Community Ecology

Community Ecology

  • Damian Settle added an answer:
    How to take into account strangler figs in calculations of basal areas?
    In tropical forest inventories, strangler figs are common. How estimate the basal area of a strangler figs and their tree hosts? This issue is very imporatant as it may lead to important mistakes in total basal area estimation.
    Damian Settle · James Cook University

    Dear Thomas;

    Did you find a suitable method? I am facing a similar issue. I am interested determining the Basal area of fig trees. Both free standing, multiple stemmed individuals and/or parasitic stranglers. Is there an effective way to determine basal area short of measuring every stem?  

  • Valérie Coudrain added an answer:
    Can we compare species diversity (i.e. Shannon, Simpson's) and evenness between sites that have large differences in abundance of individuals?
    I would like to know if it is meaningful to compare species diversity and eveness between sites that range from 3 individuals to up to several hundred individuals. Especially for eveness, I have the impression that we can get quite similar values for totally different abundances of individuals, which renders interpretation difficult.
    Valérie Coudrain · French National Institute for Agricultural Research

    Thank you very much.

    @ Zdenek: your paper is really interesting and helpful

  • Rachda Berrached added an answer:
    What should be the sample size in leaf anatomical study at population level (i.e., number of plant individuals, leaves, and measurements)?

    The aim of the study is to compare montane and lowland populations of a plant species with respect to leaf anatomy. The montane populations also include those situated on different altitudes. I collected 25 plant individuals from each population on a defined area: the whole plants as a herbarium material as well as the shoots with leaves (3 vegetative and 3 flower-terminated ones from each individual) as alcohol-fixed material. The plant is small-leaved and each individual contains dozens of leaves on both types of shoots.

    Now the question is how many leaves of each individual to analyze anatomically and how many measurements of each particular quantitative trait (e.g., size and density of stomata, hairs, leaf thickness and size, etc.) to take from each leaf? Also, what would be the statistical methods most suitable to use in such a study? Thanks in advance.

    Rachda Berrached · University of Science and Technology Houari Boumediene

    Hi Eugene;

    I propose this paper, I think it is really important for you.

    Good luck.

  • Catherine Theresa Imperial Mampo added an answer:
    Is there a relation between a community's diversity and it's stability? What would be the trend for the different levels of succession in a community?
    For example, would a pioneer community have more elasticity (return to it's pre-disturbance state) but low amplitude (disturbance threshold allowing return)?
    Catherine Theresa Imperial Mampo · Ateneo de Manila University

    This article is also useful: https://www.researchgate.net/profile/Samuel_Mcnaughton/publication/201999402_Diversity_and_stability_of_ecological_communities_a_comment_on_the_role_of_empiricism_in_ecology/links/5446612a0cf2f14fb80f355d.pdf

  • Alfonso Nebra added an answer:
    How should I analyze my stream fauna data in JMP?

    Good Day,

    I am trying to figure the analysis I need to do for my project. I study shrimp and fish in 3 tropical intermittent streams. I am testing to see if there is a difference in species composition at different elevations. My experimental design includes a low, mid-, and high elevation site in each stream. I have selected 3 streams, so therefore 9 sites total. I chose 3 streams so I can say with confidence that a species distribution changes with elevation. I have been sampling for a year. I have sampled at each site 4 random times in the year; therefore, I have collected 12 samples for each stream (4 at the low site, 4 at the mid-site and 4 at the high elevation site). Altogether 36 samples. We have a dry and wet season here. Seasonality is a covariable.

    What is the best way to setup my data? Recommendations for analysis? Help is much appreciated:)

    Thank You,

    Kayla

    Alfonso Nebra · IRTA Institute of Agrifood Research and Technology

    I aggre with Scott's answer; in order to complement this 'visual' tool you can perfom ANOSIM analysis: "Analysis of similarities" hypothesis for differences between groups of community samples (defined a priori), using permutation/randomisation methods on resemblance matrix. Handles one way and two way crossed/nested designs with replication. Also handles two way crossed layout with no replication" text extracted from  PRIMER software manual.

