

Moyo et al. [93]

Allamanda cathartica

Flower

39 nm; spherical

(E,E)-geranyl linalool, n-pentacosane, 1,8-cineole and n-tricosane

Karunakaran et al. [94]

Carica papaya

Peel

10–30 nm; spherical

Vitamins (C, K, E), amino acids, carbohydrates, β-carotene, lycopene and polyphenols

Kokila et al. [95]

Vitis vinifera

Leaf

200 nm; spherical

Hydroxyl groups and phenolic compounds mainly myricetin, ellagic acid, kaempferol and gallic acid

El-Sherbiny et al. [96]

Solanum indicum

Leaf

10–50 nm; spherical

Phenolic compounds

Sengottaiyan et al. [97]

Tectona grandis

Leaf

26–28 nm; spherical

Phenols

Devadiga et al. [98]

Soymida febrifuga

Leaf

10–20 nm; spherical

Phenolic groups, amino acids, aliphatic and aromatic amines, amide-I and amide-II

Sowmyyan and Lakshmi [99]

Cardiospermum halicacabum

Leaf

SEM-less than 100 nm; spherical

Polyphenols and phenol

Sundararajan et al. [100]

Ammannia baccifera

 

105–125 nm; spherical

Polyphenols, flavonoids and proteins

Jadhav et al. [101]

Diospyros paniculata

Root

17 nm (avg); spherical

Phenolics and proteins

Rao et al. [102]

Simarouba glauca

Leaf

33–50 nm; spherical

Amino groups and hydroxyl groups

Kanchana and Zantye [103]

Origanum majorana and Citrus sinensis

Leaf

40–70 nm; feather and 26–60 nm; spherical, cubical respectively

Proteins and phenolic compounds

Singh et al. [104]

Salmalia malabarica

Gum

7 ± 2 nm; spherical

Carbonyl and hydroxyl group

Krishna et al. [105]

Psidium guajava

Leaf

10–90 nm; spherical

Leucocyanidin, flavonoids, tannins, saponins, carotenes, vitamin C, B6 and carbohydrates

Bose and Chatterjee [106]

Allium cepa

Bulb

Balamanikandan et al. [107]

Justicia glauca

Leaf

10–20 nm; spherical

Phenolic compounds

Awad et al. [108]

Skimmia laureola

Leaf

Irregular, spherical, hexagonal

Tritepenoids, skimmidiol and coumarins

Ahmed et al. [109]

Andrographis echioides

Leaf

~ 68.06 nm; cubic

Carbohydrates, tannins, saponins, flavonoids, alkaloids, quinones, glycosides, triterpenoids, phenols, steroids, phytosteroids and anthraquinones

Elangovan et al. [110]

Putranjiva roxburghii

Leaf

5.74 nm; spherical

Amino groups

Ali et al. [111]

Ixora coccinea

Flower

5–10 nm; spherical

Alkaloids, tannins, glycosides, flavonoids, saponins, terpenes and carbohydrates

Nalvolthula et al. [112]

Emblica officinalis

Fruit

10–70 nm; spherical

Alkaloids, phenolic compounds, amino acids and tannins

Ramesh et al. [113]

Hibiscus rosa-sinensis

Petals

~ 18.79 nm; spherical

Proteins

Nayak et al. [114]

Bauhinia variegata

Leaf

32 nm; spherical, triangular, truncated triangles, decahedral

Reducing sugar, saponins, anthraquinone, alkaloids and terpenoids

Govindarajan et al. [115]

Pteridium aquilinum

Leaf

SEM-35–65 nm; spherical

Phenols, alkaloids, tannins, flavonoids, proteins, carbohydrates, saponins. glycosides, steroids and triterpenoids

Panneerselvam et al. [116]

Aristolochia indica

Leaf

30–55 nm; spherical and cubical

Phenols

Murugan et al. [117]

Cassia roxburghii

Leaf

~ 32 nm; spherical, triangular, truncated triangles, decahedral

Muthukumaran et al. [118]

Anisomeles indica

Leaf

TEM-18–35 nm; SEM-50–100 nm; spherical

Alcohols, phenols and carboxylic group

Govindarajan et al. [119]

Hybanthus enneaspermus

Plant

16–26 nm; spherical, hexagonal, triangular

Proteins

Suman et al. [120]

Amaranthus dubius

Leaf, stem, root

Stem: 30–35 nm; Root: 18–21 nm; Leaf: 18–21 nm

Polyphenol compounds and aldehydes

Sigamioney et al. [121]

Ziziphus jujuba

Fruit

25.75 nm; spherical

Alcohols and phenols

Sreekanth et al. [122]

Chrysophyllum oliviforme

Leaf

25 nm; flower

Flavonoids, saponins, catechic tannins, traces of anthraquinones, reducing sugars and phenolic compounds

Varghese et al. [123]

Plumeria alba

Flowers

~ 36.19 nm; spherical

Amino, carboxylic and sulfhydryls

Mata et al. [124]

Impatiens balsamina

Flowers

5–40 nm; spherical

Alkaloids, tannins, glycosides, flavonoids, saponins, terpenes and carbohydrates

Nalavothula et al. [125]

Fraxinus excelsior

Leaf

25–40 nm; spherical and polydisperse

Flavonoids, alkaloids, glycosides, terpenoids, phenolic compounds, amino acid residues and peptides of proteins

Parveen et al. [126]

Pongamia pinnata

Leaf

AFM-15–35 nm; spherical

Alkaloids, glycosides, flavonoids, saponins, carbohydrates, tannins, phenolic compounds and fat

Priya et al. [127]

Pongamia pinnata

Seed

5–30 nm; spherical

Pongaflavanol, tunicatachalcone, pongamol, galactoside and glybanchalcone

Beg et al. [128]

Areca catechu

Nut

18.2 and 24.3 nm; spherical

Polyphenols

Rajan et al. [129]

Ficus talboti

Leaf

9–12 nm; spherical

Flavonoids, alkaloids, saponins, phenolic compounds, tannins, phytosterol and glycosides

Arunachalam et al. [130]

Sida cordifolia

Leaf

10–30 nm; spherical, prism

Alkaloids, quinazolines, cryptoleptins, phytosterols, flavonoids and saponins

Srinithya et al. [131]

Clerodendrum phlomidis

Leaf

TEM 10–15 nm; SEM 23–42 nm; spherical

Phenolics, flavonoids, terpenoids and steroids

Sriranjani et al. [132]

Theobroma cacao

Pod husk

4–32 nm; face-centered cubic

Proteins and phenolic compounds

Lateef et al. [133]

Ficus carica

Fruit

20–80 nm (thermal approach), 10–30 nm (ultra sonication approach); spherical

Kumar et al. [134]

Parkia speciosa Hassk

Pod

20–50 nm; predominantly spherical

Fatimah [135]

Boerhaavia diffusa

Whole plants

25 nm; spherical

 

Vijay Kumar et al. [136]

Pelargonium endlicherianum

Roots

Different size; spherical

Gallic acid, apocynin and quercetin

Karatoprak et al. [137]

Artocarpus heterophyllus

Seeds

10.78 nm; irregular

Lectin—a single major protein

Jagtap and Bapat [138]

Ceropegia thwaitesii

Leaf

100 nm; spherical

Triterpenoids; and methoxy groups of protein

Muthukrishnan et al. [139]

Alternanthera sessilis

Leaf

30 nm; various shape

Alkaloid, tannins, ascorbic acid, carbohydrates and proteins

Niraimathi et al. [140]