  • Joe Shelnutt added an answer:
    Does anyone have suggestions for developing a course ecological recovery potential screening tool, to address multiple ecosystems across a landscape?

    The location is a corridor from the Florida panhandle, westward to east Texas. Longleaf pine is a significant component of this landscape but riparian, wetland, seepage bogs, and other fragmented ecosystems need to be addressed simultaneously within this landscape. Developing a course tool to prioritize connectivity and where ecological restoration should/can occur is needed. 

    Joe Shelnutt · Texas A&M University System

    Thank you Olga! 

  • Michael F. Merigliano added an answer:
    What method should I use for comparing similarity of species compositions among subsampled sites?

    I have sampled 4 sites for bryophytes using quadrats in and around 4 wetlands. (I recorded abundance data.) Two of the wetlands are embedded in deciduous woodland, two in coniferous woodland.

    I'm trying to ask two main questions:

    -whether the species compositions of the wetlands are more similar to the other wetlands or their surrounding woodlands

    -whether the species compositions of the wetlands in each forest type are more similar to the other wetlands of the same type or to a wetland of the other forest type

    Is there a test I can do to answer these questions?

    I've done an NMDS ordination of the data. The polygons surround all the quadrats from each of the four sites, the spiders connect the wetland and woodland quadrats from each site. The wetland quadrats are colored blue, woodland green. Conifer is the plus hardwood is the triangle.

    It seems to show that the two largest wetlands are most similar to each other (despite being in different forest types). It seems to show that the smaller wetlands each are more similar to the larger wetland of the same forest type. (Although the hardwood wetland is almost as similar to the surrounding woodlands as the other hardwood wetland.)

    Is there some way to test if this is actually significant?

    Michael F. Merigliano · University of Montana

    Although somewhat off-topic, a concern is the very small sample size (n =4, at most). There may be enough power if the differences between sites are very high with little noise, but your NMDS graph indicates otherwise.

    A good, basic source for metrics and analysis of community data is McCune and Grace 2002. Analysis of Ecological Communities.

  • Valério De Patta Pillar added an answer:
    How can I compare community functional diversity across space and time?

    I am working with a dataset of six communities that were sampled at two time points. I am looking for a simple way to see whether functional diversity of each community has changed from time point A to time point B.

    My functional data is count data [number of species per community with a given functional trait]. As such, my dataset seems too small for most ordination approaches. Overall, I am investigating multiple traits within three different functional categories [growth form, habitat preference, and symbiont status]. At the moment, I am treating each functional category as a separate dataset.

    Thank you!

    Valério De Patta Pillar · Universidade Federal do Rio Grande do Sul

    Dear Klara, it is important to clarify your question:

    You could compute functional diversity of each community at time point A and compare to functional diversity of the same communities at time point B. For this I suggest using Rao entropy, for which you will need to compute a dissimilarity matrix between species based on their traits (if the traits are of mixed type, the Gower index may be useful). In this case you can only tell about the temporal change in the overall functional diversity of each community, and nothing about the functional identity of the community components. This is a limitation analogous to when communities are compared by their species diversity (e.g., by using Shannon diversity). 

    Another option is to compare the communities based on their functional composition, for which you may consider the definition of fuzzy-weighted community composition. This is described in Pillar et al. (2009, http://dx.doi.org/10.1111/j.1654-1103.2009.05666.x). See also Pillar & Duarte (2010, http://dx.doi.org/10.1111/j.1461-0248.2010.01456.x) in the context of phylogenetic analysis. The fuzzy-weighting requires as input a similarity matrix between species based on their traits (which could be the above mentioned Gower index), which after proper standardisation to unit column will define a fuzzy set matrix U of species by species. The fuzzy-weighted community composition is given by matrix X obtained by matrix multiplication (X = UW), where W is the matrix of species composition in the communities.

  • Bernabé Moreno added an answer:
    Which biotic & abiotic components should I sample/measure in order to elucidate if a system is rather pelagic- or benthic- controlled?

    Benthic realm and its biotic composition is highly important in glacio-marine fjords, specially when considering the cryosphere dynamics and the resulting phenomena (sedimentation, resuspension, freshwater influx, inter alia).
    Also, in Antarctic seasonal bays (i.e. Mackellar Inlet  (King George Island, South Shetlands), where I've sampled macrobenthic communities for previous research (see: http://goo.gl/YOy16D)) pelagic realm also plays a key role in terms of primary production and its consequent influence on higher trophic levels.

    It's certain that analysing the benthic composition is more predictive when trying to speculate future scenarios. I presumably assume that the Mackellar Inlet is mainly a benthic-controlled system. Nevertheless, in order to be sure of this hypothesis I should go further through an integrated analysis of both realms. 

    The protocol that my colleagues usually execute is: macrobenthic survey (van Veen grab 0.05m2), collect plankton with plankton nets, and measure abiotic variables like temperature, pH, conductivity, turbidity and marine currents patterns (speed & direction).


    I'd like to know if there's any specific protocol pointing straightforward to my question. What other measurements should I consider?

    Thanks for the help. Cheers.

    BSc. Bernabé Moreno

    Bernabé Moreno · Universidad Científica del Sur

    Thank you all for your substantive comments. They're already being very useful to help me structure some kind of study. Cheers.

  • Mika Yasuda added an answer:
    Is functional alpha diversity equal to functional richness?

    Pool et al (2014) quantify alpha functional diversity as the volume of the convex hull filled by the fish species of each community in two-dimensional functional space using the values from the first two functional axes.

    But I wonder taxonomic alpha diversity is simply the species richness, so the alpha functional diversity can be functional richness...

    Mika Yasuda · Chinese Academy of Sciences

    Thank you very much for your answer, Thiago,

    I will read these paperes as well.

    Best wishes,

    Mika

  • Alan Feest added an answer:
    Should Simpson's E or Shannon's E be preferred for evenness estimates?

    I have a multi-year dataset with about 100 species where the Simpson's D is already available.

    As I want to look at evenness I wonder about the differences between Simpson's E and Shannon's E, and if any one of them is to be preferred.

    Alan Feest · University of Bristol

    Klaus

    I agree that a single measure of biodiversity is not very informative and my work on "biodiversity quality" is based on the picture expressed by a range of indices.  Simpson's E sometimes shows change first when biodiversity is changing as it reflects the relationship between species populations.

    Hope this is helpful.

    Alan

  • Sebastian Dardanelli added an answer:
    Is it possible to incorporate detection probabilities to nestedness analysis?
    Is it possible to incorporate detection probabilities to nestedness analysis? The only approach I have seen that specifically deal with this issue are the papers from Cam et al. 2000 (Ecol Appl. & Oikos).
    Sebastian Dardanelli · Instituto Nacional de Tecnología Agropecuaria

    Hola Alexis! Si lo tenía a ese gracias! Parece que además de esos papers de Cam y el weighted nestedness no hay nada más. Voy a probar con esas dos cosas juntas para presencia ausencia y presencia ponderada por abundancias.  

    Abrazo!

  • Irene Zweimüller added an answer:
    Which clustering method is the most realistic and descriptive in ecological terms?

    I know that both 'Single-linkage' and 'Complete-linkage' clustering are monotonic methods (non-metric), which is great under a theoretical point of view. Nevertheless, 'Group-average' clusters sometimes are easier to describe.

    I'm working with Antarctic macrobenthic communities, and I would like to know which of these three methods is the most adequate for an environmental analysis based on your own experience.
    Thanks & cheers!

    Irene Zweimüller · University of Vienna

    When you use cluster analysis, I recommend to standardize your variables (for example z-transformation, which results in mean=0 and SD=1 for the z.transformed variables). Ward´s clustering method (together with squared Euclidian distances) gives the best results - at least in my experience. 