Dryopteris crassirhizoma

Rhizome

5–60 nm; almost spherical

Alcohol, amines, alkanes, carboxylic acid and or ester

Lee et al. [141]

Leptadenia reticulate

Leaf

50–70 nm; crystalline, face centered and spherical

Phenolics, terpenoids, polysaccharides and flavones

Swamy et al. [142]

Ipomoea batatas

Root

TEM 30–120 nm; AFM 50–200 nm; polygonal

Glycoalkaloids, mucin, dioscin, choline, polyphenols and anthocyanins

Wang et al. [143]

Sambucus nigra

Fruit

26 nm; spherical

Polyphenols

Moldovan et al. [144]

Millettia pinnata

Flower

16–38 nm; spherical

Multi-functional aromatic gropus

Rajakumar et al. [145]

Coptis chinensis

Plant extract

15 nm; spherical

Polyphenols

Ahmad et al. [146]

Lycium barbarum

Fruit

3–15 nm; spherical

Tannias, flavanoids, ascorbic acid and alkaloids

Dong et al. [147]

Embelia ribes

Seed

20–30 nm; crystalline, uniform and spherical

Alkaloids, quinones, proteins, reducing sugars and saponins

Dhayalan et al. [148]

 Zizyphus xylopyrus

Bark

60–70 nm; spherical

Reducing agents

Maria et al. [149]

Table 2

Bio-surfactants and or stabilizing agents used during synthesis of silver nanoparticles from various bacterial stains

Bacteria

Size and shape

Biosurfactants and or stabilizing agent

Key references

Pseudomonas aeruginosa BS-161R

15.1 ± 5.8 nm; spherical

Rhamnolipids

Kumar et al. [150]

Brevibacterium casei MSA19

Biosurfactant

Kiran et al. [151]

Bacillus cereus NK1

50–80 nm; spherical

URAK (a fibrinolytic enzyme)

Deepak et al. [152]

Gluconacetobacter xylinum

5–40 nm

Cellulose

Liu et al. [153]

Streptomyces coelicolor

28–50 nm; irregular

Actinorhodin pigment

Manikprabhu and Lingappa [154]

Bacillus subtilis MSBN 17

60; spherical

Bioflocculant

Sathiyanarayanan et al. [155]

Salmonella typhimurium

3–11 nm

Flagellin

Gopinathan et al. [156]

Bacillus athrophaeus

5–30 nm; polydispersed

Spores

Hosseini-Abari et al. [157]

Lactobacillus rhamnosus GG ATCC 53103

2–15 nm; spherical, triangular, rod-shaped and hexagonal

Exopolysaccharide

Kanmani and Lim [158]

Nostoc commune

15–54 nm; spherical

Extracellular polysaccharide/matrix

Morsy et al. [159]

Pseudomonas aeruginosa

1.13 nm; spherical

Biosurfactant

Farias et al. [160]

Ochrobactrum rhizosphaerae

10 nm; spherical

Glycolipoprotein

Gahlawat et al. [161]

Gordonia amicalis HS-11

5–25 nm; spherical

Glycolipid

Sowani et al. [162]

Bacillus subtilis

Surfactin

Mendrek et al. [163]

Extracellular synthesis of Ag NPs comprises of the trapping of metal ions on the outer surface of the cells and reducing them in the presence of enzymes or biomolecules, while intracellular synthesis occurs inside the microbial cells. It has been suggested that the extracellular synthesis of nanoparticles is cheap, favors large-scale production and requires simpler downstream processing. Thus, the extracellular method for the synthesis of nanoparticles is preferable [164] in comparison to the intracellular method. Ganesh Babu and Gunasekaran [165] and Kalimuthu et al. [166] have demonstrated that the intracellular synthesis requires additional steps for instance, ultrasound treatment or reactions with suitable detergents to release the synthesized silver nanoparticles. Further, the rate of biosynthesis of Ag NPs and their stability is a significant part in industrial production. Therefore, a proper monitoring of reaction conditions is also important (Fig. 1).
Fig. 1
Fig. 1

Biosynthesis of silver nanoparticles and their optimization techniques

From bacteria

In recent years, the potential of biosynthesis of Ag NPs using bacteria has been realized [15, 153, 156159]. For instance, Pseudomonas stutzeri AG259—isolated from silver mine was used to produce Ag NPs inside the cells [167]. In addition, several bacterial strains (gram negative as well as gram positive) namely A. calcoaceticus, B. amyloliquefaciens, B. flexus, B. megaterium and S. aureus have been used for both extra- and intracellular biosynthesis of Ag NPs [168174]. These Ag NPs are spherical, disk, cuboidal, hexagonal and triangular in shape. They have been fabricated using culture supernatant, aqueous cell-free extract or cells (Table 3). Saifuddin et al. [14] have demonstrated an extracellular biosynthesis of Ag NPs ( 5–50 nm) using a combination of culture supernatant of B. subtilis and microwave irradiation in water. Shahverdi et al. [15] have reported rapid biosynthesis of Ag NPs (within 5 min) using the culture supernatants of K. pneumonia, E. coli and Enterobacter cloacae. Saravanan et al. [172] have also reported an extracellular synthesis of Ag NPs using B. megaterium cultured supernatant, within minutes in presence of aqueous solutions of Ag+ ions.
Table 3

Bacteria-mediated synthesis of silver nanoparticles

Bacteria

Size and shape

Location

Key references

Acinetobacter calcoaceticus

8–12 nm; spherical

Extracellular

Singh et al. [175]

A. haemolyticus MMC8

4–40 nm

Extracellular

Gaidhani et al. [176]

Aeromonas sp. SH10

6.4 nm

Extracellular and intracellular

Mouxing et al. [177]

Wang et al. [178]

Bordetella sp.

63–90 nm

Extracellular

Thomas et al. [179]

Enterobacter aerogenes

25–35 nm; spherical

Extracellular

Karthik and Radha [180]

Escherichia coli

42.2–89.6 nm; spherical

Extracellular

Gurunathan et al. [181]

Geobacter sulfurreducens

 

Extracellular

Law et al. [182]

Gluconobacter roseus

10 nm

Extracellular

Krishnaraj and Berchmans [183]

Idiomarina sp.

25 nm

Intracellular

Seshadri et al. [184]

Klebsiella pneumoniae

15–37 nm; spherical

Extracellular

Duraisamy and Yang [185]

5–32 nm

Extracellular

Shahverdi et al. [15]

Morganella sp.

10–40 nm; quasispherical

Extracellular

Parikh et al. [186]

Proteus mirabilis

10–20 nm; spherical

Extracellular and intracellular

Samadi et al. [187]

Pseudomonas aeruginosa SM1

6.3 ± 4.9 nm; spherical, disk-shaped

Extracellular

Srivastava and Constanti [188]

8–24 nm; spherical

Extracellular

Kumar and Mamidyala [189]

5–25 nm; quasispherical

Intracellular

Otaqsara [190]

Rhodobacter sphaeroides

Spherical 3–15

Extracellular

Bai et al. [191]

Rhodopseudomonas palustris

Spherical 5–20

Extracellular

Chun-Jing and Hong-Juan [192]

Shewanella oneidensis MR-1

2–16 nm; spherical (Ag2S)

Extracellular

Debabov et al. [193]

Stenotrophomonas maltophilia

93 nm; cuboidal

Extracellular

Oves et al. [194]

Vibrio alginolyticus

50–100 nm; Spherical

Extracellular and intracellular

Rajeshkumar et al. [195]

Xanthomonas oryzae

14.86 nm; spherical, triangular,

rod-shaped

Extracellular

Narayanan and Sakthivel [196]

Yersinia enterocolitica

10–80 nm

Extracellular

Pourali et al. [197]

Bacillus sp.