    If you have extreme values in your variables, you may need to do a log-transformation before you start.

    good luck, Irene

  • Raymond K. Timm added an answer:
    Is it worthwhile to only report a pattern in community ecology, without including an analysis of the potential environmental variables explaining it?

    I was recently told by a referee that my manuscript about the long term temporal patterns of a fish community in a tropical wetland was irrelevant and useless because it did not include an analysis of the potential factors explaining such pattern, meaning environmental variables. These were not included because information for the years of my study is not available.

    I would like to  know if this is a widespread opinion among community ecologists, and if the state of the art is such that works limited to describe community patterns are not necessary anymore.

    Thank you, I am looking forward to get to know your opinions.   

    Raymond K. Timm · Cramer Fish Sciences

    Gabriella - sorry to hear about the harsh review.  Nobody deserves that.  I would chime in to say that it sounds like your study is stuck in the landscape ecology hinterlands between descriptive and functional metrics.  in landscape ecology, functional  metrics are of course the objective.  With that said, describing patterns quantitatively is an important part of understanding how landscapes function - and has to be done first.  If you don't already have it, check out FRAGSTATS and associated publications (Kevin McGarigal).  They developed a free and very powerful utility to quantify patterns.  Also, I might suggest resubmitting to Landscape Ecology and do what you can with other environmental response data to perform analyses and frame up hypotheses to build on your progress.  Good Luck.

  • Elizabeth Kierepka added an answer:
    What is the best way to import microsatellite data to perform a dbRDA?

    I am interesting in looking at the relationship of several environmental variables on genetic differentiation across 16 bee populations (Many individuals per population) using dbRDA. Using Legendre and Legendre (2012) as a guide, I have generated a distance matrix for my microsatellite data, and then performed a principal coordinates analysis. I now have two questions:
    1. Negative eigenvectors need to be a corrected. Which would be the best method to do so?
    2. The PCoA gives me an eigenvalue for each population at each axis, as well as the overall eigenvalue for each axis. I am assuming that it is the eigenvalues for population at each axis that are important. Is there a standard format used by vegan for this type of data?
    I am new to analyzing community-type data, so any suggestions of pointers would be greatly appreciated. Thanks!

    Elizabeth Kierepka · University of Georgia

    Hi Jess,

    For dbRDA, there are R packages and separate programs that will perform the dbRDA all in one function. I have used vegan with the function capscale as well as DistLM by Anderson 2003 (PC program). Typically in a dbRDA, all the axes with positive eigenvalues are retained (at least in the calculation methods I have used), and axes with negative eigenvalues are not used in the analyses.  

    What you will use as your dependent variable are the scores from the PCoA, but any dbRDA function will do that for you. I also suggest that you run a partial dbRDA because you will have issues with spatial autocorrelation if you are running any community or spatial type data in your analyses. 

    I have code on Dryad from my previous manuscript comparing dbRDA and others in landscape genetics, but briefly here's what I did in vegan:

    ###gen file must not have headers, and it needs to be either a square or triangular matrix#######

    gen<-read.table(file="Your_PairwiseGeneticDistance_File.txt")

    xy<-read.table(file="xy_coordinates_for_each_study_site.txt")

    land<-read.table(file="landscapedata_for_each_population.txt")

    in vegan:

    dbRDA<-capscale(gen~land)

    p.dbRDA<-capscale(gen~land+Condition(xy))

    stats.full<-anova.cca(dbRDA, by="term")

    stats.p<-anova.cca(p.dbRDA, by="term")

    This will give you your F-stats, inertia, and p-value for each landscape variable you tested. If you want the F-stat, inertia, and p-value for the full model, just leave off the by="term". 

    Hope this helps,

    Liz 

  • Sergey Popov added an answer:
    What software can be used to study the structure of a metacommunity?

    Dear colleagues, prompt software for calculation of parameters a metacommunity. It is desirable to be able to use tables Excel. How can I adequately describe the effect of spatial scale on the part of the community?

    Sergey Popov ·

    Вот консольный режим и непривычен. Но, видимо, все равно придется и его освоить. Пока у меня основные программы SPSS, MapInfo, QuantumGIS, Surfer и серия программ для методов SADIE.

  • Summer M Burdick added an answer:
    Which is the best method to relate species occurrences to human impact variables in a sparse data matrix?

    I have a data-set of macrophyte species (Presence/Absence, %-Cover) collected in river sites together with environmental (e.g. discharge, river slope, substratum composition...) and human impact variables (e.g. morphological quality scores, %-landuse in catchment...). The species data matrix is rather sparse, meaning many species occur in a few sites but are absent from many others, also because the data has been sampled along a long environmental gradient. I now want to quantify how species occurrence to particular environmental variables (either single or jointly) and particularily to human impact. One tricky thing in this regard is that some of the human impact variables are covarying with important environmental variables (e.g. discharge ~ %-landuse), making it challengig to quantify the effect of humans on species occurrences alone.

    I already came along a number of techniques used in this context (e.g. CCA, INDVAL). However, I still concluded this is an interesting subject to discuss and hence I would like to hear your personal opinion about i.) the kind of analyses you would consider most suitable and ii.) how to deal with the sparcity of species and the mentioned covariation in the data-set.

    Thanks, and I look forward to hear from you!

    Summer M Burdick · United States Geological Survey

    You might consider using an occupancy modeling approach (MacKenzie et al. 2006).  This approach is good when your response variable is binary (presence/absence). There are occupancy models that allow you to look at the presence and absence of multiple species along an environmental gradient. One benefit of this approach is that it allows you to compare specific competing hypotheses.

    You can deal with correlated parameters in several ways. 1) Where you have two variables just pick one 2) you could use a PCA or some other method to distill these variables into one meaningful component that can be used in your occupancy models or 3) you could fit a series of occupancy models that include and interaction between correlated terms. If you then compare these models with AIC you may be able to determine which variable is more important. However, if you have completely correlated variables you may never be able to tell which one is causing and effect. 

    I hope this is helpful. 

    MacKenzie, D., Nichols, J., Royle, J.A., Pollock, K., Bailey, L., and Hines, J., 2006. Occupancy Estimation and Modeling: Inferring Patterns and Dynamics of Species Occurrence. Elsevier Academic Press

  • Ken Sulak added an answer:
    Is it necessary to standardize for sampling effort before comparing asymptotic species richness?

    If you want to compare diversity e.g. Hill numbers across species assemblages you need to standardize for sample size or sample completeness. Does the same count for asymptotic species richness estimators (such as Chao indices or ICE and ACE)? You calculate the same, namely 'true' species richness (often based on the number of singletons), so I guess it already corrects for differences in sampling effort?

    Second (related) question:

    Can anyone explain why I find different values for the same estimators calculated with different programs? Using the same abundance dataset I calculated ACE and Chao1 in EstimateS, R (fossil) and SPADE...and I got three different values for each estimator.

    I know that EstimateS uses resampling and that it cannot calculate ACE, but strangely the Chao1 values are lower than the estimated species richness when doubling the reference sample.

    Ken Sulak · United States Geological Survey

    None of the conventional measures of diversity and species richness, like H and H', are truly sample size independent.   They are advertised as such, but fail when sample  sizes are low.  Species rarefaction curve analysis is perhaps the best way to compare species richness - if you have a number of samples from each study area to enable rarefaction curve analysis.  There is excellent, inexpensive, and easily usable software to apply to the analysis.  This is EstimateS.  I recommend it very strongly.  Easy to use, can dump Excel or flat data files straight in, and 95% confidence bounds are calculated.  The fundamental rationale is that a large number of random draws are made upon the grouped data for each comparative study site.  When the ESPP curve becomes asymptotic at X species, you can determine a Y number of pooled specimens that provides a solid estimate of species richness at that group sample size - for comparison with other pooled samples from other sites.  You can plot the 95%CIs around the curves, evaluate for overlap.  If not overlap at the selected Y number of specimens, then the two sites are significantly different.   There are other softwares out there to do the same thing - but none is so easy to use.