5–15 nm

Extracellular and periplasmic space

Pugazhenthiran et al. [198]

B. cereus

4–5 nm; spherical

Intracellular

Ganesh Babu and Gunasekaran [165]

B. flexus

12 and 65 nm; spherical and triangular

Extracellular

Priyadarshini et al. [173]

B. licheniformis Dahb1

18.69–63.42 nm; spherical

Cell free extract

Shanthi et al. [199]

B. safensis LAU 13

5–30 nm; spherical

Extracellular

Lateef et al. [200]

B. methylotrophicus DC3

10–30 nm; spherical

Wang et al. [201]

B. subtilis

Triangular, hexagonal

Extracellular

Kannan et al. [202]

B. subtilis MTCC 3053

20–60 nm; polydispersed(AgCl)

Paulkumar et al. [203]

B. thuringiensis

43.52–142.97 nm

Extracellular

Banu et al. [204]

Brevibacterium casei

10–50 nm; spherical

Intracellular

Kalishwaralal et al. [205]

Corynebacterium SH09

10–15 nm

Extracellular

Zhang et al. [206]

Enterococcus faecalis

10–80 nm

Extracellular

Pourali et al. [197]

Exiguobacterium sp.

5–50 nm; spherical

Extracellular

Tamboli and Lee [207]

Geobacillus stearothermophilus

5–35 nm; spherical

Extracellular

Fayaz et al. [208]

Lactobacillus mindensis

2–20 nm; spherical (Ag2O)

Extracellular

Dhoondia and Chakraborty [209]

Rhodococcus sp.

10–15 nm; spherical

Extracellular

Otari et al. [210]

Staphylococcus epidermidis

10–80 nm

Extracellular

Pourali et al. [197]

Thermoactinomyces sp.

20–40 nm; spherical

Extracellular

Deepa et al. [211]

Ureibacillus thermosphaericus

10–100 nm; spherical

Extracellular

Juibari et al. [212]

Rapid synthesis of Ag NPs has been achieved by the interaction of a bacterial strain S-27, belonging to Bacillus flexus group and 1 mM AgNO3 in aqueous medium [173]. The colourless supernatant solution turned yellow and finally brown. Its UV–vis spectrum exhibited a sharp peak at 420 nm due to the surface plasmon resonance (SPR) of silver nanoparticles. Anisotropic nanoparticles of 12 and 65 nm size were stable in the dark for 5 months at room temperature although their slow degradation cannot be prevented. They were crystalline with a face centered cubic structure. These nanoparticles were found to be effective against multidrug resistant gram positive and gram negative bacteria. The colour intensity and rate of interaction depend on the concentration of the reacting components.

Das et al. [174] have reported extracellular biosynthesis of Ag NPs from the Bacillus strain (CS11). The interaction of 1 mM AgNO3 with the bacteria at room temperature yielded nanoparticles within 24 h which showed a peak at 450 nm in UV–vis spectrum. Their size from TEM analysis was found to range between 42 and 92 nm (Table 3).

From fungi

Biosynthesis of Ag NPs from both pathogenic and nonpathogenic fungi has been investigated extensively [10, 164, 213215] (Table 4). It has been reported that silver ions are reduced extracellularly in the presence of fungi to generate stable Ag NPs in water [214, 216].
Table 4

Fungus-mediated synthesis of silver nanoparticles

Fungus

Size and shape

Location

Key references

Aspergillu flavus

8.92 nm; spherical

Cell wall

Vigneshwaran et al. [217]

A. fumigatus

Extracellular

Bhainsa and D’Souza [218]

A. terreus

1–20 nm; spherical

Extracellular

Li et al. [219]

Cladosporium cladosporioides

10–100 nm

Balaji et al. [220]

Coriolus versicolor

25–75, 444–491 nm; spherical

Extracellular and intracellular

Sanghi and Verma [221]

Fusarium oxysporum

Extracellular

Ahmad et al. [222]

20–50 nm; spherical

Extracellular

Durán et al. [164]

5–50 nm

Senapati et al. [223]

Humicola sp.

5–25 nm; spherical

Extracellular

Syed et al. [224]

Macrophomina phaseolina

5–40 nm; spherical

Cell-free filtrate

Chowdhury et al. [225]

Pediococcus pentosaceus

Extracellular

Shahverdi et al. [15]

Penicillium brevicompactum

58.35 ± 17.88 nm

Shaligram et al. [226]

P. fellutanum

5–25 nm; spherical

Extracellular

Kathiresan et al. [215]

P. nalgiovense AJ12

25 ± 2.8 nm; spherical

Cell-free filtrate

Maliszewska et al. [227]

Phaenerochaete chrysosporium

5–200 nm; pyramidal

Vigneshwaran et al. [228]

Phoma glomerata

60–80 nm; spherical

Birla et al. [229]

Pleurotus ostreatus

< 40 nm; spherical

Al-Bahrani et al. [230]

P. sajor-caju

30.5 ± 4.0 nm; spherical

Extracellular

Vigneshwaran et al. [231]

Trichoderma asperellum

13–18 nm; nanocrystalline

Extracellular

Mukherjee et al. [232]

T. reesei

5–50 nm

Extracellular

Vahabi et al. [233]

T. viride

5–40 nm; spherical

Extracellular

Fayaz et al. [234]

T. viride

2–5 nm; spherical

40–65 nm; rectangular

50–100 nm; penta/hexagonal (Obtained at varying pH, reaction time and temperature of the reaction mixture)

Cell free extract

Kumari et al. [235]

Syed et al. [224] have also reported the extracellular synthesis of Ag NPs from thermophilic fungus Humicola sp. All manipulations were done in aqueous medium at room temperature. Mycelia were suspended in 100 mL of 1 mM AgNO3 solution in an Erlenmeyer flask at 50 °C and the mixture was left in a shaker for 96 h at pH 9 and monitored for any change in colour. The solution showed a change in colour from yellow to brown due to the formation of Ag NPs [222]. It is a simple process for the extracellular synthesis of Ag NPs from Humicola sp. TEM micrograph showed nicely dispersed nanoparticles mainly of spherical shape ranging between 5 and 25 nm. They are crystalline with a face centered cubic structure [236]. IR spectrum of Ag NPs in the suspension showed peaks at 1644 and 1523 cm−1 assigned to amide I and amide II bands of protein corresponding to –C=O and N–H stretches. Owaid et al. [237] have reported the biosynthesis of Ag NPs from yellow exotic oysters mushroom, Pleurotus cornucopiae var. citrinopileatus. The dried basidiocarps were powdered, boiled in water and the supernatant was freeze dried. Different concentrations of hot water extract of this lyophilized powder were mixed with 1 mM AgNO3 at 25 °C and incubated for 24, 48 and 72 h. Change in colour from yellow to yellowish brown exhibited an absorption peak at 420 and 450 nm in UV–vis region which is the characteristic of spherical silver nanoparticles. The width of the absorption peak suggests the polydispersed nature of nanoparticles [221]. IR spectrum of Ag NPs exhibited absorption peaks at 3304, 2200, 2066, 1969, 1636, 1261, 1094 and 611 cm−1 for different groups. Although, authors have indicated the presence of polysaccharide and protein in the mushroom they have ignored their stretching frequencies in the IR spectrum. However, the peak at 3304 has been assigned to υ (OH) of carboxylic acid and those at 2200 and 1969 cm−1 have been attributed to unsaturated aldehydes. The other peaks below 1500 cm−1 are due to unsaturated alkaloids. The field emission scanning electron and high-resolution transmission electron micrograph suggested that the Ag NPs are spherical with average size ranging between 20 and 30 nm.