  • Giovanni Gaglianone added an answer:
    Is there any publication on scientific sampling by skin diving?

    Recently, I collected qualitative samples of marine soft-bottom zoobenthic communities at 10-15 meters depth by skin diving. I used hand-operated corers of 8cm diameter. I wonder whether there is any publication/report/manual on sampling procedures by skin diving.

    Giovanni Gaglianone · Sapienza University of Rome

    Hi Ferruccio,
    only some consideration: in my scientific diver courses and in related technical documentation (ISSD, AIOSS, European Scientific Diving Panel) I have never read about skin diving scientific sampling methods, probably because the limited time available in this type of reconnaissance does not allow any particular activity for the more (as envy Pellizzari, Genoni & Co.  :)  !!!). On the contrary, it’s obvious, time limitation often do not allow you to use many of SCUBA techniques.
    Try to ask Professor Cinelli, an institution in scientific diving (!), or, to name some researchers and colleagues which you know very well, very often in water (lucky men!): M. Abbiati, S. Acunto, C.N. Bianchi, M. Ponti, that with their experience, could help you more than me, I’m sure!

    Regards
    Giovanni

  • Claire Wordley added an answer:
    Can we calculate Convex Hull volumes with categorical data?
    I am calculating Convex Hulls for high-dimensional trait data for a set of communities (Functional Richness) to understand how species pack and fill trait space. I was wondering if these calculations can be done using categorical trait data or are the analyses affected by not having a matrix of continuous values? Is there a way to circumvent this issue?
    Claire Wordley · University of Leeds

    I also managed this using PCoA on Gower distances as suggested by http://villeger.sebastien.free.fr/ , it worked well. 

  • Madhukar Baburao Deshmukh added an answer:
    Which are the best methods to remove termites?

    Hi all,

    We have been working with a termite species from the genus Odontotermes. We'd like to permanently remove termites from some mounds to observe their potential cascading ecosystem effects. Has anyone tried to do this?

    It seems like one option to remove termites would be with insecticides, but we're worried this effect would only be temporary and termites may recolonize. One thing we've seen is people using plaster of Paris as a way to study mound architecture. Do you think we might be able to use plaster to permanently "plug" termite mounds? Anyone have any experience with these methods?

    Madhukar Baburao Deshmukh · Shivaji University, Kolhapur

    To remove termites you can use organophosphorus pesticide in the form of  chloropyriphos spray or Mix. chloropyriphos formulation with soil or infected area.

  • Marcus Fritze added an answer:
    Can bat population reduction due to White-nose Disease or other factors be linked to changes in guano communities that rely on bats for nutrients?

    Besides our concern over bat populations for their own distinctiveness and inherent value, we must recognize that bats support unique communities of cave life through their guano deposition.  Declines in bat populations due to new stresses, including White-nose disease, would likely result in loss of biodiversity and/or abundance of life in cave environments.  Is anyone looking into this directly?  Can anyone suggest new study sites or approaches to test this in future research?

    Marcus Fritze · Landkreis Mansfeld-Südharz

    Welcome! :)

  • Paula Meli added an answer:
    I'm looking for a "plant trait similarity index", any suggestions?
    I would like to test how dissimilar are some traits of an intruduced species with respect to an established community.
  • Rocco Labadessa added an answer:
    How can I quantify the edge effect on plant communities?

    Values of plant species cover have been sampled at an increasing distance from the edge of a grassland patch.

    I was thinking about methods enabling to quantify the community change along such a gradient. What would you suggest?

    In order to compare different edge types, is there any specific measure for the magnitude of the edge effect? 

    Have you ever addressed this issue or could you recommend publications in this field?

    Rocco Labadessa

    Dear, thank you all for your replies.

    I wish to specially thank Audrey and Andy for their thorough considerations and useful suggestions...the discussion is getting even more intriguing.