Very recently, Al-Bahrani et al. [230] reported biogenic synthesis of Ag NPs from tree oyster mushroom Pleurotus ostreatus. Dried aqueous extract of mushroom (1–6 mg/mL) and 1 mM AgNO3 were mixed and incubated in the dark for 6–40 h. The colour change from pale yellow to dark brownish yellow indicated the formation of silver nanoparticles. The UV–vis spectrum showed a sharp and broad absorption band at 420 nm. They are polydispersed nanoparticles of 10–40 nm with an average size of 28 nm. Several fungi namely, Aspergillus flavus, A. fumigates, Fusarium oxysporum, Fusarium acuminatum, F. culmorum, F. solani, Metarhizium anisopliae, Phoma glomerate, Phytophthora infestans, Trichoderma viride, Verticillium sp. have been used for both extra- and intracellular biosynthesis of Ag NPs [10, 164, 216219, 222]. These nanoparticles are of various sizes and shapes (Table 4).

From plants

Plant related parts such as leaves, stems, roots, shoots, flowers, barks, seeds and their metabolites have been successfully used for the efficient biosynthesis [1, 238] of nanoparticles (Fig. 1). Very recently, Beg et al. [128] have reported green synthesis of Ag NPs from seed extract of Pongamia pinnata. The formation of nanoparticles was confirmed by an absorption max at 439 nm. The well dispersed nanoparticles with an average size of 16.4 nm had zeta potential equal to − 23.7 mV which supports dispersion and stability. Interaction of Ag NPs with human serum albumin was investigated and showed negligible change in α helics. In a very recent publication Karatoprak et al. [137] have reported green synthesis of Ag NPs from the medicinal plant extract Pelargonium endlicherianum. The plant containing gallic acid, apocyanin and quercetin act as reducing agents to produce silver nanoparticles. Phytomediated synthesis of spherical Ag NPs from Sambucus nigra fruit extract has been reported by Moldovan et al. [144]. XRD analysis showed them to be crystalline. The in vivo antioxidant activity was investigated against Wistar rats which showed promising activity. It suggests that functionalization of Ag NPs with natural phytochemicals may protect the cell proteins from ROS production. Ag NPs have also been synthesized from aqueous leaf extract of Artocapus altilis. They were moderately antimicrobial and antioxidant. Thalictrum foliolosum root extract mediated Ag NPs synthesis has been confirmed on the basis of the appearance of a sharp peak at 420 nm in UV–vis region of the spectrum [239]. The monodispersed spherical nanoparticle of 15–30 nm had face centered cubic geometry. Shape and size dependent controlled synthesis of Ag NPs from Aloe vera plant extract and their antimicrobial efficiency has been reported by Logaranjan et al. [35]. The UV–vis peak at 420 nm confirmed the formation of silver nanoparticles. After microwave irradiation of the sample, Ag NPs of 5–50 nm with octahedral geometry was obtained. Nearly two to fourfold antibacterial activity of Ag NPs was observed compared to commonly available antibiotic drugs. Biosynthesis of Ag NPs from the aqueous extract of Piper longum fruit extract has been also achieved [240]. The nanoparticles were spherical in shape with an average particle size of 46 nm determined by SEM and dynamic light scattering (DLS) analyser. The polyphenols present in the extract are believed to act as a stabilizer of silver nanoparticles. The fruit extract and the stabilized nanoparticles showed antioxidant properties in vitro. The nanoparticles were found to be more potent against pathogenic bacteria than the flower extract of P. longum. Ag NPs have been fabricated from leaf extract of Ceropegia thwaitesii and formation was confirmed from absorption of SPR at 430 nm. The nanoparticles of nearly 100 nm diameter were crystalline in nature [139]. Plant extract of Ocimum tenuiflorum, Solanum tricobatum, Syzygium cumini, Centella asiatica and Citrus sinensis have been used to synthesize Ag NPs of different sizes in colloidal form [249]. The size of all nanoparticles was found to be 22–65 nm. They were all stable and well dispersed in solution. Niraimathi and co-workers [140] have reported biosynthesis of Ag NPs from aqueous extract of Alternanthera sessilis and showed that the extract contains alkaloids, tannins, ascorbic acid, carbohydrates and proteins which serve as reducing as well as capping agents. Biomolecules in the extract also acted as stabilizers for silver nanoparticles. Ag NPs from seed powder extract of Artocarpus heterophyllus have been synthesized [138]. The morphology and crystalline phase of the nanoparticles were determined by SEM, TEM and SAED, EDAX and IR spectroscopy. They were found to be irregular in shape. The extract was found to contain amino acids, amides etc. which acted as reducing agents for AgNO3 to produce silver nanoparticles. The quantity of phenols, anthocyanins and benzoic acid were determined in the berry juices and were responsible for the transformation of silver ions to Ag NPs [241]. UV–vis spectra displayed an absorbance peak at 486 nm for lingonberry and 520 nm for cranberry containing silver nanoparticles. Since the two absorption peaks are different they cannot be assigned only to Ag NPs but also partly to different quantities of the reducing chemicals present in the juices. However, the spectra indicated the presence of polydispersed silver nanoparticles. Puiso et al. [241] have proposed that due to irradiation of water by UV rays, strong oxidants and reductants as photolysis products are formed. They reduce silver ions to Ag NPs or silver oxide. The photolysis products may produce oxidant and reductant but it depends upon the quantum of radiation and exposure time which may not be enough to produce a sufficient quantity of redox chemicals to reduce Ag+ to Ag NPs or Ag2O. This hypothesis is conceptually incorrect because Ag2O cannot be formed as it requires a very strong oxidizing agent. On the other hand, AgNO3 itself is slowly reduced in water, but in the presence of reducing agents the reaction proceeds at a rapid rate. The SPR is dependent on the size, shape and agglomeration of Ag NPs which is reflected from the UV–vis spectra [242]. Mock et al. [243] have found different scattered colors in hyperspectral microscopic images which are mainly due to the different shape and size of silver nanoparticle in the colloidal solution. The blue, green, yellow and red colors have been attributed to spherical, pentagonal, round-triangle and triangle shapes, respectively.

Zaheer and Rafiuddin [12] have reported the synthesis of Ag NPs using oxalic acid as reducing agent and mistook it as green synthesis. Formation of nanoparticles was confirmed by a change in color of the solution which showed an absorption peak at 425 nm (Fig. 2a) in the UV–visible region. It was also noted that a scattered silver film was formed on the wall of the container that shines and reflects light (Fig. 2b) which is the characteristic of monodispersed spherical Ag NPs [244, 245]. Since the size of nanoparticles varies between 7 and 19 nm the silver film is not uniform. It is different from regular silver mirror due to irregular shape and size of nanoparticles (Fig. 2c). Actually, very small size nanoparticles can be obtained when AgNO3 is exposed to a reducing agent for a longer duration of time [246]. The kinetics and mechanism proposed for the formation of Ag NPs by oxalic acid is not convincing [12] because oxalic acid in no case can produce CO2 unless it reacts with any carbonate salt or heated at a very high temperature. The authors [12] have proposed following reactions to prove that the colour of Ag NPs in solution is due to Ag 4 2+ formation that absorbs at 425 nm (Scheme 1). The formation of Ag 4 2+ is highly improbable even if the above reaction is kinetically very fast. Also, the stabilization of Ag 4 2+ is questionable (Scheme 1). This hypothesis of Ag 4 2+ formation is beyond imagination and does not carry any experimental evidence in its support. Absorbance of Ag NPs in solution varies between 400 and 445 nm depending on the nature of reducing agent used for their fabrication. The SPR band in UV–vis spectrum is due to electron oscillation around the surface of nanoparticles. The reduction process is instantaneous and no further spectral change occurs after 60 min. Indicating the completion of redox process. Ag NPs are circular, triangular, hexagonal and polydispersed at 70 °C. The EDAX and XRD spectra support each other.
Fig. 2
Fig. 2

a UV–visible spectra of yellow color silver solution. b and c SEM images of the self-assembled silver nanoparticle mirror like illumination on the walls of the glass. Reaction conditions: [Ag+] = 20.0 × 10−4 mol dm−3; [oxalic acid] = 4.0 × 10−4 mol dm−3; [CTAB] = 10.0 × 10−4 mol dm−3; temperature = 30 °C [12]

Scheme 1
Scheme 1

Reduction of Ag+ ions by oxalic acid [12]

Synthesis of Ag NPs from aqueous extract of Cleistanthus collinus and their characterization by UV–vis, FTIR, SEM, TEM and XRD has been reported by Kanipandian et al. [247]. The crystalline Ag NPs of 20–40 nm showed significant free radical scavenging capacity. Tippayawat et al. [27] have reported a green and facile synthesis of Ag NPs from Aloe vera plant extract. They were characterized by UV–vis, SEM, TEM and XRD. Fabrication of Ag NPs was confirmed on the basis of the appearance of a sharp peak at 420 nm in UV–vis region of the spectrum. In addition, they have reported that the reaction time and temperature markedly influence the fabrication of silver nanostructures. Ag NPs were spherical in shape and particle size ranged from 70.70 ± 22 to 192.02 ± 53 nm. Their size changes with time and temperature of the reaction mixture used during fabrication (Fig. 3).
Fig. 3
Fig. 3

SEM images of silver nanoparticles were obtained at a 100 °C for 6 h, b 150 °C for 6 h, c 200 °C for 6 h, d 100 °C for 12 h, e 150 °C for 12 h and f 200 °C for 12 h [36]

Green synthesis of Ag NPs from Boerhaavia diffusa plant extract has been reported by Vijay Kumar et al. [136] where the extract acted as both the reducing as well as capping agent. The colloidal solution of Ag NPs showed an absorption maximum at 418 nm in the UV–vis spectrum. The XRD and TEM analyses revealed a face centered cubic structure with an average particle size of 25 nm. Ag NPs of 5–60 nm have been synthesized from Dryopteris crassirhizoma rhizome extract in presence of sunlight/LED in 30 min [235]. XRD studies showed face centered cubic structure of silver nanoparticles.

Green synthesis of Ag NPs using 1 mM aqueous AgNO3 and the leaf extract of Musa balbisiana (banana), Azadirachta indica (neem) and Ocimum tenuiflorum (black tulsi) has been done [248]. They were characterized by UV–vis, SEM, TEM, DLS, EDS and FTIR spectroscopy. They were found to accelerate the germination rate of Vigna radiata (Moong Bean) and Cicer arietinum (Chickpea). It is therefore, believed that Ag NPs are not toxic to such crops at germination level. Stable and capped Ag NPs from aqueous fruit extract of Syzygium alternifolium of 5–68 nm have been synthesized [92]. Nearly 12.7% of silver was detected from EDAX. The polydispersed spherical nanoparticles were capped and stabilized by the phenols and proteins present in the fruit extract. Biosynthesis of Ag NPs from methanolic leaf extract of Leptadenia reticulate has been done [142]. They were crystalline, face centred and spherical particles of 50–70 nm. They exhibited antibacterial activity and radical scavenging activity. Purple sweet potato (Ipomoea batatas L.) root extract has been exploited to synthesize Ag NPs [143]. Organic components in the extract acted both as reducing and capping agents. Ag NPs have shown remarkable antibacterial activity against four clinical and four aquatic pathogens. Sweet potato root extract is known to contain glycoalkaloids, mucin, dioscin, choline, polyphenols and anthocyanins which function as antioxidant, free radical scavenger, antibacterial agent and reducing agents. In presence of Ag NPs these functions are further enhanced.

Cytotoxicity of silver nanoparticles

Cytotoxicity of nanomaterials depends on their size, shape, coating/capping agent and the type of pathogens against which their toxicity is investigated. Nanoparticles synthesized from green method are generally more toxic than those obtained from the non-green method. Some pathogens are more prone to nanomaterials, especially Ag NPs than others due to the presence of both the Ag ions released and Ag NPs. They slowly envelop the microbes and enter into the cell inhibiting their vital functions. It is clear that the fabrication and application of nanoparticles has resulted in public awareness of their toxicity and impact on the environment [249, 250]. Nanoparticles are relatively more toxic than bulk materials. They are toxic at cellular, subcellular and biomolecular levels [251]. Oxidative stress and severe lipid peroxidation have been noticed in fish brain tissue on exposure to nanomaterials [252]. The cytotoxicity by Ag NPs is believed to be produced through reactive oxygen species (ROS) as a consequence of which a reduction in glutathione level and an increase in ROS level occur. From in vitro studies on animal tissue and cultured cells, Kim and Ryu [253] have observed an increase in oxidative stress, apoptosis and genotoxicity when exposed to silver nanoparticles. Since such studies have been made with varying sizes of Ag NPs and coatings under different conditions a direct correlation cannot be made. Hackenberg and coworkers [254] reported reduced viability at a dose of 10 µg/mL of Ag NPs of over 50 nm size in human mesenchymal cells whereas some people reported no toxicity [255] even at a higher dose (100 µg/mL). Besides, stability and aging of the sample are also important factors as an increase in toxicity has been reported by aged Ag NPs stored in water for 6 months which is related to the release of silver ions [256]. It seems that the toxicity is a cumulative effect of Ag NPs and silver ions. Some workers have shown that the toxicity of Ag NPs is due to released Ag ions [257] while others have attributed the toxicity to Ag NPs [258].

Vijay Kumar et al. [136] obtained Ag NPs from B. diffusa plant extract and tested them against three fish bacterial pathogens. It was found that Ag NPs were most effective against Flavobacterium branchiophilum. Ag NPs fabricated from P. longum fruit extract exhibited cytotoxic effect against MCF-7 breast cancer cell lines with an IC50 of 67 μg/mL/24 h [240]. They also exhibited antioxidant and antimicrobial effects. Ag NPs were produced by using P. endlicherianum plant extract; and have shown that the inhibitory activity was increased against gram positive and gram negative bacteria when they were exposed to Ag NPs at a very low dose of 7.81 to 6.25 ppm [137]. Latha et al. [89] have fabricated Ag NPs from leaf extract of Adathoda vasica and studied their antimicrobial activity against Vibrio parahaemolyticus in agar medium. The nanoparticles were found to be significantly active against V. parahaemolyticus but were nontoxic to Artemia nauplii. V. parahaemolyticus is a prevalent sea food borne enteropathogen which is closely associated with mortality in Siberian tooth carps, milk fish [259], abalone [260] and shrimps [251]. Vibrio infection in cultured fish and shrimps causes large scale mortality. Quite often, the whole population perishes. The use of antibiotic has made them resistant. Under such conditions, Ag NPs have appeared as an effective remedy which saves shrimps from perishing. Ag NPs from seed powder extract of A. heterophyllus have also exhibited antibacterial activity against gram positive and gram negative bacteria [138].