    This also leads me to hope for a cooperative research.

    rocco

  • Nathalie Niquil added an answer:
    Is it possible to do a Fuzzy Correspondence Analysis (FCA) under constraint, like a CCA (Canonical Correspondance Analysis)?

    Hello, we are working on biological traits analysis with fuzzy coding and would like to make the link with abiotic conditions.

    How do you do it?

    Nathalie Niquil · French National Centre for Scientific Research

    Thank you for your answers !

  • Mrigakhi Borah added an answer:
    How many days are required by Cyclosia sp. moth to complete its life cycle?
    Especially the caterpillar stage remains for how many days, can anybody tell me?
    Mrigakhi Borah · Tezpur University

    That means it depends on the climatic condition of the area.

  • Thiago Gonçalves-Souza added an answer:
    Does anybody know if it is always necessary to use a p adjustment for Fourth Corner Analysis?

    In the exploratory analysis of my data, I see a clear pattern of relationships between certain environmental variables and species traits. When I carry out a fourth corner analysis it points out to those relationships, but with the p adjustments the significance is lost. 

    Thiago Gonçalves-Souza · Universidade Federal Rural de Pernambuco

    Sent.

  • Dorothy Bullecer added an answer:
    If higher stability entails higher diversity, how come there is low diversity in climax communities?
    Climax communities are said to be in a state of equilibrium because organisms have already adapted to their environment and succession is no longer taking place. Therefore, it can be assumed that it is stable. If climax communities have high levels of stability, why is it low in diversity?
    Dorothy Bullecer · Ateneo de Manila University

    Hi, Mikee!

    Higher stability doesn't necessarily entail higher diversity. In fact, it is those communities with intermediate levels of stability that have the highest diversity.

    A community is known to be stable when there is no apparent change in the number of species and population size over a long period of time. It is then important to note that a community's stability is prevented by periodic or stochastic disturbances that give way to recolonization. It is the climax community that is most stable since the species that comprise it, which are the dominant late successional species, are least affected by gradual changes in the physical environment unlike the communities with lower stability. This high stability in climax communities would lead to a low species diversity since the time between disturbances is long, allowing dominance by one or a few number of species that, in turn, competitively exclude other species. It is the communities with intermediate levels of stability that are most diverse since the interval between disturbances are long enough for a wide variety of species to colonize and become established but are disturbed before successional replacements result in dominance and competitive exclusion.

  • Giovanni Zurlini added an answer:
    What is the best diversity metric in community ecology--species richness, Simpson's index, Shannon's index, or another metric?
    There are many metrics for measuring biodiversity in community ecology. It seems most diversity metrics are based on the spatially nested hierarchical organization of regional biotas. I am wanting your opinions about what the best metric is for measuring community diversity and comparing such patterns across scales. There are probably many squibbles about this, and some people might for example say that Shannon's index is irrelevant and shouldn't be reported. What do you think?
    Giovanni Zurlini · Università del Salento

    Dear Francesco, but once you get  the "True" diversity and decompose it into its alpha, beta and gamma components what are you going to do with it?  I am really curious to know.

  • Philip Phil-Eze added an answer:
    Does anyone have experience using the Shannon Wiener Diversity Index Score?

     I just completed the shannon Wiener diversity index and calculated a score of (H)=2.154890613. The values range from 0 to 5, with common ranges usually between 1.5 to 3.5. Can I really say that the population is diverse? What other index should I use when getting a score like this? Thanks

    Philip Phil-Eze · University of Nigeria

    The diversity index is a dimesionless value. On the face of it, one can say whether diversity is high, i.e tending towards the upper limit of 5 or diversity is low, i.e. tending towards the lowest level of 0. However, it is important to relate diversity with the taxa under study, the abundance of population of individual species and the eveness of the distribution. Simple interpretation of Shannon Weiner diversity index as high or low is too elementary an analysis. refer to the references from Reza.

About Community Ecology

In ecology, a community is an assemblage of two or more populations of different species occupying the same geographical area.

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