Ag NPs fabricated from leaf extract of C. thwaitesii have shown antibacterial efficacy against Salmonella typhi, Shigella flexneri and Klbsiella pneumoniae indicating them to be significant. Niraimathi and co-workers [140] have also fabricated Ag NPs from aqueous extract of A. sessilis and showed significant antibacterial and antioxidant activities. Ag NPs from Ocimum tenuiflorum, Solanum tricobatum, Syzygium cumini, Centella asiatica and Citrus sinensis have also shown antibacterial activity against S. aureus, P. aeruginosa, E. coli and K. pneumoniae. The highest activity of nanoparticles was observed against S. aureus and E. coli [261]. Antimicrobial activity of colloidal Ag NPs was found to be higher than the plant extract alone. Lee et al. [141] synthesized Ag NPs from Dryopteris crassirhizoma and found them to be highly effective against B. cereus and P. aeruginosa. Similarly, Ag NPs obtained from leaf extract of banana, neem and black tulsi were also active against E. coli and Bacillus sp. [248]. Hazarika et al. [239] have performed antimicrobial screening of Ag NPs obtained from T. foliolosum root extract against six bacteria and three fungi which showed morphological changes in the bacterial cells. Fabricated of Ag NPs from Millettia pinnata flower extract and their characterization together with anti-cholinesterase, antibacterial and cytotoxic activities have been reported by Rajakumar et al. [145]. Spherical shaped Ag NPs ranging from 16 to 38 nm exhibited excellent inhibitory efficacy against acetyl cholinesterase and butyl cholinesterase. They also exhibited cytotoxic effects against brine shrimp.

Ag NPs obtained from S. alternifolium have also exhibited high toxicity towards bacterial and fungal isolates [92]. Ag NPs fabricated from L. reticulate [142] were found to be toxic to HCT15 cancer cell line. Kanipandian et al. [247] have reported that Ag NPs obtained from C. collinus aqueous extract exhibit dose dependent effects against human lung cancer cell (A549) and normal cell (HBL-100). The IC50 for cancer cells was very low (30 µg/mL) but since Ag NPs synthesized from C. collinus were toxic to normal cells they cannot be used in vivo. However, if the plant extract contains some antioxidants, the whole mixture may exhibit this property but the nanoparticles alone are incapable to do so. Ag NPs from Aloe vera plant extract have shown varying degrees of antibactericidal effects [36]. Ag NPs obtained at 100 °C for 6 h and 200 °C for 12 h (varying temperature and reaction time) exhibited change in bacterial cell membrane when contacted with the nanoparticles (Fig. 4). They were more effective for gram negative bacteria (P. aeruginosa, ATCC27803). In addition, they have also shown minimal cytotoxicity to human peripheral blood mononuclear cells.
Fig. 4
Fig. 4

SEM images of the bacterial strains. a Staphylococcus epidermidis, Gram-positive, b Pseudomonas aeruginosa, Gram-negative, c S. epidermidis treated with 100-6 h silver nanoparticles (0.04 mg/mL), d P. aeruginosa treated with 100–6 h silver nanoparticles (0.04 mg/mL) [36]

The particle size, agglomeration and sedimentation are related to the cytotoxicity of silver nanoparticles. It has been demonstrated from Alamar Blue (AB) and Lactate dehydrogenase test (LDH) that Ag NPs of 10 nm coated with citrate and PVP separately, are toxic to human lung cells [262] when exposed for 24 h. AB test is a measure of cell proliferation and mitochondrial activity. However, the LDH measures the cytotoxicity of Ag NPs in terms of membrane damage from the cytoplasm. Both the citrate and PVP coated nanoparticles of 10 nm exhibited significant toxicity after 24 h at the highest dose of 50 µg/mL. Ag NPs of larger dimensions did not alter cell viability [263, 264]. Cytotoxicity is related to enzyme inhibition which is correlated to the release of Ag ions because they inhibit the catalytic activity of LDH.

It has been observed that Ag NPs damaged DNA but they did not increase ROS when cells were exposed to them for 24 h at a dose of 20 µg/mL [263]. Gliga et al. [262] have suggested that silver ions from AgCl are released in the biological fluid and complexed. The formation of AgCl is possible only if the fluid is contaminated with Cl ions, nevertheless it cannot ionize to Ag+ and Cl ions since AgCl is almost insoluble in aqueous medium [265]. The experiment with extracellularly released silver ions in cell medium did not exhibit toxicity, perhaps it would have reacted with Cl ions to yield insoluble AgCl.

Cytotoxicity is related to the size of Ag NPs irrespective of the coating agent. Carlson et al. [266] have shown an increase in ROS production for 15 nm hydrocarbon coated Ag NPs relative to 55 nm. It has been reported by Liu et al. [267] that 5 nm Ag-nanoparticles were more toxic than 20 and 50 nm nanoparticles to four cell lines, namely, A549, HePG2, MCF-7 and SGC-7901. Wang et al. [268] have also reported that smaller nanoparticles (10–20 nm) induce greater cytotoxicity than the larger ones (110 nm), and citrate coated 20 nm Ag NPs produced acute neutrophilic inflammation in the lungs of mice compared to those with larger ones. The cell viability and DNA damage may be explained by ROS generation [269] which may be contradictory to findings by others in in vitro studies [253].

It is hypothesized that irreparable DNA damage is due to the interaction of Ag NPs with repair pathways. Since this work has been done in vitro, the DNA once damaged may not have the ability to repair. However, in living systems the cells have the ability to undergo repair and multiply but such experiments have seldom been done. It is however, unanimously agreed that both Ag NPs and silver ions are present at the subcellular level. The transformation of Ag to Ag+ ions occurs due to their interaction with biomolecules in the cell membrane. The release of elemental silver is directly proportional to the size of nanoparticles in a non-linear fashion [270]. The size dependent toxicity is related to the intracellular release of silver ions. Although, agglomeration of nanoparticles reduces their release, the antibacterial effect was hindered under anaerobic condition, because in absence of oxygen, the oxidation process Ag → Ag+ ceases to continue. Ag NPs exhibited excellent activity against Y. enterocolitica, P. vulgaris, E. coli, S. aureus and S. faecalis. Since the nanoparticles are smaller than the bacterial cell they may stick to their cell walls disallowing permeation of essential nutrients leading to the death of microorganisms [236]. Smaller size is related to greater surface area of nanoparticles and their agglomeration around the cell wall inhibits the cell division of microbes.

Besides their application in diverse areas, Ag NPs are extensively used as antioxidant and antimicrobial agents regardless of the process of their synthesis [271, 272]. They are more toxic to microorganisms than human beings. Antibacterial and antifungal activities of Ag NPs were tested against B. cereus, S. aureus, C. koseri, P. aeruginosa bacteria and C. albicans fungus respectively. It has been proposed that Ag NPs penetrate into the bacterial cell and interact with the thiol, hydroxyl and carboxyl groups of the biomolecules present in them, eventually deactivating the vital functions by releasing Ag+ ions. The authors have, however, not explained how the Ag+ ions were produced. We firmly believe that silver ions must have been produced through a redox mechanism and subsequently complexed with electron donating thiol and phosphate groups inhibiting the cell replication of pathogens. It is well known that silver ions strongly bind with sulfur and oxygen containing electron donor groups in living system and arrest the functioning of vital organs that lead to the death of animal.

Ag NPs synthesized from lingonberry and cranberry juices [241] were tested for their activity against microbes commonly found in food and food products namely, S. aureus, S. typhi, L. monocytogenes, B. cereus, E. coli, B. subtillis and C. albicans. They observed that Ag NPs were more effective towards S. aureus, B. subtillis and B. cereus. Antibacterial activity was screened against B. cereus and S. aureus which produce toxins in food products [243]. A similar study has also been reported by Nanda and Saravanan [168] on other pathogens such as S. aureus, S. epidermidies and S. pyogens. The decrease in antimicrobial effect of Ag NPs against food borne bacteria has been ascribed to low pH or high NaCl content in food. The high concentration of NaCl may increase the toxicity towards bacteria because they may kill them. However, it is concluded that Ag NPs may be used in packaging to prevent infection in food products by microbes.

Zhao and Stevens [273] have studied antimicrobial effects of Ag salts on 12 species of bacteria and showed that they are highly effective against them. It has also been shown [274] that Ag NPs with amphiphilic hyperbranched macro molecules act as antimicrobial coating agents. Kim et al. [275] have thoroughly screened the antimicrobial effect of Ag NPs prepared from AgNO3 and NaBH4 as reducing agent. They examined the efficacy of a wide range of concentrations of Ag NPs starting from 0.2 to 33 nM. At a concentration of 33 nM of Ag NPs the growth inhibition of E. coli and E. aureus was almost comparable with the positive control, although at 13.2 nM concentration a significant effect was observed. However, the inhibitory effect of 1.6–6.6 nM of Ag NPs is nearly the same (~ 55% relative to control). It was observed that silver nanoparticle is most effective against E. coli and has a mild inhibitory effect on S. aureus. However, gold nanoparticles of the same concentration were ineffective against these microbes, although it also belongs to the same group of elements.

Ag NPs synthesized from fungus Humicola sp. were investigated for their cytotoxicity on NIH3T3 mouse embryonic fibroblast cell line and MDA-MB-231 human breast carcinoma cell line [224]. In both cell lines, the cell viability declined in a dose-dependent manner. Cytotoxicity of Ag NPs was recorded at a concentration of 250 µg/mL; the cell viability declined by 20 83% in the case of NIH3T3 and 42 18% for MDA-MB-231 cell line at 1000 µg/mL concentration. Very recently [269], it has been investigated that Ag NPs in conjugation with other metals such as TiO2@Ag nanoparticles act against leishmaniasis. These nanoparticles along with other drugs for leishmania, like neglumine antimoniate at nontoxic concentrations increase the efficacy of both drugs. This combination of drug led to the inhibition of L. tropica amastigotes at a very high rate of 80–95%. Also, it increased the metabolic activities 7–20-fold.

Owaid et al. [237] have produced Ag NPs from aqueous extract of P. cornucopiae var. citrinopileatus which served both as reducing and stabilizing agent. Their antimicrobial activity was investigated against four pathogenic Candida sp. namely C. albicans, C. glabrate, C. krusei and C. pseudotropicalis. Ag NPs at 60 µg/well showed a significant increase in inhibition of candida sp. However, pure extract was ineffective against all microbes at 20–40 µg/well. Mechanism of action has been ascribed to the interaction between the positive charge on silver ion and the negative charge on the cell membrane of microorganism [25, 35]. Due to electrostatic attraction between the two the silver ions penetrate into the microbial cell via diffusion leading to their death. Ag NPs synthesized using fungus Trichoderma viride were examined for their antimicrobial activity in combination with various antibiotics (ampicillin, kanamycin, erythromycin and chloramphenicol) against both gram positive and gram negative bacteria [234]. Antibacterial activities of antibiotics were increased in the presence of Ag NPs against the tested strains and P. aeruginosa. The original aqueous extract of P. ostreatus was found to be ineffective against all bacterial strains at 25–75 µg/mL.

Allahverdiyev et al. [276] have reported that the combination of Ag NPs with antibiotics decreases the toxicity toward human cells by reducing the required dosage. Furthermore, these combinations restore the ability of the drug to kill bacteria that have acquired resistance to them [175]. Hence, a separate approach of using Ag NPs synthesized from bacterial strains alone and in combination can act as effective novel antimicrobials to sensitize resistant pathogens. Nevertheless, a study with E. coli has demonstrated that the bacteria could become resistant to Ag NPs on its regular exposure for 225 generations through genetic mutations [277]. Thus, a precaution should be taken to avoid the constant exposure of microorganisms against such types of nanoparticles. In addition, treatment with bacterial Ag NPs has shown the cell viability reduction in a dose-dependent manner in HeLa cervical cancer [278, 279], MDA-MB-231breast cancer [280], A549 adenocarcinoma lung cancer [281] and HEP2 [282] cell lines. Ag NPs produced from bacterial strains exhibited cytotoxicity to cancer cells but their impact on normal healthy cells cannot be ignored.

Mechanism of antibacterial activity

As discussed previously, several reports are available which have shown that Ag NPs are effective against pathogenic organisms namely B. subtilis, Vibrio cholerae, E. coli, P. aeruginosa, S. aureus, Syphilis typhus etc. [10, 11, 109, 145]. Ag NPs with larger surface area provide a better contact with microorganisms [283]. Thus, these particles are capable to penetrate the cell membrane or attach to the bacterial surface based on their size. In addition, they were reported to be highly toxic to the bacterial strains and their antibacterial efficiency is increased by lowering the particle size [284]. Many arguments have been given to explain the mechanism of growth inhibition of microbes by Ag NPs but most convincing is the formation of free radical which has also been supported by the appearance of a peak at 336.33 in the electron spin resonance (ESR) spectrum of Ag NPs [275]. The free radical generation is quite obvious because in a living system they can attack membrane lipids followed by their dissociation, damage and eventually inhibiting the growth of these microbes [285]. It is worth noting that the equal mass of silver Ag NPs and that of Ag ions exhibit identical growth inhibition of E. coli and S. aureus. In a study, the highly antibacterial activity has been ascribed to the release of silver cation from Ag NPs [173]. The Ag+ permeated into bacteria through the cell wall [286, 287] as a consequence of which the cell wall ruptures leading to denaturation of protein and death. Since Ag ions are positively charged and much smaller than neutral Ag NPs they can easily interact with electron rich biomolecules in the bacterial cell wall containing S or P and N. Some researchers have reported that interaction between the positive charge on Ag NPs and negative charge on the cell membrane of the microorganisms is the key to growth inhibition of the microbes [286, 287]. On the other hand, Sondi et al. [288] have reported that antibacterial activity of Ag NPs toward gram negative bacteria depends on its concentration. The nanoparticles form pits in the cell wall of microbes, get accumulated, and permeate into the bacterial cell leading to their death. It has been reported [289, 290] that Ag free radical formation and antimicrobial property are inter related which has been confirmed by ESR [275]. They claim that such an antimicrobial study included both the positively charged silver ions and negatively charged silver nanoparticles.

The absorption of Ag NPs at 391 nm is the signature of spherical nanoparticles due to their surface plasmon resonance [291]. This absorption spectrum does not undergo any change even when the suspension of Ag NPs is diluted ten times indicating that they are not agglomerated. Besides Ag NPs and silver compounds, there are other inorganic ions which also possess antibacterial properties [241, 287, 292]. It is known that silver ions bind to the protein of the microorganisms preventing their further replication but the organisms also avoid interacting with these ions and produce cysts to become resistant.

Ag NPs may be oxidized to Ag+ but cannot be reduced [287, 289]. Silver is known to have 4d10, 5s1 outermost electronic configuration and it cannot hold an extra electron to become Ag anion. Silver salt of sulphathiazine is used in burn therapy to protect the skin from infection by pseudomonas species. Silver is released slowly from the salt which is sufficiently toxic to microorganisms. Since the salt is sparingly soluble the silver acts on the external cell structure. Silver salt and Ag NPs exhibit cytotoxicity against a broad range of microorganisms, although the toxicity depends on the quantum of silver ions released [275].

The monodispersed nanoparticles of uniform size are produced. Graphene oxide exhibits antibacterial activity against E. coli [293, 294] but Ag NPs functionalized graphene based material show enhanced antibacterial activity [295, 296]. Graphene oxide is nicely dispersed in polar solvents like water which allows the deposition of nanoparticle for its use in various fields. Antibacterial activity of both Ag NPs and Ag-graphene oxide composite has been tested in a wide range of concentration between 6.25 and 100 µg/mL against both gram positive and gram negative bacteria. It was noticed that both Ag NPs and Ag-graphene oxide composite were more effective against gram positive than gram negative bacterial strains. Ag-graphene oxide is a better growth inhibitor of S. Typhi, even at a very low concentration of 6.25 µg/mL, than Ag NPs of the same concentration. However, Ag NPs and Ag-graphene oxide do not show any inhibitory effect against gram positive bacteria, S. aureus and S. epidermis below 50 µg/mL. It was also noted that graphene oxide alone is ineffective against these bacteria even at a higher concentration of 100 µg/mL [293, 296].

Silver ions released from Ag NPs may penetrate into bacterial cell components such as peptidoglycan, DNA and protein preventing them from further replication [297, 298]. Release of Ag+ ions means the oxidation of elemental silver which requires an oxidizing agent.
$$ {\rm Silver}\,\, {\rm nanoparticle} \to {\rm Ag}^+ + {\rm e}^- $$

The organic groups like carbonyl and protein in the bacterial cell wall are electron donors rather than electron acceptors and hence they cannot produce Ag+ ions from Ag atoms, nevertheless the Ag+ ions are produced which confirms the presence of an oxidizing agent [296, 299]. Ag+ ions are thus bonded to the proteins of bacteria and inhibit their vital functions.

Tho et al. [300] have shown that spherical Ag NPs of 2.76–16.62 nm size fabricated from Nelumbo nucifera seed extract are highly toxic to Gram negative bacteria. The antibacterial property has been ascribed to the attachment of Ag NPs to the surface of cell membrane disallowing permeation and respiration of the cells.

The outer layer of gram negative bacteria is made up of a lipopolysaccharide layer and the inner layer is composed of a linear polysaccharide chain forming a three-dimensional network with peptides. Ag NPs get accumulated due to attraction between the negative charge on the polysaccharides and weak positive charge on the silver nanoparticles. It stops the cell replication of the microbes.

Toxicity by nanoparticles is generally triggered by the formation of free radicals, such as ROS [301, 302]. If the ROS is produced it may cause membrane disruption and disturb the permeability. The mechanism of growth inhibition follows electrostatic interaction, adsorption and penetration of nanoparticles into the bacterial cell wall. Toxicity of nanoparticles also depends on composition, surface modification, intrinsic properties and type of microorganisms [9, 303306]. For instance, TiO2-nanoparticles can increase peroxidation of the lipid membrane disrupting the cell respiration [307]. The biogenic Ag NPs in combination with antibiotics like erythromycin, chloramphenicol, ampicilin and kanamycin enhance the toxicity against gram positive and gram negative bacteria [308, 309]. A possible mechanism is presented in Fig. 5. Besides, Ag NPs are also toxic to nitrifying bacteria [310]. The ROS include superoxide (O2), hydroxyl (·OH), peroxy (RCOO·) and hydrogen peroxide (H2O2). RNS includes nitric oxide (NO·) and nitrogen dioxide (NO2) [311, 312]. The cell replication and development of microbes in ROS containing atmosphere will cease to continue. However, this process may be delayed in presence of an antioxidant such as an enzyme or a non-enzymatic component which scavenges the free radicals [313].
Fig. 5
Fig. 5

Mechanism of action of silver nanoparticles against bacterial cells

Conclusion

Regardless of the method of fabrication, Ag NPs are used as an antimicrobial agent, electrochemical sensors, biosensors, in medicine, health care, agriculture and biotechnology. They have great bactericidal potential against both gram positive and gram negative pathogens. Since Ag NPs coupled with antibiotics are active against many drug resistant bacteria they can be used as easily accessible medicine for the treatment of several infections. Ag NPs in the drug delivery system, quite often increase the solubility, stability and bio-distribution enhancing their efficiency. In presence of nanoparticles the absorption of medicine increases several times therefore, Ag NPs may be used as a drug delivery system.

Although, the long-term effect of nanoparticles on human health and crops is not clear. A large number of nanoparticles are being explored in many areas of industry technology, biotechnology and agriculture. It is known that various forms of silver from laundry, paints, clothes etc. and biosolids reach the sewage and sludge. It has been reported that nano sized Ag2S are formed in the activated sludge as a consequence of the reaction between silver nanoparticles/Ag+ ions and the sulfide produced in sewage. It is not possible for Ag NPs in the elemental form to react with evolved H2S. Only Ag+ ions may react with H2S to yield Ag2S according to the reaction given below.
$$ 2{\rm AgNO}_3+ {\rm H}_2 {\rm S} \to {\rm Ag}_2 {\rm S}+ 2{\rm HNO}_3$$
Ag2S or AgNO3 may be ionized to give free Ag+ ions which inhibit the bacterial growth. Besides many advantages of Ag NPs there are some disadvantages too. They inhibit the growth of nitrifying bacteria, thereby inhibiting the biological nitrogen removal. As little as 1–20 ppm Ag NPs have been reported to be effective against microbes. It is anticipated that Ag NPs may be used as an inexpensive broad spectrum antimicrobial agent to protect plant crops and infections in human beings.

Declarations

Authors’ contributions

AH, KSS and RAKR gathered the research data. AH and KSS analyzed these data and wrote this review paper. All the authors read and approved the final manuscript.

Acknowledgements

Authors are thankful to publishers for permission to adopt figures in this review.

Competing interests

The authors declare that they have no competing interests.

Availability of data and materials

Not applicable.

Consent for publication

Not applicable.

Ethics approval and consent to participate

Not applicable.

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Authors’ Affiliations

(1)
Department of Chemistry, Aligarh Muslim University, Aligarh, Uttar Pradesh, 202002, India
(2)
Department of Biology, College of Natural and Computational Sciences, University of Gondar, P.O. Box # 196, Gondar, Ethiopia
(3)
Department of Applied Chemistry, Zakir Husain College of Engineering and Technology, Aligarh Muslim University, Aligarh, Uttar Pradesh, 202002, India

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